Table of Contents Author Guidelines Submit a Manuscript
Oxidative Medicine and Cellular Longevity
Volume 2016, Article ID 8386362, 26 pages
http://dx.doi.org/10.1155/2016/8386362
Review Article

Chlorinated Phospholipids and Fatty Acids: (Patho)physiological Relevance, Potential Toxicity, and Analysis of Lipid Chlorohydrins

Institute for Medical Physics and Biophysics, Faculty of Medicine, Leipzig University, Leipzig, Germany

Received 5 September 2016; Revised 24 October 2016; Accepted 6 November 2016

Academic Editor: Kota V. Ramana

Copyright © 2016 Jenny Schröter and Jürgen Schiller. This is an open access article distributed under the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.

Abstract

Chlorinated phospholipids are formed by the reaction of hypochlorous acid (HOCl), generated by the enzyme myeloperoxidase under inflammatory conditions, and the unsaturated fatty acyl residues or the head group. In the first case the generated chlorohydrins are both proinflammatory and cytotoxic, thus having a significant impact on the structures of biomembranes. The latter case leads to chloramines, the properties of which are by far less well understood. Since HOCl is also widely used as a disinfecting and antibacterial agent in medicinal, industrial, and domestic applications, it may represent an additional source of danger in the case of abuse or mishandling. This review discusses the reaction behavior of in vivo generated HOCl and biomolecules like DNA, proteins, and carbohydrates but will focus on phospholipids. Not only the beneficial and pathological (toxic) effects of chlorinated lipids but also the importance of these chlorinated species is discussed. Some selected cleavage products of (chlorinated) phospholipids and plasmalogens such as lysophospholipids, (chlorinated) free fatty acids and α-chloro fatty aldehydes, which are all well known to massively contribute to inflammatory diseases associated with oxidative stress, will be also discussed. Finally, common analytical methods to study these compounds will be reviewed with focus on mass spectrometric techniques.

1. Introduction

Inflammation, as an adaptive response to noxious stimuli such as infection or tissue injury, is an important and complex physiological process mediated by the immune system [1]. In general, a homeostatically controlled inflammatory response is a beneficial “weapon” of the organism to “fight” against infections and infiltrating microorganisms such as bacteria, but a tissue malfunction or homeostatic imbalance in favor of proinflammatory mediators can become very harmful to mammals due to the permanent stimulation of immune cells such as granulocytes or macrophages. A dysregulated immune response may lead, for instance, to tissue degeneration as observed in the loss of cartilage during rheumatoid arthritis [2]. Neutrophilic granulocytes (a crucial cellular part of the immune system) activated during chronic inflammation generate not only proteolytic enzymes and antibacterial proteins but also considerable amounts of reactive oxygen and nitrogen species (ROS, RNS) including both nonradical species (hypochlorous acid (HOCl) and peroxynitrite (ONOO)) and different free radicals, which are, transient compounds with at least one unpaired electron (superoxide anion (), nitric oxide ()) [3]. It is important to note that common atmospheric oxygen (“triplet oxygen”, O2) already represents a diradical (-) where the spins of the valence electrons are in parallel orientation. This 3Σg state is rather stable and explains why oxygen undergoes reactions only at elevated temperatures or under enzyme catalysis. This behavior changes significantly if singlet oxygen is considered: in this state (1Σg) oxygen is much more reactive due to the antiparallel orientation of the valence electrons. A more detailed discussion of these aspects is, however, beyond the scope of this paper. Although oxygen is needed by all aerobic organisms, its concentration has to be tightly regulated: the replacement of atmospheric air by pure (100%) O2 would be strongly toxic for living organisms. Animals used for experimental purposes die after a few days in a pure oxygen atmosphere as a result of excessive oxidation reactions, which cannot be compensated by the organism. It has also been shown that the tumor incidence increases if the oxygen partial pressure in the air exceeds only slightly the standard value of about 21% [4].

1.1. Generation of HOCl and Other Reactive Oxygen Species

O2 is converted by a number of different enzyme-triggered reactions into even more reactive compounds. In the first step, O2 is converted into superoxide (HOO), which exists at physiological pH primarily in the form of the deprotonated superoxide anion radical (). These radicals dismutate either spontaneously or particularly in the presence of the enzyme superoxide dismutase (SOD) into hydrogen peroxide (H2O2). The enzyme myeloperoxidase (MPO) converts H2O2 and chloride ions into HOCl, a highly reactive chlorine species (RCS) reacting with the majority of biologically relevant compounds.

HOCl (including its salt sodium hypochlorite (NaOCl)) as a molecular (2-electron) agent has a strong oxidizing and chlorinating ability to ensure high bactericidal and cytotoxic properties. This makes HOCl one of the most powerful in vivo oxidants. Accordingly, HOCl is also used as bleaching, disinfecting, and antiseptic agent for medicinal, industrial, and domestic applications [5]. Normally, the commercially available hypochlorite solution is more stable and much less reactive than the free acid (HOCl). However, both species are (due to the pK value of about 7.53) nearly equally concentrated at physiological pH (7.4). This implies that typical household cleaners (such as “Chlorix”) can be as harmful as the in vivo generated HOCl in the case of abuse or mishandling [6]: damages of virtually all relevant biomolecules as well as many tissues may be induced [7]. Some of these generated so-called disinfection by-products show evidence for their cytotoxic, genotoxic, teratogenic, and carcinogenic potential and this important aspect was recently reviewed [810]. Some typical pathological and toxic adverse effects in the case of abuse or mishandling of industrial or medicinal used HOCl are summarized in Table 1 and clearly indicate the sensitivity of health tissues to oxidative stress.

Table 1: Potential adverse effects in case of abuse or mishandling of industrial/medicinal used HOCl solution.
1.2. Reactivity of HOCl with Lipids

In contrast to free radicals such as hydroxyl radicals () and nitric oxide (), HOCl is characterized by a more selective reaction behavior. We will discuss the HOCl-induced changes of lipids [11] focusing on the phospholipids (PLs) shown in Figure 1.

Figure 1: Selected glycerophospholipids (PLs) which will be relevant for this review. Note that phosphatidylcholine (PC) and ethanolamine (PE) are zwitterionic lipids, while PS is an example of a negatively charged PL. PLs in biological samples often contain a saturated fatty acyl residue in sn-1 position, while that in sn-2 position is normally unsaturated. Ether PL are characterized either by an alkenyl or alkyl linkage in sn-1 position at the glycerol backbone. Alkenyl ether lipids are often called “plasmalogens.”

The majority of PLs consist of a glycerol backbone, esterified with two varying organic fatty acids and one molecule of phosphoric acid. The resulting phosphatidic acid (PA) is again able, via ester condensation with different alcohols, to form a large variety of PL species like phosphatidylcholine (PC) and phosphatidylethanolamine (PE) as neutral but zwitterionic representatives or phosphatidylserine (PS) as a typical example of a negatively charged PL. There are also ether PLs: the most important ones are the “plasmalogens” (often from PC and PE species) which possess a vinyl ether in the sn-1 position and can be formally considered as the reaction products of a fatty aldehyde with a hydroxyl group of the glycerol.

According to the high amount of PLs in biological membranes, they are important targets for peroxidation by free radicals or oxidation/chlorination by enzymatically generated agents. Those PLs, especially, containing highly unsaturated fatty acyl residues (particularly arachidonic acid), vinyl ether linkages, and/or reactive polar head groups (as in PE or PS) are most vulnerable to oxidation processes [12]. It is generally accepted that oxidized/chlorinated PLs exhibit significant effects in acute and chronic inflammation [13] and are thus associated with inflammatory diseases such as rheumatoid arthritis, neurodegenerative diseases, atherosclerosis, diabetes, systemic lupus erythematosus, and lung infections (Figure 2) [7, 14].

Figure 2: Summary of the known pathological effects mediated by oxidized or halogenated PLs (left) and of the inflammatory diseases in which these lipids are involved (right).

Since oxidized PLs exist in a tremendous diversity in biological samples, their detection in crude mixtures is still challenging. To overcome this problem, many different analytical approaches, in particular mass spectrometry (MS) based methods, were developed in the last decades and can now be considered as the most powerful tools in the field of “lipidomics.” “Lipidomics” is a relatively new “omics” approach which focuses on the identification of key species in the lipid metabolism, lipid biomarkers, and lipid signaling alterations in both health and disease [15]. This aspect will be discussed later in this review. However, it has to be emphasized already here that some lipid oxidation products represent transient compounds which either decay into other (more stable) products or react with other biomolecules, which makes the analysis of (at least) some lipid oxidation products a challenging task. Furthermore, the oxidation/chlorination of free fatty acids (FFAs) and especially polyunsaturated fatty acids (PUFAs) by ROS leads also to an enormous pool of bioactive lipid mediators. The most important and intensively investigated classes are the eicosanoid mediators, which are involved in different biological processes such as bone metabolism, nerve development, wound healing, immune responses, and inflammation [16]. However, FFAs represent detergents and are known to destabilize membranes if they are present in elevated amounts [17]. Since they are known as low abundant transient products with a limited stability, the analysis of oxidized/chlorinated FFAs is even more difficult than the investigation of oxidatively modified PLs [16]. Briefly, the search for new lipid and FFA biomarkers containing oxidized moieties in order to diagnose inflammatory processes at an early stage of disease is only realizable with highly specific and particularly sensitive analytical methods which need to be continuously improved.

In this review, we will focus on the PL and FFA oxidation/chlorination by selected agents with the emphasis on HOCl. Some selected products of PC and PE are illustrated in Figure 3.

Figure 3: Survey of selected products if an unsaturated PL either with a reactive headgroup (PE, (a)) or with an inert headgroup (PC, (b)) reacts with hypochlorous acid (HOCl). Note the complexity of the reactions and product patterns even if only a single PL is oxidized by HOCl.

We will summarize (i) the potential beneficial properties of HOCl and its chlorinated products (particularly chlorohydrins), (ii) the performed in vitro studies which were particularly aimed to find new biomarkers, and (iii) the predominantly reported negative properties of chlorohydrins and other chlorinated species leading to inflammatory diseases. In the last chapter we will provide an overview of the currently used analytical methods to characterize the oxidized/chlorinated products after PL and FFA treatment with HOCl, focusing on MS methods.

2. In Vivo Generation of HOCl by the MPO-H2O2 System

2.1. Release of the MPO-H2O2 System by Neutrophils

Neutrophilic granulocytes, which are one subtype of the polymorphonuclear leukocytes (PMNs), are known to play a major role during inflammatory processes. Three types of neutrophilic granules are consecutively generated during the maturation process of the cells: primary (azurophilic), secondary (specific), and tertiary (gelatinase) granules that contain the proinflammatory proteins MPO, lactoferrin, and metalloproteinase 9 (which comprises actually different proteins), respectively [18]. In healthy individuals the release of neutrophils from bone marrow is tightly regulated and known to eliminate pathogens either intra- or extracellularly via phagocytosis or the release of neutrophil extracellular traps (NETs) [19].

Since the total MPO concentration is about 5% of the whole neutrophil proteins [20], it is one of the major physiologically occurring components in these phagocytes and even increases massively during inflammatory processes. Thus, it is a widely studied enzyme in the fields of inflammation as well as oxidative stress and is often used as a biomarker for many diseases including atherosclerosis, rheumatoid arthritis, and neurodegenerative diseases [21]. The most common diseases linked with the MPO system are summarized in Table 2 and include the changes of the MPO concentration or activity, the investigated matrix, and finally the method by which the MPO amount and/or its activity was determined. For further details see the references provided in Table 2.

Table 2: Survey of selected diseases where myeloperoxidase (MPO) presumably represents a suitable “biomarker.” The alterations of MPO concentration and/or activity are emphasized.

During chronic infectious and inflammatory diseases the increased numbers of neutrophils permanently release not only MPO but also ROS during the “respiratory burst” that is triggered by the enzyme NADPH oxidase [22]. This may result, particularly in chronic inflammation, in both immunopathological processes and secondary damages in living organisms [23].

Since rheumatoid arthritis is a widespread disease with an annual incidence of 25–50/100 000 and a prevalence of 0.5–1.0% in North America and Europe [24] and has, even more, a high socioeconomic weight, it is mandatory to find early stage biomarkers to enable early treatment of the disease. The evaluation of the processes of cartilage degradation during inflammatory joint diseases is also a major research topic in our laboratory. Figure 4 shows, exemplarily for all inflammatory processes, the release of ROS (HOCl, H2O2, ) as well as antimicrobial enzymes (e.g., MPO, elastase, lysozyme) by an activated neutrophil that infiltrated into the joint space during acute joint inflammation [25]. Symptoms of rheumatoid arthritis may have periods of remission in which the symptoms disappear, alternating with periods of flare-ups, which is correlated with the extent of inflammation.

Figure 4: Overview of the released reactive oxygen species (ROS) and antimicrobial enzymes by an activated neutrophil during the inflammatory process in an inflamed joint. Due to the release of highly toxic ROS, most of them (including HOCl) do not discriminate between microbial and “healthy” targets, leading to an uncontrolled oxidation of all biomolecules and a persistent inflammation (reprinted from Schiller et al. [25], with permission from Elsevier).

These cartilage damaging agents do not discriminate between microbial and host target molecules and will thus oxidize a large number of biologically healthy targets such as cells, proteins, or polysaccharides leading to a persistent inflammation. For a detailed description of neutrophilic activity in immune response and inflammation see also [19, 26, 27]. Furthermore, a detailed review about the physiological properties of ROS and their regulatory enzymes has recently been published by Zuo and coworkers [28].

2.2. HOCl Generation during the “Chlorination” Cycle

As a member of the heme peroxidase family in myeloid cells, MPO becomes oxidized at the -ion position by H2O2 under the formation of a short-lived intermediate, compound I, with a radical cation center [29, 30]. Afterwards, compound I is regenerated to the ferric state (three-valent) of MPO, either in two consecutive 1-electron steps (via compound II) or by oxidizing Cl to HOCl (second order rate constant:  M−1s−1 [31]) during the chlorination cycle (Figure 5). Further details are available in a detailed review by Arnhold and Flemmig [32].

Figure 5: Generation of HOCl by MPO via a chlorination cycle. In the first step, MPO is oxidized by hydrogen peroxide (H2O2) into the short-lived compound I that contains a radical cation center. Compound I is further regenerated to the educt, the ferric state MPO, either by two consecutive 1-electron steps via compound II or by oxidizing Cl to HOCl (modified in accordance with [33]).

It is nearly impossible to determine the HOCl concentration under in vivo conditions, as HOCl is continuously generated by MPO (at least if H2O2 and Cl are present in sufficient amounts) but instantaneously consumed by its reaction with potential target molecules. Therefore, the stationary HOCl concentration is close to zero. However, there are also some papers available which provide dedicated HOCl amounts. Since HOCl is known from these reports to be highly abundant under inflammatory conditions (50–100 mM) [34] and even under physiological conditions (0.34 mM) in the extracellular space [35], it was assumed for many years that it is the only physiologically relevant halogenated product of MPO [36]. Nowadays, it is well accepted that MPO generates, even under physiological conditions, also hypobromous acid (HOBr) and hypothiocyanite (HOSCN), even if the corresponding bromide (20–100 μM) and thiocyanate (20–120 μM) concentrations are much lower than the chloride (100–140 μM) plasma concentrations [31]. Moreover, even cyanate/isocyanate, which are particularly important in human saliva [37], can be generated by MPO, however, to a minor extent [6, 38].

For example, Senthilmohan and Kettle [6] suggested HOBr could be an in vivo relevant major product of MPO at physiological conditions (second order rate constant:  M−1 s−1 [31]) and should be considered if investigations of inflammatory processes are performed. This is surprising, because Br is about three orders of magnitude less abundant in comparison to Cl (about 10−1 versus 10−4 M) and implies that bromide is preferentially metabolized by MPO. Furthermore, HOBr can be generated indirectly by the reaction between HOCl and bromide [39] which is also used to synthesize HOBr in the laboratory:Both HOCl and HOBr are strongly oxidizing agents with the ability to modify amino moieties in proteins, DNA or PLs (such as PE and PS) resulting in the generation of chloramines and bromamines as primary products [21].

Although a detailed discussion of these aspects is beyond the scope of our review, there are nowadays increasing indications that HOSCN (in particular compared to HOCl) may have protective effects in the organism: HOSCN shows a marked preference for thiol residues, forming products (particularly long-lived sulfenyl thiocyanate (RS-SCN)) that can be “repaired” by the organism [40], resulting in reversible cellular damage. Since HOCl (or HOBr) may react with SCN to generate HOSCN (second order rate constant:  M−1 s−1) [41] this reaction (2) may represent an important way of how the organism gets rid of excessive HOCl (HOBr)There is still significant interest in HOCl, since it is a specific product of MPO, whereas HOBr is additionally (or even preferentially) produced by the enzyme eosinophilic peroxidase (EPO) [11]. Due to its high toxicity, HOCl released by neutrophils into the phagosome seems to have a high impact in fighting against microbial pathogens and controlling the bacterial population in the host [42]. However, the impaired homeostasis between oxidants and antioxidants, in favor of ROS production, leads to an uncontrolled generation of HOCl, which is associated with chronic inflammatory diseases (Figure 2), may have carcinogenic and mutagenic potential [43], and is even known as a stable but highly reactive neurotoxic oxidant in the brain, where HOCl reacts rapidly with H2O2, or nitrite generating 1O2, , or nitryl chloride (NO2Cl) that may contribute to extensive tissue damage [44]. Due to its fast homeostatic consumption, in vivo generated HOCl cannot be measured directly, but either as stable scavenger products or via the determination of the MPO activity in the corresponding body fluid, for instance, by using the well-known conversion of guaiacol into tetrahydroguaiacol [45]. Therefore, different methods were established to measure stable HOCl-induced products, often by absorbance or luminescence methods, but increasingly also by MS [46]. The optimum biomarker for HOCl should be specific, stable, and sensitive to determine [47]. However, due to the fast turnover of HOCl, it is still a challenge to find a biomarker that combines all these properties.

2.3. Survey of MPO Activity by HOCl Determination

Although HOCl is known to chlorinate a variety of different biomolecules, amino acids are the most susceptible targets for chlorination by HOCl. The concentration of 3-chlorotyrosine (and to a minor extent 3,5-dichlorotyrosine) is often considered as the biomarker of choice for the MPO activity in vivo by different MS methods [48], because it is highly specific, comparably stable, and its concentration correlates with the MPO activity [4951]. Nevertheless, 3-chlorotyrosine is, first, only a minor product of the protein chlorination by HOCl and, second, it is only an intermediate in biological systems [52]. Since 3-chlorotyrosine reflects only a small percentage of the absolutely released HOCl, its function as a specific MPO activity biomarker is assumed to be limited [53].

The second well studied component in MPO activity studies is taurine (2-aminoethanesulfonic acid), because it is highly abundant in neutrophils with a concentration of about 22 mM [54]. Combined with HOCl, taurine serves as a system to study its fast chlorination by hypochlorite, leading to the stable oxidation product taurine chloramine (Figure 6) that can be conveniently measured via enzyme-linked immunosorbent assay (ELISA) [55]. Taurine chloramine is of low toxicity and reasonable stability and possesses both anti-inflammatory and antimicrobial properties. Its role in acute inflammatory processes is not yet fully understood but has been comprehensively discussed by Marcinkiewicz and Kontny [56].

Figure 6: Reaction of taurine, a very important organic (sulfonic) acid which is highly abundant in neutrophils, and HOCl leading to the comparably stable oxidation/chlorination product taurine chloramine, which is used as a marker for the HOCl production rate by MPO and can be easily determined by the taurine chloramine assay. For further details about the assay, see [47].

Smaller amounts of HOCl can be determined by using dyes such as 5-thio-2-nitrobenzoic acid (TNB) and 3,3′,5,5′-tetramethylbenzidine (TMB). Using TMB, taurine chloramine is treated with iodide leading to the formation of ICl which is instantly hydrolyzed to hypoiodous acid (HOI). TMB may be used afterwards directly as the chromophore, because it is readily oxidized by HOI to a strongly absorbing blue product [57] that allows the determination of μM quantities of HOCl.

In addition to the TNB and TMB assays, the NAD(P)H assay, the ascorbate assay, and the hydrogen peroxide consumption can also be used to determine the HOCl generation by MPO. These methods were reviewed by Kettle et al. only recently in 2014 [47]. Other potential biomarkers for the MPO/HOCl chlorinating system are either plasmalogens (which will be discussed in more detail later) or glutathione (γ-L-glutamyl-L-cysteinyl-glycin), which result in unsaturated (lyso)PLs and α-chloro aldehydes or glutathione sulfonamide, respectively. These compounds are easily detectable by MS methods which will be shortly discussed at the end of this paper [58, 59].

3. Reactivity of In Vivo Generated HOCl

Due to the fact that the generated HOCl is directly consumed by its reaction with abundant biomolecules, there is increasing evidence that the distribution of HOCl is not homogeneous: MPO is a strongly cationic (positively charged) protein and will therefore be particularly located close to negatively charged compounds, either negatively charged proteins and carbohydrates such as heparin [60], or negatively charged PLs, particularly PS [61], which is almost completely located in the inner leaflet of a membrane, at least in living, nonapoptotic cells. This suggests that MPO binds to apoptotic cells, which leads to an inhomogeneous distribution of HOCl within tissues.

3.1. Generation of Biomolecular Radicals

As it is produced in large quantities and represents a reactive two-electron oxidizing agent in human beings under inflammatory conditions, HOCl is several orders of magnitude more reactive than other oxidants like H2O2, (lipid) hydroperoxides, or peroxynitrite [62]. High reactivity normally goes along with nonselectivity. Therefore, HOCl affects not only infiltrated microorganisms, but also “normal” intracellular enzymes, nucleotides, carbohydrates, or lipids in the body with the capacity to change membrane compositions [63]. Nevertheless, HOCl is also a specific oxidizing/halogenating agent that discriminates between different functional groups and reacts normally in the following order: reduced sulfur moieties (thiols and thioethers) > primary and secondary amines > phenols, tertiary amines > double bonds, other aromatics, carbonyls and amides [64]. A survey of calculated and/or experimentally determined second order rate constants () are available in [65].

HOCl has the ability to generate free radicals and stable cleavage products by its reaction with small inorganic molecules or functional groups of biomolecules such as proteins, lipids, nucleotides, and carbohydrates. Figure 7 shows some selected examples for the generation of radicals from biomolecules after treatment with HOCl.

Figure 7: Overview of generated radical species by the reaction of HOCl and different biomolecules. The HOCl-induced chlorination of free amino acids (a, [66]), proteins (b, [66]), nucleosides (c, [67]), glycosaminoglycans (d, [68]), and PLs (e, [69]) leads in various consecutive reactions (implied by three arrows) to different radical species which may cause oxidative stress and favor the development of many diseases.
3.1.1. Amino Acids and Proteins

Free amino acids can be affected by HOCl in a concentration-dependent reaction at either the sulfur or the amino group in the side chain or the α-amino group of amino acids, the reaction at the sulfhydryl group being the preferred one: previous investigations provided evidence that the amino groups are not affected at all until all sulfhydryl residues have reacted [70]. The chlorination by HOCl at the α-amino group results in transient amino acid chloramines (AACLs), which are known to induce further reactions more selectively than free HOCl. Therefore, AACLs are potential secondary mediators of HOCl-induced injuries [71]. As the most abundant free amino acid (however, not in the strict classical sense, as -COOH is replaced by -SO3H in taurine), taurine chloramine (Figure 6) is one of the most important products of amino acid chlorination in human PMNs and was already shortly described in the chapter before. In general, AACLs seem to affect biological targets such as cytoplasmic molecules or glutathione and mediate the HOCl-related toxicity leading to apoptotic cell death [72]. Even without any further oxidative reactions, α-amino group AACLs decompose in the presence of water under formation of the corresponding aldehydes [50] or generate, via a one electron pathway, also N-centered radicals (Figure 7(a)), which are quickly converted into C-centered radicals by different mechanisms, for instance, inter- or intramolecular transport of a proton or decarboxylation [66]. These AACLs decompose to free radicals, which are known to be cytotoxic for tissues and organs [33] and the organism has to try to keep their concentration limited by increased degradation and/or the uptake of antioxidants. It was also shown that HOCl reacts with the same functional groups in proteins as in the case of free amino acids, but these reactions are normally somewhat slower, presumably due to the increased viscosity of protein solutions [73].

Due to their high physiological concentrations in cells, plasma, and most tissues, proteins are actually the most relevant targets for in vivo modification by HOCl and other oxidants causing numerous posttranslational modifications such as the oxidation of sulfhydryl groups and the chlorination of aromatic side chains or the chlorination of amino groups in the side chains and some other side reactions [42]. It is assumed that HOCl primarily affects more readily the functional groups in the side chains of proteins than in the peptide linkages [74]. The side chain chlorination comprises aggregation, oligomerization, destabilization, fragmentation, and/or degradation steps [42] after the formation of an N-centered radical which is further converted to a C-centered radical (Figure 7(b)) often catalyzed by transition metal ions (e.g., Cu+) [66]. Cysteine and methionine (sulfur-containing amino acids) are characterized by an about 100-fold higher reactivity with HOCl than any other functional group of proteins or other biomolecules. The HOCl-initiated chlorination of cysteine leads to labile sulfenyl chloride (R-S-Cl) and sulfenic acid (R-S-OH) intermediates, which are both known to undergo further oxidation steps with HOCl [75]. These irreversible modifications result in sulfinic (R-SO2H) or sulfonic (R-SO3H) acids as well as thiosulfinate products (R-S-SO-R2), the formation of which is accompanied by protein decomposition [5]. Methionine is almost as readily affected as cysteine and may either generate (under in vivo conditions) the reversible methionine sulfoxide or the irreversible dehydromethionine [76]. Beside sulfur-containing amino acids, the amino groups in lysine, histidine, and arginine are also preferred targets for HOCl. Although the reaction rates are reduced in comparison to cysteine, the majority of reaction products are generated irreversibly in vivo and are thus prone to further reactions with other potential reactive protein sites and/or other biomolecules [74].

3.1.2. Nucleic Acids and DNA

The HOCl-induced oxidation of nucleic acids in a DNA strand normally affects the nitrogenous base either at the primary nitrogen (“exocyclic”) in adenosine, guanosine, or cytosine or at the secondary nitrogen (“endocyclic”) in guanosine, uridine, or thymidine, the reaction at the endocyclic nitrogen seemingly being preferred [11]. These N-chlorinated products are intermediates and subsequently converted into more stable chlorinated products such as 5-chlorocytosine, 5-chlorouracil, 5-chloro-(2′-deoxy)-cytidine, 8-chloroadenine, 8-chloro-(2′-deoxy)adenosine, and 8-chloro-(2′-deoxy)guanosine [77, 78]. Using electron paramagnetic resonance (EPR) in combination with spin trapping to enhance the lifetime of the radicals of interest, the generation of N-centered radicals of nucleosides (Figure 7(c)) from transient chloramines could be monitored by disrupting the double-stranded DNA [67]. The tendency of radical formation of isolated nucleosides as well as polynucleotides can be sorted as follows: cytosine > adenosine > guanosine > thymidine [67, 79]. Some of these products were determined both in inflammation-related cell cultures and in inflamed tissues and are known to cause the dissociation of the double-stranded DNA (cleavage of the hydrogen bonds) and are therefore potential biomarkers of early inflammatory processes [80]. It is known that the concentrations of chlorinated nucleosides (5-chlorouracil) are elevated in the inflammatory exudate of humans and rats as well as in atherosclerotic plaques (AP) [55]. Moreover, there is evidence for the cytotoxic and mutagenic potential of chlorinated nucleic acids or chlorinated DNA moieties (e.g., [77, 8184]). These cytotoxic effects (i.e., frameshift mutations or base pair substitutions) can be caused by both lipid peroxidation products and HOCl-mediated protein-DNA crosslinks. Under neuropathological conditions, HOCl is continuously released from PMNs or microglia to diffuse into the brain parenchyma and maintains chlorinative stress resulting in neurodegeneration [44]. Even if noncovalent ionic interactions of DNA and proteins are physiologically very important for normal cellular functions [85], the oxidation of covalently bound protein-DNA cross linkages leads to inadequate DNA repair [86] and to mutagenic and cytotoxic effects of phagocytes on microbial pathogens and host tissue [87].

3.1.3. Carbohydrates

Oxidized carbohydrates were investigated to a much lesser extent, presumably due to their complexity [88]. As already discussed in the context of other biomolecules, free amino groups in sugars such as glucosamine are the preferred targets for HOCl. Although the reaction between HOCl and common monosaccharides is comparably slow [89, 90], the HOCl-induced transformation of free amino groups in sugars was reported to be even faster than the modification of the N-terminal amino group of peptides [91]. Moreover, HOCl causes the generation of chloramides (R-NCl-C(O)-R2) from amide groups (R-NH-C(O)-R2) of glycosaminoglycans (GAGs) in the extracellular matrix [92]. Since hyaluronan and chondroitin sulfate regulate different cellular and tissue functions and possess an N-acetyl group in the repeating disaccharide unit, they are the most intensely investigated GAGs in the extracellular matrix [93], another reason why GAGs are intensively studied is their abundance in cartilage (chondroitin sulfate) or synovial fluid (hyaluronan), where inflammation plays a major role [88]. Due to the poor oxidizing properties of the initially generated chloramides, they are prone to reacting with different reducing agents including radicals [92] and are thus only transient products. Chloramides decompose to N-centered radicals (R--C(O)-R2) followed by C-centered radicals, leading finally to the site-specific fragmentation of the glycosidic linkages in the polysaccharide chain (Figure 7(d)) under generation of GAG oligosaccharides [68]. These reactions are stimulated by the presence of low-valent transition metals such as Fe2+ or Cu+ via a one-electron reduction of the chloramide group [68]. Since GAGs are known to be involved in important cellular functions, it is assumed that oxidatively modified GAGs may lead to altered cell migration, adhesion, proliferation, growth, and even phenotyping [33]. Finally, it is known that high mass hyaluronan has anti-inflammatory properties, while low mass hyaluronan is proinflammatory [94]. Therefore, changes of the molecular weight of hyaluronan are of major importance.

3.1.4. Phospholipids

The last important class of biomolecules that can be affected by HOCl is represented by lipids, particularly PLs. It is well known that HOCl reacts with either the double bonds of the acyl chains of unsaturated PLs or the reactive functional groups in the headgroup (e.g., the amino residues in PE and PS). Although the focus of this review is on the addition of HOCl as a nonradical (molecular) agent to the double bonds of PLs which leads to chlorohydrin generation, HOCl can also trigger the formation of N-centered radicals in PE and PS by reaction with the nitrogen in the headgroup. The first step of the amino modification by HOCl is the generation of monochloramine, which can be converted (in the presence of a sufficient excess of HOCl) into the corresponding dichloramine [95], which are both only fairly stable compounds. Using EPR with spin trapping, Kawai et al. could monitor the generation of an N-centered radical from the PE dichloramine (Figure 7(e)) [69]. Via direct or radical-mediated processes, the elimination of HCl may also occur and result in the generation of the corresponding nitrile (Equation (3)), while an aldehyde is the final product of the hydrolysis of the monochloramine (vide supra)We will not focus on these aspects here to a major extent. The reader who is particularly interested in the related reaction mechanisms and further details about free radical formation from biologically important molecules by HOCl is referred to the excellent review by Panasenko and coworkers [33]. However, it is widely accepted that the radicals derived from chloramines may induce or mediate (through, e.g., tocopherol) oxidative modifications of lipids [96].

4. Phospholipid Oxidation by HOCl

A crude survey of products which may be expected if PLs are subjected to HOCl oxidation is shown in Figure 8 [97].

Figure 8: Scheme of potential reaction products from an unsaturated PL under inflammatory conditions in vivo. Please note that the term “long-chain” products refers to compounds that have a higher mass in comparison to the native PL while “short-chain” products have a smaller mass. A similar scheme has been suggested recently [97]. Although lysophospholipids (LPLs) might be also considered as “short-chain” products, they are discussed here as a distinct lipid class. This scheme should be regarded as a very crude survey and not all compounds that play a physiological role are actually listed (reprinted from [98] with permission from Elsevier).

The most relevant PL oxidation products can be sorted into (i) full chain length products (hydroperoxides, hydroxides, and epoxides), (ii) full-chain rearranged products (isoprostanes and isofurans), and (iii) truncated products (alkanals, alkenals, and hydroxyalkenals) [99]. Although compound class (iii) is currently most intensely investigated, because aldehydes may react (under the particular generation of Schiff bases and other products) with proteins and modulate in this way the activity of enzymes [100], the compounds we will discuss here in more detail belong to group (i): no truncation of the fatty acyl residue occurs if HOCl reacts with the double bonds of PLs or FFAs under generation of chlorohydrins as addition products.

The reaction between olefinic compounds (such as unsaturated lipids) and HOCl is known for more than a hundred years, including discussions about which compounds can be considered as the stable final products: chlorohydrins, glycols [101], or epoxides [102]. Nowadays, it is commonly accepted that chlorohydrins (the addition products of HOCl to the double bond) are the most abundant products when lipids are treated with HOCl, even if there are also recent reports that dimeric products of oleic acid may be also generated [103].

Beside PLs (as shown in Figure 8) containing two fatty acyl residues, which are linked to the glycerol by ester linkages, alkenyl-acyl PLs, commonly termed “plasmalogens,” are a second class of PLs that occur in significant amounts in many biological samples, for instance, in neutrophils, macrophages, glia cells, neurons, smooth muscle cells, endothelial cells, cardiac myocytes, and particularly spermatozoa [104, 105]. These plasmalogens are generated by the reaction between glycerol and a fatty aldehyde followed by the elimination of one water molecule and are often characterized by a choline or (even more abundant) an ethanolamine headgroup [106]. Although brain and spermatozoa lipids contain considerable amounts of highly unsaturated fatty acyl residues (such as docosahexaenoic acid, 22 : 6) [107], it is nowadays commonly accepted that the alkenyl ether linkage represents a site of high reactivity with a large variety of ROS [108], much higher in comparison to the “normal” double bonds along a common fatty acyl chain [109]. Therefore, plasmalogens are often considered to represent important biological antioxidants [110]. It is important to note that the resulting plasmalogen LPCs possess an unsaturated fatty acyl residue in the sn-1 position [111], which is a remarkable difference in comparison to diacyl-PCs that possess the unsaturated fatty acyl residue normally in the sn-2 position and yields exclusively saturated LPCs upon oxidation with HOCl. Therefore, the detection of unsaturated lysophospholipids (LPLs) is normally a clear indication of the presence of plasmalogens [112].

5. Beneficial Effects of Lipid Chlorohydrins and Peroxidized Lipids

The majority of authors indicate that lipid oxidation processes and the related products exert a negative effect on the organism and that everyone should attempt to minimize the extent of lipid oxidation, for instance, by the ingestion of antioxidative compounds such as vitamins [113]. However, there are also a few indications that lipid oxidation positively affects the organism [13].

There are indications that oxidized lipids are faster digested by phospholipases (particularly phospholipase A2 (PLA2), which cleaves exclusively the fatty acyl residue in sn-2 position and plays a more prominent role than PLA1) than their native (nonoxidized) counterparts. This emphasizes that the organism recognizes oxidized lipids as “foreign” and is thus interested to get rid of these molecules as fast as possible. This increasingly important aspect has been reviewed recently [114]. Conversely, this means that PLA2 enzymes (there are many different species) affect oxidized PL more readily: for instance, it could be shown that AP are characterized by an elevated content of lysophosphatidylcholine (LPC), which is presumably generated by the action of PLA2 on PC [115]. Although there are many indications that peroxidized lipids are preferentially digested by PLA2, the detailed mechanisms behind this finding are not yet completely clear. The two potential reasons are, first, the activity of the enzyme might be actually elevated in the presence of a different substrate, because this substrate fits more readily into the active site of the enzyme, and second, the presence of oxidized lipids may also be accompanied by alterations of the lipid membrane structure and this might lead to improved digestibility [116].

Different effects in comparison to peroxidized lipids have been described for HOCl-modified lipids: halogenated PLs are inhibitory to the enzyme and elevated concentrations of chlorinated (and brominated) PC molecules decrease the activity of secretory PLA2 by about 50% [34]. This could be confirmed recently by using bee venom PLA2 and liposomes of defined lipid compositions [148]. These notable differences clearly emphasize that more detailed studies of these aspects are necessary.

In general, it is known that oxidized lipids (especially oxidized arachidonyl residues) can induce protective effects by the upregulation of antioxidant genes, inhibition of inflammatory signaling pathways through Nrf2 (nuclear factor erythroid 2-related factor 2) mechanisms [149], antagonism of Toll-like receptors [150], immunomodulating and immunosuppressive action of oxidized PLs in adaptive immunity and autoimmune disease [13], activation of PPARs (peroxisome proliferator-activated receptors) which are known for their anti-inflammatory action, and the protective action against lung edema in acute lung inflammation [151]. As implied before, plasmalogens are also known as antioxidants.

6. In Vitro Generation of Chlorohydrins (Cell and Tissue Studies)

Although many papers focus on the effects of (per)oxidized lipids on selected cell lines, the effects of chlorohydrins were studied to a much lesser extent. This might be due to the fact that PL chlorohydrins (unlike, e.g., “oxPAPC” [152]) are nowadays not commercially available. However, this purchasable “oxPAPC,” which is obtained by air oxidation of PAPC, is a relatively crude mixture and contains at least three different substance classes (hydroperoxides, aldehydes, and carboxylic acids). This makes detailed assignments about which compound is responsible for the observed effects very difficult.

In one of the first chlorohydrin-related studies, Carr and coworkers treated human erythrocytes with HOCl [153] and were able to detect the generation of chlorohydrins by means of thin-layer chromatography (TLC) and by using an ELISA assay against chlorohydrins. Since lipid chlorohydrins are more polar and bulky than their parent lipids [154], their impact on membrane stability and integrity was also investigated by measuring the release of hemoglobin from the cells. Different chlorohydrins caused different effects: the addition of HOCl-treated oleic acid to the red blood cells resulted in a rapid (concentration-dependent) lysis of the cells while the effect of cholesterol CH was less pronounced and was also dependent on the type of the CH isomer with the chlorohydrin-3 being the most deleterious one. Further analysis by Vissers and coworkers [155] examining HOCl-lysed red cell ghosts by electron microscopy demonstrated considerable disruption of the cell membrane and provided evidence for complete rupture at an HOCl concentration of about 5 mM.

The same authors [156] extended their work a few years later to another cell system: when human umbilical vein endothelial cells were treated with preformed halohydrins of oleic acid, cell detachment and necrotic death can be induced with increasing doses of the halohydrins, whereas the cells were unaffected by equivalent doses of pure oleic acid as the control. Bromohydrins (which can be obtained by the treatment of lipids with HOBr which can be conveniently generated by mixing HOCl with a small excess of NaBr) caused even more lysis than the corresponding chlorohydrins at equivalent doses, presumably because bromohydrins are more readily incorporated into the endothelial cells. It was also suggested that membrane protein modification is the reaction which is primarily responsible for HOCl-mediated cell lysis [157]. Therefore, further studies of these aspects are required.

It is important to note that chlorohydrins seem to have not only structural relevance but are also actively involved in metabolic pathways. It could be shown [158] that the cellular adenosine triphosphate (ATP) level is significantly diminished when cultured myeloid (HL60) cells are incubated for 24 h with selected chlorohydrins. These effects were additionally compared with the effects of different small aldehydes (such as 4-hydroxy-2-nonenal, HNE) which are known to be generated under inflammatory conditions by cleavage at the double bond position of unsaturated fatty acyl residues. The ATP depletion by the PL chlorohydrins was slightly less than that of HNE, but greater than that of hexanal and trans-2-nonenal, which are all well-known oxidation products of lipids. This indicates that chlorohydrins directly affect the activities of enzymes.

Robaszkiewicz and coworkers [159] studied the effects of chlorohydrin PCs on human erythrocytes. It could be shown that the biophysical properties of PL bilayers of known compositions are altered in the presence of PC chlorohydrins. In particular, changes in erythrocyte shape (echinocyte formation) and aggregation were significantly altered when vesicles containing PC-CH were mixed with the cells. Similar effects were also found [160] when HUVEC-ST (endothelial cells) were treated with PC chlorohydrins. Under these conditions there was a decrease of the mitochondrial potential and an increase in the number of apoptotic cells. These effects were accompanied by an increase in the level of active caspase-3 and caspase-7 and a decrease in glutathione content and the overall antioxidant capacity of the cells. Similar effects were observed in the case of lung epithelial cells and HOCl was found to affect the redox state of A549 cells by oxidation of GSH, inactivation of antioxidant enzymes, and the increase of ROS generation [161].

It could also be shown that induced acute pancreatitis results in a substantial release not only of FFAs but also of the chlorohydrins of both oleic and linoleic acid from adipose tissue while accompanying plasma investigations evidenced only the chlorohydrin of oleic acid. Administration of 250 μM lipid chlorohydrins, the concentration found in ascitic fluid, induces the expression of TNF-α and IL-1β in peritoneal macrophages and increases the systemic inflammatory response in pancreatitis. Finally, increased concentrations of oleic acid chlorohydrin have been found in the plasma of human patients with pancreatitis [162].

7. Chlorohydrins in Diseases

The last example indicates that there is increasing evidence that products derived from the MPO/H2O2/Cl system play a crucial role in many diseases and it can be suspected that this neutrophil-derived system is, beside inflammation mediated by T-cells, a major contributor in inflammatory diseases [163, 164]. A survey of different diseases mediated by MPO activity is given in Table 2, showing only the most important diseases due to the limited space available.

7.1. Atherosclerosis

There is increasing evidence that many diseases are accompanied by inflammation. This does not only apply for classical inflammatory diseases such as gastritis and arthritis, but also for diseases such as obesity and cancer [165]. The most important and therefore most intensively studied disease is atherosclerosis [166], which is characterized by the thickening, hardening, and loss of elasticity of the walls of arteries up to the buildup of fatty plaques in the artery walls. One probable mechanism is mediated by the so-called foam cells described by the uncontrolled uptake of cholesterol and other lipids by macrophages which is presumably triggered by oxidized lipids [167].

The first hint to the involvement of chlorinated lipid species in atherosclerosis was obtained in 1996 [168]: Hazen and coworkers detected different chlorinated lipids upon the exposition of human LDL to the complete MPO system at acidic conditions with the focus on cholesterol: beside dichlorinated cholesterol, cholesterol α-chlorohydrin (6β-chlorocholestane-(3β,5α)-diol), cholesterol β-chlorohydrin (5α-chlorocholestane-(3β, 6β)-diol), and a structurally related cholesterol chlorohydrin could be detected and characterized by MS. The authors provided additional evidence that Cl2 derived from HOCl (particularly at acidic conditions which favor the presence of the free acid HOCl) is the actual chlorinating intermediate in the oxidation of cholesterol by MPO. It was suggested that Cl2 generation in acidic compartments constitutes one important pathway for the oxidation of LDL cholesterol in the artery wall.

A few years later, the presence of lipid chlorohydrins could be unequivocally confirmed in atherosclerotic lesions and it was also found that chlorinated lipids exhibit serious effects on different cell lines which may contribute to the development of the disease. These findings suggest that PL chlorohydrins formed in HOCl-treated LDL could contribute to the proinflammatory effects observed for this modified lipoprotein in vitro [169]. An interesting experiment was performed by Yang and coworkers in 2006 [170]: they infused clamped carotid arteries with 1 mM HOCl for 1 h, before reperfusion and animal recovery for up to 2 weeks. Interestingly, the results of these studies indicate that the addition of HOCl alone can lead to neointima formation containing both VSMCs (vascular smooth muscle cell) and macrophage infiltration that is consistent with the process of atherosclerosis.

A surprising observation was made in 2008 [171]. Although it is commonly accepted that the LPC levels are elevated in sera from patients with atherosclerosis and in atherosclerotic tissues [172], these are regularly saturated LPC species, as the majority of biologically relevant PLs contain an unsaturated fatty acyl residue in the sn-2 position and LPCs are typically generated by the enzyme PLA2 which cleaves the fatty acid in the sn-2 position. The authors demonstrated for the first time that LPC-chlorohydrins are elevated over 60-fold in human atherosclerotic lesions and therefore may have unique proatherogenic properties compared to common saturated LPCs. This emphasizes the role of plasmalogens in the disease [110]. The important role of plasmalogens in AP could already be shown in 2003 by Thukkani and coworkers as they found a 1400-fold higher concentration of the α-chloro fatty aldehyde (α-ClFALD) 2-ClHDA compared to normal aorta samples [173]. Interested readers will find more information about the role of plasmalogens in atherosclerosis in a recent review by Ford [174]. It has also been hypothesized recently that the type of the generated LPC is of (patho-)physiological relevance [175], because LPC is a major constituent of oxidatively modified LDL and is generally considered to be atherogenic. However, some studies have also shown antiatherogenic properties of some LPC species [175]. These controversial findings are apparently caused by changes of the degree of saturation of the fatty acyl moiety of the LPC species. The presence of (ω)-PUFAs at the sn-1 position of LPC makes LPC anti-atherogenic [176], while the presence of saturated fatty acids renders LPC atherogenic [177]. It is important to note that LPC is not only generated by PLA2, but LPC may be considered as a general product of the decay of oxidized lipids. This aspect will be discussed in more detail below.

7.2. Arthritis

Upon acute inflammation, the synovial fluid from patients suffering from rheumatic diseases usually contains a large number of granulocytes and cell numbers of the order of about 1 × 109 cells in 30 mL synovial fluid are not exceptional [178, 179]. Since neutrophils (beside macrophages) are a rich source of the enzyme MPO, it is not surprising that synovial fluids are also characterized by significant MPO activities [120]. It is well known from investigations using classical assays such as the determination of thiobarbituric acid reactive substances, lipid hydroperoxides, or diene conjugates that the lipid compositions of synovial fluids change significantly under inflammatory conditions [180]. Although little attempts were performed to characterize the entire profile of oxidized lipids in the synovial fluids [181], it could be shown in 2005 that the LPC content correlates with the severity (inflammatory state) of the disease and even the success of a medical cure could be monitored by the decreasing LPC content [182]. In 2015 novel peptidoaldehydes from GSH and α-ClFALD in human neutrophils and a mouse model could be identified for the first time, indicating that α-ClFALD is produced as a result of MPO activity [183]. There is also increasing evidence that LPC represents just a transient compound [184]: lysophosphatidic acid (LPA) is mainly produced by the hydrolysis of LPC catalyzed by the enzyme lysophospholipase D, which is also called autotaxin (ATX). LPA interacts with specific G-protein coupled receptors and is involved in the regulation of cellular survival, proliferation, differentiation, and motility. Therefore, an elevated LPC content (mediated either by ROS or PLA2 activity) may be considered an important prerequisite of LPA generation. The inhibition of the LPA receptor has also been suggested as a promising way to suppress the symptoms of arthritis [185].

7.3. Other Diseases

There are many other diseases, for instance, multiple sclerosis, pulmonary fibrosis, liver fibrosis, and hepatitis, which are characterized by elevated LPC contents and/or enhanced MPO activities and/or enhanced lipid peroxidation product contents. These diseases have recently been reviewed and the interested reader is advised to consult [186].

8. Analysis of Chlorinated Lipids Using Different Mass Spectrometry Methods

Lipid oxidation products are classically assessed by photometric assays such as the determination of the thiobarbituric acid reactive substances (TBARS), the diene conjugates, or the number of hydroperoxides. Although these assays are simple and sensitive [187], they are not the methods of choice to determine chlorinated lipids. MS techniques using different ionization methods are much better suited for that purpose and will therefore be shortly discussed in this chapter. The HOCl-induced oxidation of plasmalogens was also investigated by MS, where plasmalogens gave even higher yields of LPC than diacyl-PCs with the same number of double bonds [109], confirming the extreme oxidation-sensitivity of plasmalogens. Since the analysis of FFA is easier in comparison to (phospho)lipids, they were formerly nearly exclusively investigated focusing on gas chromatography mass spectrometry (GC-MS) methods.

8.1. Gas Chromatography Mass Spectrometry

By using GC combined with different detection methods (i.e., ultraviolet (UV), MS, flame ionization detector (FID), or fluorescence) FFA oxidation products can be easily studied and the identification of many different products is made possible. Although GC offers an excellent resolution (even the separation of isomeric FFA is possible), only volatile organic compounds are detectable, which requires a mandatory esterification step of the FFA (often the fatty acid methyl ester, FAME) [188]. For more detailed information about sample preparation and GC-MS procedure regarding FFA analysis see also [189]. Using GC-MS, increased concentrations of fatty acid chlorohydrins were identified in adipose tissue, which emphasizes the systemic inflammatory response in acute inflammation [162]. Nevertheless, it has to be stressed that even the oxidation chemistry of simple compounds is very complex and increases with the complexity (number of double bonds) of the compound of interest. For instance, even the oxidation of isolated linoleic acid yields dozens of different products and this sheds light on the complexity of the product pattern [190].

Since PLs are nonvolatile, their direct separation and analysis with GC-MS is not possible. Therefore, the analysis of the fatty acyl composition of PL species requires a time-consuming sample preparation including the PL hydrolysis into diacylglycerols and FFA followed by their conversion into FAMEs [188]. However, there are some applications for the analysis of oxidized and chlorinated lipids using GC-MS. Due to their considerable reactivity with HOCl, plasmalogens readily generate oxidation products (i.e., α-ClFALD) and LPLs that are suitable for GC-MS analysis. α-ClFALDs are both hard to ionize and relatively unstable under ESI conditions. Thus, the conversion with pentafluorobenzyl (PFB) hydroxylamine into oximes improves the detection sensitivity by GC-MS, which is better in comparison to the achievable sensitivity of ESI MS [191]. In this study 2-chlorohexadecanal was investigated by GC negative ion chemical ionization (NICI) MS after PFB hydroxylamine derivatization of tissue and cell culture samples as an alternative method to LC-MS.

8.2. Electron Ionization Mass Spectrometry

Significant progress could be made in the last decades regarding the MS analysis of nonvolatile and/or high mass products. Until the eighties of the last century conventional electron ionization (EI) MS was nearly exclusively available. Using this approach, the sample is evaporated and subsequently ionized in the gas phase by collision with accelerated electrons, which (normally) leads to the removal of one electron from the analyte and the generation of radical cations. The most important prerequisite is sufficient volatility of the analyte. Therefore, this method can hardly be applied to lipids but is applicable to fatty acids subsequent to their conversion into methyl or trimethylsilyl esters to enhance their volatility [192].

Although the application range of EI is limited, the need to use volatile compounds enables the direct and straightforward combination of EI MS with GC. Among all chromatographic methods, GC offers the best separation quality for FFA and enables even the separation of different isomers. For instance, Winterbourn and coworkers [193] were able to show that both 9,10-chlorohydrin isomers of oleic acid can be differentiated by GC and that both isomers are generated in the same amount if oleic acid reacts with HOCl. Therefore, it can be concluded that the reaction between HOCl and unsaturated fatty acids is not regiospecific at all but results in a mixture of isomers. These authors have also suggested that the incorporation of chlorohydrins into cellular membranes leads to the destabilization of the lipid membranes, chlorohydrins, thus representing potential biomarkers. Similar data could be obtained by the same group regarding the chlorohydrins of cholesterol [194]. However, the biological significance of lipid chlorohydrins so far remains to be elucidated in more detail and there is also increasing evidence that the reaction between FFAs such as oleic acid and HOCl is even more complex than initially assumed. Recently, Schröter and colleagues [103] found that in addition to chlorohydrin as the main product of the reaction between HOCl and oleic acid dimeric and trimeric products are generated, the abundance decreasing from dimer to trimer. These oligomeric products were monitored by using high performance TLC (HPTLC), electrospray ionization (ESI), and matrix-assisted laser desorption and ionization (MALDI) MS. These oligomeric products might be derived either from the contribution of free radicals or from estolide formation [195].

8.3. Soft Ionization MS

Since the 1980s, a continuous stream of very creative papers was published in which new “soft ionization” techniques were presented enabling the MS analysis of native and oxidatively modified lipids without the need of previous saponification and derivatization. In contrast to EI, soft ionization MS enables direct detection of the molecular ion of the analyte. Typical soft ionization methods are ESI, APCI, and MALDI that enable direct analysis of native lipids and the corresponding oxidation products without the need of sample derivatization (like in GC-MS methods). In contrast to EI, the sample is not ionized by the loss of an electron but by the addition of a cation (often H+ or Na+, which are both omnipresent in biological samples) or deprotonation. Radical cations are normally not observed.

Basically, ESI and APCI are “softer” methods and can also easily be coupled to chromatographic separation methods such as High Performance Liquid Chromatography (HPLC). By contrast, MALDI is the more convenient method which tolerates a significant extent of impurities. Also, it generates almost exclusively singly charged ions, which makes MALDI spectra interpretation much easier [196].

8.3.1. MALDI-TOF MS

As early as in 2001, Arnhold and coworkers [197] were able to show that MALDI-TOF MS is a convenient method to study the effect of the reagent HOCl as well as the complete MPO/H2O2/Cl system on selected PCs with differently unsaturated fatty acyl residues. It could be shown by using polyunsaturated lipids (with arachidonoyl or docosahexaenoyl residues) that chlorohydrins and glycols are the most relevant products. The corresponding yields of these products could be influenced by varying the incubation time: monochlorohydrins and glycols dominated at short incubation times, while bischlorohydrins as well as products containing one chlorohydrin and one glycol moiety appeared after longer incubation. There was also evidence that LPC (lacking one fatty acyl residue in comparison to the native PL) is another important reaction product. This aspect was investigated one year later in more detail [198]. It turned out that the yield of LPC increases if PCs with a higher content of double bonds are oxidized by HOCl. This is due to the fact that PCs including an oleoyl residue (18 : 1) give only a small amount of LPC, while PLs with a docosahexaenoyl residue (22 : 6) result in considerable amounts of LPC. The generation of LPC under the influence of HOCl was explained by the introduction of electronegative elements (chlorine and oxygen) that withdraw electrons from the ester bond, thus enhancing its sensitivity to hydrolysis [198]. This is exemplarily shown in Figure 9. It is particularly notable that LPC may also be generated when phospholipases are completely absent.

Figure 9: Formation of LPLs and higher molecular weight products (particularly chlorohydrins) after incubation of different PCs with an excess of HOCl as evidenced by positive ion matrix-assisted laser desorption and ionization-time of flight mass spectrometry (MALDI-TOF MS): (a) PC 16 : 0/16 : 0; (b) PC 16 : 0/18 : 1; (c) PC 16 : 0/18 : 2; (d) PC 16 : 0/20 : 4; (e) PC 16 : 0/22 : 6. Please note that the yield of lysophosphatidylcholine (LPC, marked by the grey box) increases with the extent of unsaturation of the used PC (reprinted with slight modifications from Arnhold et al. [198] with permission from Elsevier).

Although this mechanism should be valid for all unsaturated lipids independent of the headgroup, the extent of LPL generation depends significantly on the structure of the used lipid: it was shown recently that the HOCl treatment of PE does not lead to LPE generation [199]. However, there is so far no convincing explanation for this surprising difference, and further studies to clarify this problem are urgently required.

In contrast to HOCl-induced lipid oxidations with LPC as the main product, hydroxyl radicals primarily cause scission at the position of the double bonds under generation of the corresponding aldehydes and/or carboxylic acids. This is a notable difference, although the detailed molecular reasons are still unknown. Finally, it has to be emphasized that a differentiation between HOCl and hydroxyl radicals under physiological conditions is still difficult: if an unsaturated PC is treated with the Fenton reagent in the presence of NaCl, the generation of chlorohydrins can be unequivocally monitored [200]. This implies that the in situ generated hydroxyl radicals react with the chloride under formation of HOCl. This might also be the reason why water radiolysis (the best characterized method of generation) may also lead to the generation of HOCl if water radiation is performed in the presence of an elevated salt content [201]. This can be easily verified in cell experiment by measuring the number of dead cells in dependence of the salt concentration at a constant γ-dose [202].

Finally, a warning is required: although MALDI is a soft ionization method, it is less soft than ESI MS. While chloramines of PE can be easily detected by ESI MS [95], this is not possible by MALDI MS, at least if standard MALDI matrices but not the optimum matrix is used [203]: 4-chloro-α-cyanocinnamic acid is the MALDI matrix of choice for the detection of chloramines. Although not directly within the scope of this topic, the detection of peroxidized lipids by MALDI MS is also difficult. However, there are indications that their detection can be improved if the analytes are desorbed from a target coated with nitrocellulose [204].

8.3.2. Native Lipid Mixture Analysis by ESI MS

As already indicated, ESI MS can be easily combined with chromatographic separation. Therefore, ESI coupled to HPLC (or more recently nano-HPLC) is normally the method of choice if complex lipid mixtures have to be analyzed [205]. This particularly applies because lipid oxidation products are normally only present in very small amounts in biological systems, while the native bulk lipids are by far more abundant [99]. Compounds which are present in small amounts only are normally suppressed by more abundant compounds and are thus often not detectable if the entire lipid mixtures are investigated without previous separation. The same applies if lipids with different headgroups and different tendencies to form a positive charge are investigated [206].

In a pioneering work Jerlich and coworkers [207] have shown that combined LC-ESI MS is a suitable method to monitor the oxidation products if PCs in human LDL are treated with either HOCl or the complete MPO system. It could be shown that chlorohydrin products from lipids containing oleic, linoleic, and arachidonic acids can be easily detected, but no hydroperoxides of linoleoyl or arachidonoyl lipids could be monitored. This is an important finding, since hydroperoxides were previously suspected to represent an additional reaction product which undergoes free radical-mediated reactions in the presence of HOCl [208].

Somewhat later the same authors [209] were able to show that there is a direct correlation between the content of oxidation products in the LDL sample on the one hand and the concentration of HOCl, or the MPO activity as well as the acidity of the medium, on the other hand. This could be also verified by the exposition of defined PC species to stimulated neutrophils [210]. It is nowadays commonly accepted that LC-MS is the method of choice to analyze lipid chlorohydrins, which has been reviewed recently [191]. Nevertheless, the limited commercial availability of oxidized PL standards aggravates the method development enormously. Compared to chlorinated cleavage products (α-ClFALD) of plasmalogens, their LPL chlorohydrins are easily detectable with ESI MS even without previous HPLC purification/separation [211]. These LPC-ClOH were detected by MS/MS using for example, the neutral loss scan (i.e., m/z 95 for trimethylamine of the phosphorylcholine headgroup) [212].

8.3.3. Native Lipid Mixture Analysis by APCI MS

Atmospheric pressure chemical ionization is a useful method which has facilitated lipid analysis for many years. Many classes of lipids including FFAs, PLs, sterols, and triacylglycerols are ionizable by APCI [213]. Although APCI is a soft ionization method, the relatively harsh conditions employed in the source induce some degree of fragmentation. This is sometimes helpful if no MS/MS capacity is available but aggravates the analysis of complex mixtures. Another problem regarding quantitative analysis is the strong impact of the extent of unsaturation on the ion yield. TAG can be conveniently analyzed by APCI, but APCI is not the method of choice to analyze PLs due to the relatively low sensitivity achievable. To the best of our knowledge there are only very few reports where APCI was used to analyze oxidized glycerolipids [214]. However, APCI is an excellent technique to analyze oxidized fatty acids [215]. Surprisingly, chlorinated lipids have so far not been analyzed by APCI.

8.4. Other Methods to Monitor Chlorohydrin Generation

There are not many methods [216] for evaluating the generation of lipid chlorohydrins apart from MS, but at least a few of them should be shortly mentioned.

8.4.1. Nuclear Magnetic Resonance

Although Nuclear Magnetic Resonance (NMR) suffers from comparably low sensitivity, it has often been used to study the reaction between HOCl and unsaturated fatty acids or even PLs. 1H NMR was used in the majority of cases [217] since 1H is the most sensitive NMR nucleus. The progress of the reaction between the unsaturated lipid and HOCl can be easily monitored by the disappearance of olefinic residues and the formation of the typical chlorohydrin resonances that can be easily differentiated from the resonances of simultaneously generated glycols and epoxides [89]. Due to the limited sensitivity of 13C NMR there are no reports of 13C NMR studies of lipid chlorohydrins. However, there were a few attempts to use 31P NMR to monitor lipid oxidation products. Unfortunately, chlorohydrin generation cannot be easily monitored but is only reflected by a broadened resonance of the original PL with limited information [218]. By contrast, PC and LPC can be easily differentiated by 31P NMR, and even the position of the fatty acyl residue in the LPC species can be resolved.

8.4.2. Spectroscopic Methods

Although infrared (IR) spectroscopy is surely suitable for the detection of N-Cl vibration bands which would be expected if PE or PS reacted with HOCl, there have so far been no attempts to study chloramines by IR. However, it could be shown that the reaction between for example, taurine, and HOCl is accompanied by the formation of an intense IR band at about 975 cm−1 [219], which is characteristic of N-Cl. This band is characteristic enough to confirm the presence of chlorinated compounds.

The standard method for following the reaction between HOCl and amines is UV spectroscopy, because mono- and dichloramines are characterized by a (weak) absorption in the UV range at about 254 nm [220]. Nevertheless, there is a problem if amphiphilic compounds such as lipids are investigated: although UV spectroscopy can be easily used in the case of water soluble compounds, for instance, phosphorylethanolamine or glycero-phosphorylethanolamine [65], the reliability of this assay is limited when PEs are investigated due to the light scattering effects caused by the formation of aggregates in an aqueous environment. This requires the application of suitable detergents to minimize unwanted aggregation.

8.4.3. Chromatographic Methods

As already outlined (vide supra) HPLC is widely used to separate lipid oxidation products. Although TLC seems a bit old-fashioned in comparison to HPLC, it is also widely used in lipid research, as it offers many advantages, is inexpensive, and can also be performed by nonexperts [221]. Basically, the same separations performed by HPLC may also be accomplished by TLC. For instance, the effect of HOCl on cholesterol could be monitored by TLC [194] using normal phase TLC and diethyl ether, petroleum ether, and acetic acid (70/30/1, v/v/v) as eluent, while four different reaction products (the α- and β-chlorohydrins as well as the corresponding epoxides) could be monitored in addition to cholesterol. This also applies for more complex mixtures. Oxidation products of membranes from red blood cells could be detected by TLC although the authors were not satisfied with the TLC sensitivity and therefore also made use of an ELISA approach, which is more sensitive and could be successfully applied as soon as 1 × 106 cells were available [153]. Nowadays, this sensitivity problem could also be overcome by combining TLC with MALDI MS detection, which provides a much higher sensitivity in comparison to TLC alone [222]. Applications of TLC have recently been reviewed in the context of plasmalogen oxidation product analysis [211].

8.4.4. Immunological Methods

Such methods are widely applied to monitor the HOCl-induced modification of proteins by measuring, for instance, halogenated tyrosine residues [223] and, consequently, to determine the related MPO activities [224]. However, there are also antibodies available which recognize chlorinated fatty acids or lipids: in one of the first study an antibody against the chlorohydrin of oleic acid was developed [225], although this antibody was not very specific and also recognized some other chlorinated lipids. This method was also used to investigate the modification of red cell membrane lipids by HOCl [153], but otherwise this method is not frequently used.

9. Conclusions

Nowadays, it is commonly accepted that inflammation is accompanied by the generation of ROS and RNS. Since the majority of these reactive species are transient products and/or yield transient products as primary products, the establishment of reliable and specific “biomarkers” is still a challenging task.

The focus of this review was on the reaction between HOCl that is (i) used as an important disinfectant and (ii) generated under inflammatory conditions under catalysis of the enzyme MPO and different lipids. Nevertheless, the reactions of HOCl with some other biomolecules were also discussed, because they have functional groups which possess a higher reactivity than lipids. It was shown that lipids with exclusively olefinic residues (i.e., without reactive headgroups) yield mainly the corresponding chlorohydrins. Due to the stability of these reaction products, they may be easily characterized by various methods (particularly soft ionization mass spectrometry), and even the second order rate constants () of the reactions could be determined. Comparable results are obtained when HOCl is generated by the MPO/H2O2/Cl system mimicking physiologically relevant conditions. This reaction is important for two reasons: (i) Chlorohydrin formation may lead to a destabilization of the cellular membrane and (ii) lipid peroxidation may be initiated by the reagent HOCl. Additionally, it was shown that higher unsaturated lipids also yield LPC, even in the complete absence of phospholipases. This might be an explanation of the enhanced LPC contents in joint fluids in patients with rheumatoid arthritis, which are also characterized by elevated MPO activities. A variety of chlorinated lipids can be produced by the reagent HOCl or the complete MPO/H2O2/Cl system, but only α-chloro fatty aldehydes have so far been firmly demonstrated to occur during cardiovascular diseases, while evidence for other chlorinated lipids in disease and inflammation is still lacking. Since α-chloro fatty aldehydes can exclusively be generated by plasmalogen oxidation, this emphasizes the important role of these alkenyl ether lipids and the interest plasmalogens is currently attracting.

Compared to the reactions of cholesterol and PCs, the reaction between HOCl and lipids with reactive amino residues (e.g., PE and PS) has been by far less frequently investigated, although these lipids are also very abundant in biological membranes. This might be caused by the considerable product variability under these conditions, as the chloramines which are generated as the primary products are transient products and decay into aldehydes and nitriles but may also modify other functional residues of biomolecules.

Therefore, further attempts are necessary to study these reactions in more detail. This particularly applies as it was shown very recently that chlorinated products derived from PE and PS may impact the signal transduction pathways in cells.

List of Abbreviations

AACL:Amino acid chloramine
AP:Atherosclerotic plaque
ATP:Adenosine triphosphate
ATX:Autotaxin
α-ClFALD:α-Chloro fatty aldehyde
COPD:Chronic obstructive pulmonary disease
CP:Culprit plaque
EI:Electron ionization (electron impact)
EIA:Enzyme Immunoassay
ELISA:Enzyme-Linked Immunosorbent Assay
ESI:Electrospray ionization
EPR:Electron paramagnetic resonance
FFA:Free fatty acid
FID:Flame ionization detector
GAG:Glycosaminoglycan
GC:Gas chromatography
HOBr:Hypobromous acid
HOCl:Hypochlorous acid
HOI:Hypoiodous acid
HOSCN:Hypothiocyanite
HNE:4-Hydroxy-2-nonenal
HPLC:High Performance Liquid Chromatography
HUVEC-ST:Immortalized human umbilical vein endothelial cells
IHC:Immunohistochemistry
IR:Infrared
:Second order rate constant
LC:Liquid chromatography
LDL:Low-density lipoprotein
LPA:Lysophosphatidic acid
LPC:Lysophosphatidylcholine
LPL:Lysophospholipid
MALDI:Matrix-assisted laser desorption and ionization
MPO:Myeloperoxidase
MS:Mass spectrometry
m/z:Mass over charge
NADPH:Nicotinamide adenine dinucleotide phosphate
NET:Neutrophil extracellular trap
NICI:Negative ion chemical ionization
NMR:Nuclear magnetic resonance
NaOCl:Sodium hypochlorite
Nrf2:Nuclear factor erythroid 2-related factor 2
oxPAPC:Oxidized 1-palmitoyl-2-arachidonoyl-sn-phosphatidylcholine
PA:Phosphatidic acid
PC:Phosphatidylcholine
PE:Phosphatidylethanolamine
PFB:Pentafluorobenzyl
PL:Phospholipid
PLA1:Phospholipase A1
PLA2:Phospholipase A2
PMNs:Polymorphonuclear leukocytes
PPARs:Peroxisome proliferator-activated receptors
PS:Phosphatidylserine
PUFA:Polyunsaturated fatty acid
RCS:Reactive chlorine species
RNS:Reactive nitrogen species
ROS:Reactive oxygen species
SF:Synovial fluid
SNP:Single Nucleotide Polymorphism
SOD:Superoxide dismutase
TBARS:Thiobarbituric acid reactive substances
(HP)TLC: (High performance) thin-layer chromatography
TMB:3,3′,5,5′-Tetramethylbenzidine
TNB:5-Thio-2-nitrobenzoic acid
TOF:Time-of-flight
UV:Ultraviolet
VSMC:Vascular smooth muscle cell.

Disclosure

This review was written as thesis for the postgraduate studies program “Toxikologie und Umweltschutz.” Jenny Schröter is grateful for the permission by the committee to write this review.

Competing Interests

The authors declare that there is no conflict of interests regarding the publication of this paper.

Acknowledgments

This study was supported by the German Research Council (DFG Schi 476/16-1 and SFB 1052/B6). The authors acknowledge support from the German Research Foundation (DFG).

References

  1. R. Medzhitov, “Origin and physiological roles of inflammation,” Nature, vol. 454, no. 7203, pp. 428–435, 2008. View at Publisher · View at Google Scholar · View at Scopus
  2. S. Frisenda, C. Perricone, and G. Valesini, “Cartilage as a target of autoimmunity: a thin layer,” Autoimmunity Reviews, vol. 12, no. 5, pp. 591–598, 2013. View at Publisher · View at Google Scholar · View at Scopus
  3. A. Manda-Handzlik and U. Demkow, “Neutrophils: the role of oxidative and nitrosative stress in health and disease,” in Pulmonary Infection, vol. 857 of Advances in Experimental Medicine and Biology, pp. 51–60, Springer, Berlin, Germany, 2015. View at Publisher · View at Google Scholar
  4. J. H. Forman and A. B. Fischer, “Antioxidants in the lung,” in CRC Handbook of Methods for Oxygen Radical Research, R. A. Greenwald, Ed., pp. 359–364, CRC Press, Boca Raton, Fla, USA, 1985. View at Google Scholar
  5. M. J. Gray, W.-Y. Wholey, and U. Jakob, “Bacterial responses to reactive chlorine species,” Annual Review of Microbiology, vol. 67, pp. 141–160, 2013. View at Publisher · View at Google Scholar · View at Scopus
  6. R. Senthilmohan and A. J. Kettle, “Bromination and chlorination reactions of myeloperoxidase at physiological concentrations of bromide and chloride,” Archives of Biochemistry and Biophysics, vol. 445, no. 2, pp. 235–244, 2006. View at Publisher · View at Google Scholar · View at Scopus
  7. F. H. Greig, S. Kennedy, and C. M. Spickett, “Physiological effects of oxidized phospholipids and their cellular signaling mechanisms in inflammation,” Free Radical Biology and Medicine, vol. 52, no. 2, pp. 266–280, 2012. View at Publisher · View at Google Scholar · View at Scopus
  8. C. Prasse, D. Stalter, U. Schulte-Oehlmann, J. Oehlmann, and T. A. Ternes, “Spoilt for choice: a critical review on the chemical and biological assessment of current wastewater treatment technologies,” Water Research, vol. 87, pp. 237–270, 2015. View at Publisher · View at Google Scholar · View at Scopus
  9. C. H. Jeong, C. Postigo, S. D. Richardson et al., “Occurrence and comparative toxicity of haloacetaldehyde disinfection byproducts in drinking water,” Environmental Science and Technology, vol. 49, no. 23, pp. 13749–13759, 2015. View at Publisher · View at Google Scholar · View at Scopus
  10. D. Kim, G. L. Amy, and T. Karanfil, “Disinfection by-product formation during seawater desalination: a review,” Water Research, vol. 81, pp. 343–355, 2015. View at Publisher · View at Google Scholar · View at Scopus
  11. C. M. Spickett, “Chlorinated lipids and fatty acids: an emerging role in pathology,” Pharmacology and Therapeutics, vol. 115, no. 3, pp. 400–409, 2007. View at Publisher · View at Google Scholar · View at Scopus
  12. G. O. Frühwirth, A. Loidl, and A. Hermetter, “Oxidized phospholipids: from molecular properties to disease,” Biochimica et Biophysica Acta (BBA)—Molecular Basis of Disease, vol. 1772, no. 7, pp. 718–736, 2007. View at Publisher · View at Google Scholar · View at Scopus
  13. C. Mauerhofer, M. Philippova, O. V. Oskolkova, and V. N. Bochkov, “Hormetic and anti-inflammatory properties of oxidized phospholipids,” Molecular Aspects of Medicine, vol. 49, pp. 78–90, 2016. View at Publisher · View at Google Scholar
  14. V. N. Bochkov, O. V. Oskolkova, K. G. Birukov, A.-L. Levonen, C. J. Binder, and J. Stöckl, “Generation and biological activities of oxidized phospholipids,” Antioxidants & Redox Signaling, vol. 12, no. 8, pp. 1009–1059, 2010. View at Publisher · View at Google Scholar · View at Scopus
  15. X. Han and R. W. Gross, “Global analyses of cellular lipidomes directly from crude extracts of biological samples by ESI mass spectrometry: a bridge to lipidomics,” Journal of Lipid Research, vol. 44, no. 6, pp. 1071–1079, 2003. View at Publisher · View at Google Scholar · View at Scopus
  16. G. Astarita, A. C. Kendall, E. A. Dennis, and A. Nicolaou, “Targeted lipidomic strategies for oxygenated metabolites of polyunsaturated fatty acids,” Biochimica et Biophysica Acta (BBA)—Molecular and Cell Biology of Lipids, vol. 1851, no. 4, pp. 456–468, 2015. View at Publisher · View at Google Scholar · View at Scopus
  17. S. V. Pande and J. F. Mead, “Inhibition of enzyme activities by free fatty acids,” The Journal of Biological Chemistry, vol. 243, no. 23, pp. 6180–6185, 1968. View at Google Scholar · View at Scopus
  18. N. Borregaard, “Neutrophils, from marrow to microbes,” Immunity, vol. 33, no. 5, pp. 657–670, 2010. View at Publisher · View at Google Scholar · View at Scopus
  19. E. Kolaczkowska and P. Kubes, “Neutrophil recruitment and function in health and inflammation,” Nature Reviews Immunology, vol. 13, no. 3, pp. 159–175, 2013. View at Publisher · View at Google Scholar · View at Scopus
  20. G. Wang and W. M. Nauseef, “Salt, chloride, bleach, and innate host defense,” Journal of Leukocyte Biology, vol. 98, no. 2, pp. 163–172, 2015. View at Publisher · View at Google Scholar · View at Scopus
  21. Y. Kato, “Neutrophil myeloperoxidase and its substrates: Formation of specific markers and reactive compounds during inflammation,” Journal of Clinical Biochemistry and Nutrition, vol. 58, no. 2, pp. 99–104, 2016. View at Publisher · View at Google Scholar
  22. B. Amulic, C. Cazalet, G. L. Hayes, K. D. Metzler, and A. Zychlinsky, “Neutrophil function: from mechanisms to disease,” Annual Review of Immunology, vol. 30, pp. 459–489, 2012. View at Publisher · View at Google Scholar · View at Scopus
  23. T. Strowig, J. Henao-Mejia, E. Elinav, and R. Flavell, “Inflammasomes in health and disease,” Nature, vol. 481, no. 7381, pp. 278–286, 2012. View at Publisher · View at Google Scholar · View at Scopus
  24. E. Minichiello, L. Semerano, and M.-C. Boissier, “Time trends in the incidence, prevalence, and severity of rheumatoid arthritis: a systematic literature review,” Joint, Bone, Spine, vol. 83, no. 6, pp. 625–630, 2016. View at Publisher · View at Google Scholar
  25. J. Schiller, S. Benard, S. Reichl, J. Arnhold, and K. Arnold, “Cartilage degradation by stimulated human neutrophils: reactive oxygen species decrease markedly the activity of proteolytic enzymes,” Chemistry and Biology, vol. 7, no. 8, pp. 557–568, 2000. View at Publisher · View at Google Scholar · View at Scopus
  26. H. R. Jones, C. T. Robb, M. Perretti, and A. G. Rossi, “The role of neutrophils in inflammation resolution,” Seminars in Immunology, vol. 28, no. 2, pp. 137–145, 2016. View at Google Scholar
  27. S. de Oliveira, E. E. Rosowski, and A. Huttenlocher, “Neutrophil migration in infection and wound repair: going forward in reverse,” Nature Reviews Immunology, vol. 16, no. 6, pp. 378–391, 2016. View at Google Scholar
  28. L. Zuo, T. Zhou, B. K. Pannell, A. C. Ziegler, and T. M. Best, “Biological and physiological role of reactive oxygen species—the good, the bad and the ugly,” Acta Physiologica, vol. 214, no. 3, pp. 329–348, 2015. View at Publisher · View at Google Scholar · View at Scopus
  29. J. Huang, A. Milton, R. D. Arnold et al., “Methods for measuring myeloperoxidase activity toward assessing inhibitor efficacy in living systems,” Journal of Leukocyte Biology, vol. 99, no. 4, pp. 541–548, 2016. View at Publisher · View at Google Scholar
  30. L. A. Marquez and H. B. Dunford, “Kinetics of oxidation of tyrosine and dityrosine by myeloperoxidase compounds I and II: implications for lipoprotein peroxidation studies,” The Journal of Biological Chemistry, vol. 270, no. 51, pp. 30434–30440, 1995. View at Publisher · View at Google Scholar · View at Scopus
  31. P. G. Furtmuller, U. Burner, and C. Obinger, “Reaction of myeloperoxidase compound I with chloride, bromide, iodide, and thiocyanate,” Biochemistry, vol. 37, no. 51, pp. 17923–17930, 1998. View at Publisher · View at Google Scholar · View at Scopus
  32. J. Arnhold and J. Flemmig, “Human myeloperoxidase in innate and acquired immunity,” Archives of Biochemistry and Biophysics, vol. 500, no. 1, pp. 92–106, 2010. View at Publisher · View at Google Scholar · View at Scopus
  33. O. M. Panasenko, I. V. Gorudko, and A. V. Sokolov, “Hypochlorous acid as a precursor of free radicals in living systems,” Biochemistry, vol. 78, no. 13, pp. 1466–1489, 2013. View at Publisher · View at Google Scholar · View at Scopus
  34. A. Korotaeva, E. Samoilova, T. Pavlunina, and O. M. Panasenko, “Halogenated phospholipids regulate secretory phospholipase A2 group IIA activity,” Chemistry and Physics of Lipids, vol. 167-168, pp. 51–56, 2013. View at Publisher · View at Google Scholar · View at Scopus
  35. M. Katrantzis, M. S. Baker, C. J. Handley, and D. A. Lowther, “The oxidant hypochlorite (OCl), a product of the myeloperoxidase system, degrades articular cartilage proteoglycan aggregate,” Free Radical Biology and Medicine, vol. 10, no. 2, pp. 101–109, 1991. View at Publisher · View at Google Scholar · View at Scopus
  36. D. I. Pattison, M. J. Davies, and C. L. Hawkins, “Reactions and reactivity of myeloperoxidase-derived oxidants: differential biological effects of hypochlorous and hypothiocyanous acids,” Free Radical Research, vol. 46, no. 8, pp. 975–995, 2012. View at Publisher · View at Google Scholar · View at Scopus
  37. K. M. Pruitt, D. N. Kamau, K. Miller, B. Månsson-Rahemtulla, and F. Rahemtulla, “Quantitative, standardized assays for determining the concentrations of bovine lactoperoxidase, human salivary peroxidase, and human myeloperoxidase,” Analytical Biochemistry, vol. 191, no. 2, pp. 278–286, 1990. View at Publisher · View at Google Scholar · View at Scopus
  38. Z. Wang, S. J. Nicholls, E. R. Rodriguez et al., “Protein carbamylation links inflammation, smoking, uremia and atherogenesis,” Nature Medicine, vol. 13, no. 10, pp. 1176–1184, 2007. View at Publisher · View at Google Scholar · View at Scopus
  39. J. P. Henderson, J. Byun, M. V. Williams, D. M. Mueller, M. L. McCormick, and J. W. Heinecke, “Production of brominating intermediates by myeloperoxidase. A transhalogenation pathway for generating mutagenic nucleobases during inflammation,” The Journal of Biological Chemistry, vol. 276, no. 11, pp. 7867–7875, 2001. View at Publisher · View at Google Scholar · View at Scopus
  40. T. M. Aune and E. L. Thomas, “Oxidation of protein sulfhydryls by products of peroxidase-catalyzed oxidation of thiocyanate ion,” Biochemistry, vol. 17, no. 6, pp. 1005–1010, 1978. View at Publisher · View at Google Scholar · View at Scopus
  41. J. D. Chandler and B. J. Day, “Thiocyanate: a potentially useful therapeutic agent with host defense and antioxidant properties,” Biochemical Pharmacology, vol. 84, no. 11, pp. 1381–1387, 2012. View at Publisher · View at Google Scholar · View at Scopus
  42. J.-U. Dahl, M. J. Gray, and U. Jakob, “Protein quality control under oxidative stress conditions,” Journal of Molecular Biology, vol. 427, no. 7, pp. 1549–1563, 2015. View at Publisher · View at Google Scholar · View at Scopus
  43. A. Sassa, N. Kamoshita, T. Matsuda et al., “Miscoding properties of 8-chloro-2′-deoxyguanosine, a hypochlorous acid-induced DNA adduct, catalysed by human DNA polymerases,” Mutagenesis, vol. 28, no. 1, pp. 81–88, 2013. View at Publisher · View at Google Scholar · View at Scopus
  44. R. S. Ray and A. Katyal, “Myeloperoxidase: bridging the gap in neurodegeneration,” Neuroscience and Biobehavioral Reviews, vol. 68, pp. 611–620, 2016. View at Google Scholar
  45. S. J. Klebanoff, A. M. Waltersdorph, and H. Rosen, “Antimicrobial activity of myeloperoxidase,” Methods in Enzymology, vol. 105, pp. 399–403, 1984. View at Publisher · View at Google Scholar
  46. B. Fuchs, C. Schober, G. Richter, A. Nimptsch, R. Süß, and J. Schiller, “The reactions between HOCl and differently saturated phospholipids: physiological relevance, products and methods of evaluation,” Mini-Reviews in Organic Chemistry, vol. 5, no. 3, pp. 254–261, 2008. View at Publisher · View at Google Scholar · View at Scopus
  47. A. J. Kettle, A. M. Albrett, A. L. Chapman et al., “Measuring chlorine bleach in biology and medicine,” Biochimica et Biophysica Acta (BBA)—General Subjects, vol. 1840, no. 2, pp. 781–793, 2014. View at Publisher · View at Google Scholar · View at Scopus
  48. B. S. Crow, J. Quiñones-González, B. G. Pantazides et al., “Simultaneous measurement of 3-chlorotyrosine and 3,5-cichlorotyrosine in whole blood, serum and plasma by isotope dilution HPLC-MS-MS,” Journal of Analytical Toxicology, vol. 40, no. 4, pp. 264–271, 2016. View at Publisher · View at Google Scholar
  49. J. P. Gaut, J. Byun, H. D. Tran, and J. W. Heinecke, “Artifact-free quantification of free 3-chlorotyrosine, 3-bromotyrosine, and 3-nitrotyrosine in human plasma by electron capture-negative chemical ionization gas chromatography mass spectrometry and liquid chromatography-electrospray ionization tandem mass spectrometry,” Analytical Biochemistry, vol. 300, no. 2, pp. 252–259, 2002. View at Publisher · View at Google Scholar · View at Scopus
  50. S. Fu, H. Wang, M. Davies, and R. Dean, “Reactions of hypochlorous acid with tyrosine and peptidyl-tyrosyl residues give dichlorinated and aldehydic products in addition to 3-chlorotyrosine,” The Journal of Biological Chemistry, vol. 275, no. 15, pp. 10851–10858, 2000. View at Publisher · View at Google Scholar · View at Scopus
  51. N. M. Domigan, T. S. Charlton, M. W. Duncan, C. C. Winterbourn, and A. J. Kettle, “Chlorination of tyrosyl residues in peptides by myeloperoxidase and human neutrophils,” The Journal of Biological Chemistry, vol. 270, no. 28, pp. 16542–16548, 1995. View at Publisher · View at Google Scholar · View at Scopus
  52. A. R. Mani, S. Ippolito, J. C. Moreno, T. J. Visser, and K. P. Moore, “The metabolism and dechlorination of chlorotyrosine in vivo,” The Journal of Biological Chemistry, vol. 282, no. 40, pp. 29114–29121, 2007. View at Publisher · View at Google Scholar · View at Scopus
  53. J. Talib, G. J. Maghzal, D. Cheng, and R. Stocker, “Detailed protocol to assess in vivo and ex vivo myeloperoxidase activity in mouse models of vascular inflammation and disease using hydroethidine,” Free Radical Biology & Medicine, vol. 97, pp. 124–135, 2016. View at Google Scholar
  54. M. B. Grisham, M. M. Jefferson, D. F. Melton, and E. L. Thomas, “Chlorination of endogenous amines by isolated neutrophils. Ammonia-dependent bactericidal, cytotoxic, and cytolytic activities of the chloramines,” The Journal of Biological Chemistry, vol. 259, no. 16, pp. 10404–10413, 1984. View at Google Scholar · View at Scopus
  55. N. R. Stanley, D. I. Pattison, and C. L. Hawkins, “Ability of hypochlorous acid and N-chloramines to chlorinate DNA and its constituents,” Chemical Research in Toxicology, vol. 23, no. 7, pp. 1293–1302, 2010. View at Publisher · View at Google Scholar · View at Scopus
  56. J. Marcinkiewicz and E. Kontny, “Taurine and inflammatory diseases,” Amino Acids, vol. 46, no. 1, pp. 7–20, 2014. View at Publisher · View at Google Scholar · View at Scopus
  57. J. M. Dypbukt, C. Bishop, W. M. Brooks, B. Thong, H. Eriksson, and A. J. Kettle, “A sensitive and selective assay for chloramine production by myeloperoxidase,” Free Radical Biology and Medicine, vol. 39, no. 11, pp. 1468–1477, 2005. View at Publisher · View at Google Scholar · View at Scopus
  58. O. Skaff, D. I. Pattison, and M. J. Davies, “The vinyl ether linkages of plasmalogens are favored targets for myeloperoxidase-derived oxidants: a kinetic study,” Biochemistry, vol. 47, no. 31, pp. 8237–8245, 2008. View at Publisher · View at Google Scholar · View at Scopus
  59. D. T. Harwood, A. J. Kettle, and C. C. Winterbourn, “Production of glutathione sulfonamide and dehydroglutathione from GSH by myeloperoxidase-derived oxidants and detection using a novel LC–MS/MS method,” Biochemical Journal, vol. 399, no. 1, pp. 161–168, 2006. View at Publisher · View at Google Scholar · View at Scopus
  60. E.-M. Daphna, S. Michaela, P. Eynat, A. Irit, and S. Rimon, “Association of myeloperoxidase with heparin: oxidative inactivation of proteins on the surface of endothelial cells by the bound enzyme,” Molecular and Cellular Biochemistry, vol. 183, no. 1-2, pp. 55–61, 1998. View at Publisher · View at Google Scholar · View at Scopus
  61. J. Leßig, H. Spalteholz, U. Reibetanz et al., “Myeloperoxidase binds to non-vital spermatozoa on phosphatidylserine epitopes,” Apoptosis, vol. 12, no. 10, pp. 1803–1812, 2007. View at Publisher · View at Google Scholar · View at Scopus
  62. C. C. Winterbourn, “Reconciling the chemistry and biology of reactive oxygen species,” Nature Chemical Biology, vol. 4, no. 5, pp. 278–286, 2008. View at Publisher · View at Google Scholar · View at Scopus
  63. N. Thieblemont, H. L. Wright, S. W. Edwards, and V. Witko-Sarsat, “Human neutrophils in auto-immunity,” Seminars in Immunology, vol. 28, no. 2, pp. 159–173, 2016. View at Publisher · View at Google Scholar
  64. M. Deborde and U. von Gunten, “Reactions of chlorine with inorganic and organic compounds during water treatment—kinetics and mechanisms: a critical review,” Water Research, vol. 42, no. 1-2, pp. 13–51, 2008. View at Publisher · View at Google Scholar · View at Scopus
  65. D. I. Pattison, C. L. Hawkins, and M. J. Davies, “Hypochlorous acid-mediated oxidation of lipid components and antioxidants present in low-density lipoproteins: absolute rate constants, product analysis, and computational modeling,” Chemical Research in Toxicology, vol. 16, no. 4, pp. 439–449, 2003. View at Publisher · View at Google Scholar · View at Scopus
  66. C. L. Hawkins and M. J. Davies, “Reaction of HOCl with amino acids and peptides: EPR evidence for rapid rearrangement and fragmentation reactions of nitrogen-centred radicals,” Journal of the Chemical Society, Perkin Transactions, vol. 2, no. 9, pp. 1937–1946, 1998. View at Google Scholar
  67. C. L. Hawkins and M. J. Davies, “Hypochlorite-induced damage to DNA, RNA, and polynucleotides: formation of chloramines and nitrogen-centered radicals,” Chemical Research in Toxicology, vol. 14, pp. 1071–1081, 2001. View at Google Scholar
  68. M. D. Rees, C. L. Hawkins, and M. J. Davies, “Hypochlorite-mediated fragmentation of hyaluronan, chondroitin sulfates, and related N-acetyl glycosamines: evidence for chloramide intermediates, free radical transfer reactions, and site-specific fragmentation,” Journal of the American Chemical Society, vol. 125, no. 45, pp. 13719–13733, 2003. View at Publisher · View at Google Scholar · View at Scopus
  69. Y. Kawai, H. Kiyokawa, Y. Kimura, Y. Kato, K. Tsuchiya, and J. Terao, “Hypochlorous acid-derived modification of phospholipids: characterization of aminophospholipids as regulatory molecules for lipid peroxidation,” Biochemistry, vol. 45, no. 47, pp. 14201–14211, 2006. View at Publisher · View at Google Scholar · View at Scopus
  70. J. Arnhold, S. Hammerschmidt, M. Wagner, S. Mueller, K. Arnold, and E. Grimm, “On the action of hypochlorite on human serum albumin,” Biomedica Biochimica Acta, vol. 49, no. 10, pp. 991–997, 1990. View at Google Scholar · View at Scopus
  71. A. Robaszkiewicz, G. Bartosz, and M. Soszyński, “Effect of N-chloroamino acids on the erythrocyte,” Free Radical Research, vol. 42, no. 1, pp. 30–39, 2008. View at Publisher · View at Google Scholar · View at Scopus
  72. S. A. Salama and R. M. Snapka, “Amino acid chloramine damage to proliferating cell nuclear antigen in mammalian cells,” In Vivo, vol. 26, no. 4, pp. 501–517, 2012. View at Google Scholar · View at Scopus
  73. J. Schiller, B. Fuchs, J. Arnhold, and K. Arnold, “Contribution of reactive oxygen species to cartilage degradation in rheumatic diseases: molecular pathways, diagnosis and potential therapeutic strategies,” Current Medicinal Chemistry, vol. 10, no. 20, pp. 2123–2145, 2003. View at Publisher · View at Google Scholar · View at Scopus
  74. C. L. Hawkins, D. I. Pattison, and M. J. Davies, “Hypochlorite-induced oxidation of amino acids, peptides and proteins,” Amino Acids, vol. 25, no. 3-4, pp. 259–274, 2003. View at Publisher · View at Google Scholar · View at Scopus
  75. Z. Cai and L.-J. Yan, “Protein oxidative modifications: beneficial roles in disease and health,” Journal of Biochemical and Pharmacological Research, vol. 1, no. 1, pp. 15–26, 2013. View at Google Scholar
  76. A. V. Peskin, R. Turner, G. J. Maghzal, C. C. Winterbourn, and A. J. Kettle, “Oxidation of methionine to dehydromethionine by reactive halogen species generated by neutrophils,” Biochemistry, vol. 48, no. 42, pp. 10175–10182, 2009. View at Publisher · View at Google Scholar · View at Scopus
  77. B. S. Rayner, D. T. Love, and C. L. Hawkins, “Comparative reactivity of myeloperoxidase-derived oxidants with mammalian cells,” Free Radical Biology and Medicine, vol. 71, pp. 240–255, 2014. View at Publisher · View at Google Scholar · View at Scopus
  78. Y. Kawai, H. Morinaga, H. Kondo et al., “Endogenous formation of novel halogenated 2′-deoxycytidine: hypohalous acid-mediated DNA modification at the site of inflammation,” The Journal of Biological Chemistry, vol. 279, no. 49, pp. 51241–51249, 2004. View at Publisher · View at Google Scholar · View at Scopus
  79. V. Kuttappan-Nair, F. Samson-Thibault, and J. R. Wagner, “Generation of 2′-deoxyadenosine N6-aminyl radicals from the photolysis of phenylhydrazone derivatives,” Chemical Research in Toxicology, vol. 23, no. 1, pp. 48–54, 2010. View at Publisher · View at Google Scholar · View at Scopus
  80. T. Asahi, H. Kondo, M. Masuda et al., “Chemical and immunochemical detection of 8-halogenated deoxyguanosines at early stage inflammation,” The Journal of Biological Chemistry, vol. 285, no. 12, pp. 9282–9291, 2010. View at Publisher · View at Google Scholar · View at Scopus
  81. B. I. Fedeles, B. D. Freudenthal, E. Yau et al., “Intrinsic mutagenic properties of 5-chlorocytosine: a mechanistic connection between chronic inflammation and cancer,” Proceedings of the National Academy of Sciences of the United States of America, vol. 112, no. 33, pp. E4571–E4580, 2015. View at Publisher · View at Google Scholar · View at Scopus
  82. N. Güngör, A. M. Knaapen, A. Munnia et al., “Genotoxic effects of neutrophils and hypochlorous acid,” Mutagenesis, vol. 25, no. 2, pp. 149–154, 2010. View at Publisher · View at Google Scholar · View at Scopus
  83. A. Valavanidis, T. Vlachogianni, and C. Fiotakis, “8-Hydroxy-2′-deoxyguanosine (8-OHdG): a critical biomarker of oxidative stress and carcinogenesis,” Journal of Environmental Science and Health Part C: Environmental Carcinogenesis and Ecotoxicology Reviews, vol. 27, no. 2, pp. 120–139, 2009. View at Publisher · View at Google Scholar · View at Scopus
  84. C. Badouard, M. Masuda, H. Nishino, J. Cadet, A. Favier, and J.-L. Ravanat, “Detection of chlorinated DNA and RNA nucleosides by HPLC coupled to tandem mass spectrometry as potential biomarkers of inflammation,” Journal of Chromatography B: Analytical Technologies in the Biomedical and Life Sciences, vol. 827, no. 1, pp. 26–31, 2005. View at Publisher · View at Google Scholar · View at Scopus
  85. N. Y. Tretyakova, A. Groehler, and S. Ji, “DNA-protein cross-links: formation, structural identities, and biological outcomes,” Accounts of Chemical Research, vol. 48, no. 6, pp. 1631–1644, 2015. View at Publisher · View at Google Scholar · View at Scopus
  86. C. L. Hawkins, D. I. Pattison, and M. J. Davies, “Reaction of protein chloramines with DNA and nucleosides: evidence for the formation of radicals, protein-DNA cross-links and DNA fragmentation,” Biochemical Journal, vol. 365, no. 3, pp. 605–615, 2002. View at Publisher · View at Google Scholar · View at Scopus
  87. P. A. Kulcharyk and J. W. Heinecke, “Hypochlorous acid produced by the myeloperoxidase system of human phagocytes induces covalent cross-links between DNA and protein,” Biochemistry, vol. 40, no. 12, pp. 3648–3656, 2001. View at Publisher · View at Google Scholar · View at Scopus
  88. B. Fuchs and J. Schiller, “Glycosaminoglycan degradation by selected reactive oxygen species,” Antioxidants & Redox Signaling, vol. 21, no. 7, pp. 1044–1062, 2014. View at Publisher · View at Google Scholar · View at Scopus
  89. J. Arnhold, O. M. Panasenko, J. Schiller, Y. A. Vladimirov, and K. Arnold, “The action of hypochlorous acid on phosphatidylcholine liposomes in dependence on the content of double bonds. Stoichiometry and NMR analysis,” Chemistry and Physics of Lipids, vol. 78, no. 1, pp. 55–64, 1995. View at Publisher · View at Google Scholar · View at Scopus
  90. W. A. Prütz, “Hypochlorous acid interactions with thiols, nucleotides, DNA, and other biological substrates,” Archives of Biochemistry and Biophysics, vol. 332, no. 1, pp. 110–120, 1996. View at Publisher · View at Google Scholar · View at Scopus
  91. D. I. Pattison and M. J. Davies, “Absolute rate constants for the reaction of hypochlorous acid with protein side chains and peptide bonds,” Chemical Research in Toxicology, vol. 14, no. 10, pp. 1453–1464, 2001. View at Publisher · View at Google Scholar · View at Scopus
  92. A. Akeel, S. Sibanda, S. W. Martin, A. W. J. Paterson, and B. J. Parsons, “Chlorination and oxidation of heparin and hyaluronan by hypochlorous acid and hypochlorite anions: effect of sulfate groups on reaction pathways and kinetics,” Free Radical Biology and Medicine, vol. 56, pp. 72–88, 2013. View at Publisher · View at Google Scholar · View at Scopus
  93. M. D. Rees, C. L. Hawkins, and M. J. Davies, “Hypochlorite and superoxide radicals can act synergistically to induce fragmentation of hyaluronan and chondroitin sulphates,” The Biochemical Journal, vol. 381, no. 1, pp. 175–184, 2004. View at Publisher · View at Google Scholar · View at Scopus
  94. C. Termeer, J. P. Sleeman, and J. C. Simon, “Hyaluronan—magic glue for the regulation of the immune response?” Trends in Immunology, vol. 24, no. 3, pp. 112–114, 2003. View at Publisher · View at Google Scholar · View at Scopus
  95. G. Richter, C. Schober, R. Süß, B. Fuchs, C. Birkemeyer, and J. Schiller, “Comparison of the positive and negative ion electrospray ionization and matrix-assisted laser desorption ionization-time-of-flight mass spectra of the reaction products of phosphatidylethanolamines and hypochlorous acid,” Analytical Biochemistry, vol. 376, no. 1, pp. 157–159, 2008. View at Publisher · View at Google Scholar · View at Scopus
  96. L. J. Hazell, M. J. Davies, and R. Stocker, “Secondary radicals derived from chloramines of apolipoprotein B-100 contribute to HOCl-induced lipid peroxidation of low-density lipoproteins,” The Biochemical Journal, vol. 339, no. 3, pp. 489–495, 1999. View at Publisher · View at Google Scholar · View at Scopus
  97. M. R. M. Domingues, A. Reis, and P. Domingues, “Mass spectrometry analysis of oxidized phospholipids,” Chemistry and Physics of Lipids, vol. 156, no. 1-2, pp. 1–12, 2008. View at Publisher · View at Google Scholar · View at Scopus
  98. B. Fuchs, K. Bresler, and J. Schiller, “Oxidative changes of lipids monitored by MALDI MS,” Chemistry and Physics of Lipids, vol. 164, no. 8, pp. 782–795, 2011. View at Publisher · View at Google Scholar · View at Scopus
  99. C. M. Spickett and A. R. Pitt, “Oxidative lipidomics coming of age: advances in analysis of oxidized phospholipids in physiology and pathology,” Antioxidants & Redox Signaling, vol. 22, no. 18, pp. 1646–1666, 2015. View at Publisher · View at Google Scholar · View at Scopus
  100. C. Code, A. K. Mahalka, K. Bry, and P. K. J. Kinnunen, “Activation of phospholipase A2 by 1-palmitoyl-2-(9′-oxo-nonanoyl)-sn-glycero-3-phosphocholine in vitro,” Biochimica et Biophysica Acta—Biomembranes, vol. 1798, no. 8, pp. 1593–1600, 2010. View at Publisher · View at Google Scholar · View at Scopus
  101. W. P. Evans, “Über die Abspaltungsgeschwindigkeiten von Chlorwasserstoff aus Chlorhydrinen und ihre Beziehung zur stereochemischen Konstitution,” Zeitschrift für Physikalische Chemie, vol. 7, pp. 337–357, 1981. View at Google Scholar
  102. P. Petrenko-Kritschenko and A. Konschin, “Ueber die Leichtigkeit der Bildung ringförmiger Verbindungen,” Justus Liebig's Annalen der Chemie, vol. 342, no. 1, pp. 51–59, 1905. View at Publisher · View at Google Scholar
  103. J. Schröter, H. Griesinger, E. Reuß et al., “Unexpected products of the hypochlorous acid-induced oxidation of oleic acid: a study using high performance thin-layer chromatography-electrospray ionization mass spectrometry,” Journal of Chromatography A, vol. 1439, pp. 89–96, 2016. View at Publisher · View at Google Scholar
  104. W.-Y. Wang, C. J. Albert, and D. A. Ford, “Approaches for the analysis of chlorinated lipids,” Analytical Biochemistry, vol. 443, no. 2, pp. 148–152, 2013. View at Publisher · View at Google Scholar · View at Scopus
  105. N. E. Braverman and A. B. Moser, “Functions of plasmalogen lipids in health and disease,” Biochimica et Biophysica Acta—Molecular Basis of Disease, vol. 1822, no. 9, pp. 1442–1452, 2012. View at Publisher · View at Google Scholar · View at Scopus
  106. H. Goldfine, “The appearance, disappearance and reappearance of plasmalogens in evolution,” Progress in Lipid Research, vol. 49, no. 4, pp. 493–498, 2010. View at Publisher · View at Google Scholar · View at Scopus
  107. B. Fuchs, K. Müller, U. Paasch, and J. Schiller, “Lysophospholipids: potential markers of diseases and infertility?” Mini-Reviews in Medicinal Chemistry, vol. 12, no. 1, pp. 74–86, 2012. View at Publisher · View at Google Scholar · View at Scopus
  108. R. C. Murphy, “Free-radical-induced oxidation of arachidonoyl plasmalogen phospholipids: antioxidant mechanism and precursor pathway for bioactive eicosanoids,” Chemical Research in Toxicology, vol. 14, no. 5, pp. 463–472, 2001. View at Publisher · View at Google Scholar · View at Scopus
  109. J. Leßig and B. Fuchs, “HOCl-mediated glycerophosphocholine and glycerophosphoethanolamine generation from plasmalogens in phospholipid mixtures,” Lipids, vol. 45, no. 1, pp. 37–51, 2010. View at Publisher · View at Google Scholar · View at Scopus
  110. S. Wallner and G. Schmitz, “Plasmalogens the neglected regulatory and scavenging lipid species,” Chemistry and Physics of Lipids, vol. 164, no. 6, pp. 573–589, 2011. View at Publisher · View at Google Scholar · View at Scopus
  111. J. Leßig, J. Schiller, J. Arnhold, and B. Fuchs, “Hypochlorous acid-mediated generation of glycerophosphocholine from unsaturated plasmalogen glycerophosphocholine lipids,” The Journal of Lipid Research, vol. 48, no. 6, pp. 1316–1324, 2007. View at Publisher · View at Google Scholar · View at Scopus
  112. A. Üllen, G. Fauler, H. Köfeler et al., “Mouse brain plasmalogens are targets for hypochlorous acid-mediated modification in vitro and in vivo,” Free Radical Biology and Medicine, vol. 49, no. 11, pp. 1655–1665, 2010. View at Publisher · View at Google Scholar · View at Scopus
  113. O. Cynshi and R. Stocker, “Inhibition of lipoprotein lipid oxidation,” Handbook of Experimental Pharmacology, no. 170, pp. 563–590, 2005. View at Google Scholar
  114. D. Hasanally, R. Chaudhary, and A. Ravandi, “Role of phospholipases and oxidized phospholipids in inflammation,” in Phospholipases in Health and Disease, pp. 55–72, Springer, New York, NY, USA, 2014. View at Google Scholar
  115. B. Davis, G. Koster, L. J. Douet et al., “Electrospray ionization mass spectrometry identifies substrates and products of lipoprotein-associated phospholipase A2 in oxidized human low density lipoprotein,” The Journal of Biological Chemistry, vol. 283, no. 10, pp. 6428–6437, 2008. View at Publisher · View at Google Scholar · View at Scopus
  116. M. G. Salgo, F. P. Corongiu, and A. Sevanian, “Enhanced interfacial catalysis and hydrolytic specificity of phospholipase A2 toward peroxidized phosphatidylcholine vesicles,” Archives of Biochemistry and Biophysics, vol. 304, no. 1, pp. 123–132, 1993. View at Publisher · View at Google Scholar · View at Scopus
  117. D. N. Bateman, “Household products,” Medicine, vol. 40, no. 3, pp. 125–126, 2012. View at Publisher · View at Google Scholar · View at Scopus
  118. S. D. Richardson, M. J. Plewa, E. D. Wagner, R. Schoeny, and D. M. DeMarini, “Occurrence, genotoxicity, and carcinogenicity of regulated and emerging disinfection by-products in drinking water: a review and roadmap for research,” Mutation Research—Reviews in Mutation Research, vol. 636, no. 1–3, pp. 178–242, 2007. View at Publisher · View at Google Scholar · View at Scopus
  119. H. R. Spencer, V. Ike, and P. A. Brennan, “Review: the use of sodium hypochlorite in endodontics—potential complications and their management,” British Dental Journal, vol. 202, no. 9, pp. 555–559, 2007. View at Publisher · View at Google Scholar · View at Scopus
  120. A. Nzeusseu Toukap, C. Delporte, C. Noyon et al., “Myeloperoxidase and its products in synovial fluid of patients with treated or untreated rheumatoid arthritis,” Free Radical Research, vol. 48, no. 4, pp. 461–465, 2014. View at Publisher · View at Google Scholar · View at Scopus
  121. W. Wang, Z. Jian, J. Guo, and X. Ning, “Increased levels of serum myeloperoxidase in patients with active rheumatoid arthritis,” Life Sciences, vol. 117, no. 1, pp. 19–23, 2014. View at Publisher · View at Google Scholar · View at Scopus
  122. L. K. Stamp, I. Khalilova, J. M. Tarr et al., “Myeloperoxidase and oxidative stress in rheumatoid arthritis,” Rheumatology, vol. 51, no. 10, pp. 1796–1803, 2012. View at Publisher · View at Google Scholar · View at Scopus
  123. J. Schiller, J. Arnhold, K. Sonntag, and K. Arnold, “NMR studies on human, pathologically changed synovial fluids: role of hypochlorous acid,” Magnetic Resonance in Medicine, vol. 35, no. 6, pp. 848–853, 1996. View at Publisher · View at Google Scholar · View at Scopus
  124. J. Ilisson, M. Zagura, K. Zilmer et al., “Increased carotid artery intima-media thickness and myeloperoxidase level in children with newly diagnosed juvenile idiopathic arthritis,” Arthritis Research & Therapy, vol. 17, article 180, pp. 1–7, 2015. View at Publisher · View at Google Scholar · View at Scopus
  125. C. Pruunsild, K. Heilman, K. Zilmer et al., “Plasma level of myeloperoxidase in children with juvenile idiopathic arthritis (a pilot study),” Open Medicine, vol. 5, no. 1, pp. 36–40, 2010. View at Google Scholar
  126. L. Q. Chen, A. Rohatgi, C. R. Ayers et al., “Race-specific associations of myeloperoxidase with atherosclerosis in a population-based sample: the Dallas Heart Study,” Atherosclerosis, vol. 219, no. 2, pp. 833–838, 2011. View at Publisher · View at Google Scholar · View at Scopus
  127. A. V. Sokolov, K. V. Ageeva, O. S. Cherkalina et al., “Identification and properties of complexes formed by myeloperoxidase with lipoproteins and ceruloplasmin,” Chemistry and Physics of Lipids, vol. 163, no. 4-5, pp. 347–355, 2010. View at Publisher · View at Google Scholar · View at Scopus
  128. S. Sugiyama, Y. Okada, G. K. Sukhova, R. Virmani, J. W. Heinecke, and P. Libby, “Macrophage myeloperoxidase regulation by granulocyte macrophage colony-stimulating factor in human atherosclerosis and implications in acute coronary syndromes,” The American Journal of Pathology, vol. 158, no. 3, pp. 879–891, 2001. View at Publisher · View at Google Scholar · View at Scopus
  129. A. Daugherty, J. L. Dunn, D. L. Rateri, and J. W. Heinecke, “Myeloperoxidase, a catalyst for lipoprotein oxidation, is expressed in human atherosclerotic lesions,” The Journal of Clinical Investigation, vol. 94, no. 1, pp. 437–444, 1994. View at Publisher · View at Google Scholar · View at Scopus
  130. H. Rangé, J. Labreuche, L. Louedec et al., “Periodontal bacteria in human carotid atherothrombosis as a potential trigger for neutrophil activation,” Atherosclerosis, vol. 236, no. 2, pp. 448–455, 2014. View at Publisher · View at Google Scholar · View at Scopus
  131. J. A. Ronald, J. W. Chen, Y. Chen et al., “Enzyme-sensitive magnetic resonance imaging targeting myeloperoxidase identifies active inflammation in experimental rabbit atherosclerotic plaques,” Circulation, vol. 120, no. 7, pp. 592–599, 2009. View at Publisher · View at Google Scholar · View at Scopus
  132. M. Begum, J. Ashok Kumar, H. P. D'Souza et al., “Myeloperoxidase, malondialdehyde and serum lipids in type 2 diabetes mellitus,” Journal of Investigational Biochemistry, vol. 4, no. 1, pp. 13–17, 2015. View at Google Scholar
  133. Y. E. Eksi, Z. E. Karaali, K. Incekara, and H. A. Ergen, “Myeloperoxidase and glutamate-cysteine ligase polymorphisms in type 2 diabetes mellitus: a preliminary study,” Journal of Medical Biochemistry, vol. 33, no. 2, pp. 156–161, 2013. View at Publisher · View at Google Scholar · View at Scopus
  134. J. J. Wiersma, M. C. Meuwese, J. N. I. Van Miert et al., “Diabetes mellitus type 2 is associated with higher levels of myeloperoxidase,” Medical Science Monitor, vol. 14, no. 8, pp. CR406–CR410, 2008. View at Google Scholar · View at Scopus
  135. K. Uchimura, A. Nagasaka, R. Hayashi et al., “Changes in superoxide dismutase activities and concentrations and myeloperoxidase activities in leukocytes from patients with diabetes mellitus,” Journal of Diabetes and Its Complications, vol. 13, no. 5-6, pp. 264–270, 1999. View at Publisher · View at Google Scholar · View at Scopus
  136. S. Tzikas, D. Schlak, K. Sopova et al., “Increased myeloperoxidase plasma levels in patients with Alzheimer's disease,” Journal of Alzheimer's Disease, vol. 39, no. 3, pp. 557–564, 2014. View at Publisher · View at Google Scholar · View at Scopus
  137. R. A. Maki, V. A. Tyurin, R. C. Lyon et al., “Aberrant expression of myeloperoxidase in astrocytes promotes phospholipid oxidation and memory deficits in a mouse model of Alzheimer disease,” The Journal of Biological Chemistry, vol. 284, no. 5, pp. 3158–3169, 2009. View at Publisher · View at Google Scholar · View at Scopus
  138. P. S. Green, A. J. Mendez, J. S. Jacob et al., “Neuronal expression of myeloperoxidase is increased in Alzheimer's disease,” Journal of Neurochemistry, vol. 90, no. 3, pp. 724–733, 2004. View at Publisher · View at Google Scholar · View at Scopus
  139. D.-K. Choi, S. Pennathur, C. Perier et al., “Ablation of the inflammatory enzyme myeloperoxidase mitigates features of Parkinson's disease in mice,” The Journal of Neuroscience, vol. 25, no. 28, pp. 6594–6600, 2005. View at Publisher · View at Google Scholar · View at Scopus
  140. E. Gray, T. L. Thomas, S. Betmouni, N. Scolding, and S. Love, “Elevated activity and microglial expression of myeloperoxidase in demyelinated cerebral cortex in multiple sclerosis,” Brain Pathology, vol. 18, no. 1, pp. 86–95, 2008. View at Publisher · View at Google Scholar · View at Scopus
  141. R. M. Nagra, B. Becher, W. W. Tourtellotte et al., “Immunohistochemical and genetic evidence of myeloperoxidase involvement in multiple sclerosis,” Journal of Neuroimmunology, vol. 78, no. 1-2, pp. 97–107, 1997. View at Publisher · View at Google Scholar · View at Scopus
  142. R. W. Telles, G. A. Ferreira, N. P. Da Silva, and E. I. Sato, “Increased plasma myeloperoxidase levels in systemic lupus erythematosus,” Rheumatology International, vol. 30, no. 6, pp. 779–784, 2010. View at Publisher · View at Google Scholar · View at Scopus
  143. M. Koziol-Montewka, A. Kolodziejek, and J. Oles, “Study on myeloperoxidase role in antituberculous defense in the context of cytokine activation,” Inflammation, vol. 28, no. 2, pp. 53–58, 2004. View at Publisher · View at Google Scholar · View at Scopus
  144. A. Zhu, D. Ge, J. Zhang et al., “Sputum myeloperoxidase in chronic obstructive pulmonary disease,” European Journal of Medical Research, vol. 19, article 12, pp. 1–11, 2014. View at Publisher · View at Google Scholar · View at Scopus
  145. C. O'Donnell, P. Newbold, P. White, B. Thong, H. Stone, and R. A. Stockley, “3-Chlorotyrosine in sputum of COPD patients: relationship with airway inflammation,” COPD: Journal of Chronic Obstructive Pulmonary Disease, vol. 7, no. 6, pp. 411–417, 2010. View at Publisher · View at Google Scholar · View at Scopus
  146. V. M. Keatings and P. J. Barnes, “Granulocyte activation markers in induced sputum: comparison between chronic obstructive pulmonary disease, asthma, and normal subjects,” American Journal of Respiratory and Critical Care Medicine, vol. 155, no. 2, pp. 449–453, 1997. View at Publisher · View at Google Scholar · View at Scopus
  147. A. Van Der Vliet, M. N. Nguyen, M. K. Shigenaga, J. P. Eiserich, G. P. Marelich, and C. E. Cross, “Myeloperoxidase and protein oxidation in cystic fibrosis,” American Journal of Physiology—Lung Cellular and Molecular Physiology, vol. 279, no. 3, pp. L537–L546, 2000. View at Google Scholar · View at Scopus
  148. J. Schröter, R. Süß, and J. Schiller, “MALDI-TOF MS to monitor the kinetics of phospholipase A2-digestion of oxidized phospholipids,” Methods, vol. 104, pp. 41–47, 2016. View at Publisher · View at Google Scholar · View at Scopus
  149. F. Gruber, H. Mayer, B. Lengauer et al., “NF-E2-related factor 2 regulates the stress response to UVA-1-oxidized phospholipids in skin cells,” The FASEB Journal, vol. 24, no. 1, pp. 39–48, 2010. View at Publisher · View at Google Scholar · View at Scopus
  150. P. Bretscher, J. Egger, A. Shamshiev et al., “Phospholipid oxidation generates potent anti-inflammatory lipid mediators that mimic structurally related pro-resolving eicosanoids by activating Nrf2,” EMBO Molecular Medicine, vol. 7, no. 5, pp. 593–607, 2015. View at Publisher · View at Google Scholar · View at Scopus
  151. V. J. Hammond, A. H. Morgan, S. Lauder et al., “Novel keto-phospholipids are generated by monocytes and macrophages, detected in cystic fibrosis, and activate peroxisome proliferator-activated receptor-γ,” The Journal of Biological Chemistry, vol. 287, no. 50, pp. 41651–41666, 2012. View at Publisher · View at Google Scholar · View at Scopus
  152. A. Watson, N. Leitinger, and M. Navab, “Structural identification by mass spectrometry of oxidized phospholipids in minimally oxidized low density lipoprotein that induce monocyte/endothelial interactions,” Journal of Biological Chemistry, vol. 272, no. 21, pp. 13597–13607, 1997. View at Publisher · View at Google Scholar
  153. A. C. Carr, M. C. M. Vissers, N. M. Domigan, and C. C. Winterbourn, “Modification of red cell membrane lipids by hypochlorous acid and haemolysis by preformed lipid chlorohydrins,” Redox Report, vol. 3, no. 5-6, pp. 263–271, 1997. View at Publisher · View at Google Scholar · View at Scopus
  154. A. C. Carr, E. A. Decker, Y. Park, and B. Frei, “Comparison of low-density lipoprotein modification by myeloperoxidase-derived hypochlorous and hypobromous acids,” Free Radical Biology and Medicine, vol. 31, no. 1, pp. 62–72, 2001. View at Publisher · View at Google Scholar · View at Scopus
  155. M. C. M. Vissers, A. Stern, F. Kuypers, J. Van Den Berg, and C. C. Winterbourn, “Membrane changes associated with lysis of red blood cells by hypochlorous acid,” Free Radical Biology and Medicine, vol. 16, no. 6, pp. 703–712, 1994. View at Publisher · View at Google Scholar · View at Scopus
  156. M. C. M. Vissers, A. C. Carr, and C. C. Winterbourn, “Fatty acid chlorohydrins and bromohydrins are cytotoxic to human endothelial cells,” Redox Report, vol. 6, no. 1, pp. 49–56, 2001. View at Publisher · View at Google Scholar · View at Scopus
  157. M. C. M. Vissers, A. C. Carr, and A. L. P. Chapman, “Comparison of human red cell lysis by hypochlorous and hypobromous acids: insights into the mechanism of lysis,” Biochemical Journal, vol. 330, no. 1, pp. 131–138, 1998. View at Publisher · View at Google Scholar · View at Scopus
  158. G. Dever, L.-J. Stewart, A. R. Pitt, and C. M. Spickett, “Phospholipid chlorohydrins cause ATP depletion and toxicity in human myeloid cells,” FEBS Letters, vol. 540, no. 1–3, pp. 245–250, 2003. View at Publisher · View at Google Scholar · View at Scopus
  159. A. Robaszkiewicz, F. H. Greig, A. R. Pitt, C. M. Spickett, G. Bartosz, and M. Soszyński, “Effect of phosphatidylcholine chlorohydrins on human erythrocytes,” Chemistry and Physics of Lipids, vol. 163, no. 7, pp. 639–647, 2010. View at Publisher · View at Google Scholar · View at Scopus
  160. A. Robaszkiewicz, G. Bartosz, A. R. Pitt et al., “HOCl-modified phosphatidylcholines induce apoptosis and redox imbalance in HUVEC-ST cells,” Archives of Biochemistry and Biophysics, vol. 548, pp. 1–10, 2014. View at Publisher · View at Google Scholar · View at Scopus
  161. A. Robaszkiewicz, M. Pogorzelska, G. Bartosz, and M. Soszyński, “Chloric acid(I) affects antioxidant defense of lung epitelial cells,” Toxicology in Vitro, vol. 25, no. 7, pp. 1328–1334, 2011. View at Publisher · View at Google Scholar · View at Scopus
  162. N. Franco-Pons, J. Casas, G. Fabriàs et al., “Fat necrosis generates proinflammatory halogenated lipids during acute pancreatitis,” Annals of Surgery, vol. 257, no. 5, pp. 943–951, 2013. View at Publisher · View at Google Scholar · View at Scopus
  163. A. Petrelli and F. van Wijk, “CD8+ T cells in human autoimmune arthritis: the unusual suspects,” Nature Reviews Rheumatology, vol. 12, no. 7, pp. 421–428, 2016. View at Publisher · View at Google Scholar
  164. C. C. Winterbourn and A. J. Kettle, “Biomarkers of myeloperoxidase-derived hypochlorous acid,” Free Radical Biology and Medicine, vol. 29, no. 5, pp. 403–409, 2000. View at Publisher · View at Google Scholar · View at Scopus
  165. Y. Zhao, C. V. Forst, C. E. Sayegh, I.-M. Wang, X. Yang, and B. Zhang, “Molecular and genetic inflammation networks in major human diseases,” Molecular BioSystems, vol. 12, pp. 2318–2341, 2016. View at Publisher · View at Google Scholar
  166. E. Malle, G. Marsche, J. Arnhold, and M. J. Davies, “Modification of low-density lipoprotein by myeloperoxidase-derived oxidants and reagent hypochlorous acid,” Biochimica et Biophysica Acta—Molecular and Cell Biology of Lipids, vol. 1761, no. 4, pp. 392–415, 2006. View at Publisher · View at Google Scholar · View at Scopus
  167. M. G. Sorci-Thomas and M. J. Thomas, “Microdomains, inflammation, and atherosclerosis,” Circulation Research, vol. 118, no. 4, pp. 679–691, 2016. View at Publisher · View at Google Scholar · View at Scopus
  168. S. L. Hazen, F. F. Hsu, K. Duffin, and J. W. Heinecke, “Molecular chlorine generated by the myeloperoxidase-hydrogen peroxide-chloride system of phagocytes converts low density lipoprotein cholesterol into a family of chlorinated sterols,” The Journal of Biological Chemistry, vol. 271, no. 38, pp. 23080–23088, 1996. View at Publisher · View at Google Scholar · View at Scopus
  169. G. J. Dever, R. Benson, C. L. Wainwright, S. Kennedy, and C. M. Spickett, “Phospholipid chlorohydrin induces leukocyte adhesion to ApoE−/− mouse arteries via upregulation of P-selectin,” Free Radical Biology and Medicine, vol. 44, no. 3, pp. 452–463, 2008. View at Publisher · View at Google Scholar · View at Scopus
  170. J. Yang, Y. Cheng, R. Ji, and C. Zhang, “Novel model of inflammatory neointima formation reveals a potential role of myeloperoxidase in neointimal hyperplasia,” American Journal of Physiology—Heart and Circulatory Physiology, vol. 291, no. 6, pp. H3087–H3093, 2006. View at Publisher · View at Google Scholar · View at Scopus
  171. M. C. Messner, C. J. Albert, J. McHowat, and D. A. Ford, “Identification of lysophosphatidylcholine-chlorohydrin in human atherosclerotic lesions,” Lipids, vol. 43, no. 3, pp. 243–249, 2008. View at Publisher · View at Google Scholar · View at Scopus
  172. T. Matsumoto, T. Kobayashi, and K. Kamata, “Role of lysophosphatidylcholine (LPC) in atherosclerosis,” Current Medicinal Chemistry, vol. 14, no. 30, pp. 3209–3220, 2007. View at Publisher · View at Google Scholar · View at Scopus
  173. A. K. Thukkani, J. McHowat, F.-F. Hsu, M.-L. Brennan, S. L. Hazen, and D. A. Ford, “Identification of α-chloro fatty aldehydes and unsaturated lysophosphatidylcholine molecular species in human atherosclerotic lesions,” Circulation, vol. 108, no. 25, pp. 3128–3133, 2003. View at Publisher · View at Google Scholar · View at Scopus
  174. D. A. Ford, “Lipid oxidation by hypochlorous acid: chlorinated lipids in atherosclerosis and myocardial ischemia,” Clinical Lipidology, vol. 5, no. 6, pp. 835–852, 2010. View at Publisher · View at Google Scholar · View at Scopus
  175. O. A. Akerele and S. K. Cheema, “Fatty acyl composition of lysophosphatidylcholine is important in atherosclerosis,” Medical Hypotheses, vol. 85, no. 6, pp. 754–760, 2015. View at Publisher · View at Google Scholar · View at Scopus
  176. N. D. Hung, D.-E. Sok, and M. R. Kim, “Prevention of 1-palmitoyl lysophosphatidylcholine-induced inflammation by polyunsaturated acyl lysophosphatidylcholine,” Inflammation Research, vol. 61, no. 5, pp. 473–483, 2012. View at Publisher · View at Google Scholar · View at Scopus
  177. N. Aiyar, J. Disa, Z. Ao et al., “Lysophosphatidylcholine induces inflammatory activation of human coronary artery smooth muscle cells,” Molecular and Cellular Biochemistry, vol. 295, no. 1-2, pp. 113–120, 2007. View at Publisher · View at Google Scholar · View at Scopus
  178. K. A. Brown, “The polymorphonuclear cell in rheumatoid arthritis,” Rheumatology, vol. 27, no. 2, pp. 150–155, 1988. View at Publisher · View at Google Scholar · View at Scopus
  179. J. W. Hollingsworth, E. R. Siegel, and W. A. Creasey, “Granulocyte survival in synovial exudate of patients with rheumatoid arthritis and other inflammatory joint diseases,” Yale Journal of Biology and Medicine, vol. 39, no. 5, pp. 289–296, 1967. View at Google Scholar · View at Scopus
  180. A. Seven, S. Güzel, M. Aslan, and V. Hamuryudan, “Lipid, protein, DNA oxidation and antioxidant status in rheumatoid arthritis,” Clinical Biochemistry, vol. 41, no. 7-8, pp. 538–543, 2008. View at Publisher · View at Google Scholar · View at Scopus
  181. M. K. Kosinska, G. Liebisch, G. Lochnit et al., “A lipidomic study of phospholipid classes and species in human synovial fluid,” Arthritis & Rheumatism, vol. 65, no. 9, pp. 2323–2333, 2013. View at Publisher · View at Google Scholar · View at Scopus
  182. B. Fuchs, J. Schiller, U. Wagner, H. Häntzschel, and K. Arnold, “The phosphatidylcholine/lysophosphatidylcholine ratio in human plasma is an indicator of the severity of rheumatoid arthritis: investigations by 31P NMR and MALDI-TOF MS,” Clinical Biochemistry, vol. 38, no. 10, pp. 925–933, 2005. View at Publisher · View at Google Scholar · View at Scopus
  183. M. A. Duerr, R. Aurora, and D. A. Ford, “Identification of glutathione adducts of α-chlorofatty aldehydes produced in activated neutrophils,” Journal of Lipid Research, vol. 56, no. 5, pp. 1014–1024, 2015. View at Publisher · View at Google Scholar · View at Scopus
  184. B. Orosa, S. García, and C. Conde, “The autotaxin-lysophosphatidic acid pathway in pathogenesis of rheumatoid arthritis,” European Journal of Pharmacology, vol. 765, pp. 228–233, 2015. View at Publisher · View at Google Scholar · View at Scopus
  185. B. Orosa, S. García, P. Martínez, A. González, J. J. Gómez-Reino, and C. Conde, “Lysophosphatidic acid receptor inhibition as a new multipronged treatment for rheumatoid arthritis,” Annals of the Rheumatic Diseases, vol. 73, no. 1, pp. 298–305, 2014. View at Publisher · View at Google Scholar · View at Scopus
  186. I. Sevastou, E. Kaffe, M.-A. Mouratis, and V. Aidinis, “Lysoglycerophospholipids in chronic inflammatory disorders: the PLA2/LPC and ATX/LPA axes,” Biochimica et Biophysica Acta—Molecular and Cell Biology of Lipids, vol. 1831, no. 1, pp. 42–60, 2013. View at Publisher · View at Google Scholar · View at Scopus
  187. K. Moore and L. J. Roberts II, “Measurement of lipid peroxidation,” Free Radical Research, vol. 28, no. 6, pp. 659–671, 1998. View at Publisher · View at Google Scholar · View at Scopus
  188. K.-Y. Tserng and R. Griffin, “Quantitation and molecular species determination of diacylglycerols, phosphatidylcholines, ceramides, and sphingomyelins with gas chromatography,” Analytical Biochemistry, vol. 323, no. 1, pp. 84–93, 2003. View at Publisher · View at Google Scholar · View at Scopus
  189. O. Quehenberger, A. M. Armando, and E. A. Dennis, “High sensitivity quantitative lipidomics analysis of fatty acids in biological samples by gas chromatography-mass spectrometry,” Biochimica et Biophysica Acta—Molecular and Cell Biology of Lipids, vol. 1811, no. 11, pp. 648–656, 2011. View at Publisher · View at Google Scholar · View at Scopus
  190. G. Spiteller, “Linoleic acid peroxidation—the dominant lipid peroxidation process in low density lipoprotein-and its relationship to chronic diseases,” Chemistry and Physics of Lipids, vol. 95, no. 2, pp. 105–162, 1998. View at Publisher · View at Google Scholar · View at Scopus
  191. B. K. Wacker, C. J. Albert, B. A. Ford, and D. A. Ford, “Strategies for the analysis of chlorinated lipids in biological systems,” Free Radical Biology and Medicine, vol. 59, pp. 92–99, 2013. View at Publisher · View at Google Scholar · View at Scopus
  192. S. Tumanov, V. Bulusu, and J. J. Kamphorst, “Analysis of fatty acid Metabolism using stable isotope tracers and mass spectrometry,” Methods in Enzymology, vol. 561, pp. 197–217, 2015. View at Publisher · View at Google Scholar
  193. C. C. Winterbourn, J. J. M. van den Berg, E. Roitman, and F. A. Kuypers, “Chlorohydrin formation from unsaturated fatty acids reacted with hypochlorous acid,” Archives of Biochemistry and Biophysics, vol. 296, no. 2, pp. 547–555, 1992. View at Publisher · View at Google Scholar · View at Scopus
  194. A. C. Carr, J. J. M. van den Berg, and C. C. Winterbourn, “Chlorination of cholesterol in cell membranes by hypochlorous acid,” Archives of Biochemistry and Biophysics, vol. 332, no. 1, pp. 63–69, 1996. View at Publisher · View at Google Scholar · View at Scopus
  195. T. A. Isbell, R. Kleiman, and B. A. Plattner, “Acid-catalyzed condensation of oleic acid into estolides and polyestolides,” Journal of the American Oil Chemists' Society, vol. 71, no. 2, pp. 169–174, 1994. View at Publisher · View at Google Scholar · View at Scopus
  196. B. Fuchs, R. Süß, and J. Schiller, “An update of MALDI-TOF mass spectrometry in lipid research,” Progress in Lipid Research, vol. 49, no. 4, pp. 450–475, 2010. View at Publisher · View at Google Scholar · View at Scopus
  197. J. Arnhold, A. N. Osipov, H. Spalteholz, O. M. Panasenko, and J. Schiller, “Effects of hypochlorous acid on unsaturated phosphatidylcholines,” Free Radical Biology and Medicine, vol. 31, no. 9, pp. 1111–1119, 2001. View at Publisher · View at Google Scholar · View at Scopus
  198. J. Arnhold, A. N. Osipov, H. Spalteholz, O. M. Panasenko, and J. Schiller, “Formation of lysophospholipids from unsaturated phosphatidylcholines under the influence of hypochlorous acid,” Biochimica et Biophysica Acta—General Subjects, vol. 1572, no. 1, pp. 91–100, 2002. View at Publisher · View at Google Scholar · View at Scopus
  199. C. Schober, J. Schiller, F. Pinker, J. G. Hengstler, and B. Fuchs, “Lysophosphatidylethanolamine is—in contrast to—choline—generated under in vivo conditions exclusively by phospholipase A2 but not by hypochlorous acid,” Bioorganic Chemistry, vol. 37, no. 6, pp. 202–210, 2009. View at Google Scholar
  200. J. Wu, K. Teuber, M. Eibisch, B. Fuchs, and J. Schiller, “Chlorinated and brominated phosphatidylcholines are generated under the influence of the Fenton reagent at low pH—a MALDI-TOF MS study,” Chemistry and Physics of Lipids, vol. 164, no. 1, pp. 1–8, 2011. View at Publisher · View at Google Scholar · View at Scopus
  201. M. Saran, I. Beck-Speier, B. Fellerhoff, and G. Bauer, “Phagocytic killing of microorganisms by radical processes: consequences of the reaction of hydroxyl radicals with chloride yielding chlorine atoms,” Free Radical Biology and Medicine, vol. 26, no. 3-4, pp. 482–490, 1999. View at Publisher · View at Google Scholar · View at Scopus
  202. M. Saran and W. Bors, “Radiation chemistry of physiological saline reinvestigated: evidence that chloride-derived intermediates play a key role in cytotoxicity,” Radiation Research, vol. 147, no. 1, pp. 70–77, 1997. View at Publisher · View at Google Scholar · View at Scopus
  203. T. Jaskolla, B. Fuchs, M. Karas, and J. Schiller, “The new matrix 4-chloro-α-cyanocinnamic acid allows the detection of phosphatidylethanolamine chloramines by MALDI-TOF mass spectrometry,” Journal of the American Society for Mass Spectrometry, vol. 20, no. 5, pp. 867–874, 2009. View at Publisher · View at Google Scholar · View at Scopus
  204. M. B. O'Rourke, S. P. Djordjevic, and M. P. Padula, “The quest for improved reproducibility in MALDI mass spectrometry,” Mass Spectrometry Reviews, 2016. View at Publisher · View at Google Scholar
  205. M. Wang, C. Wang, R. H. Han, and X. Han, “Novel advances in shotgun lipidomics for biology and medicine,” Progress in Lipid Research, vol. 61, pp. 83–108, 2016. View at Publisher · View at Google Scholar
  206. J. Schiller, R. Süß, B. Fuchs, M. Müller, O. Zschörnig, and K. Arnold, “MALDI-TOF MS in lipidomics,” Frontiers in Bioscience, vol. 12, pp. 2568–2579, 2007. View at Google Scholar
  207. A. Jerlich, A. R. Pitt, R. J. Schaur, and C. M. Spickett, “Pathways of phospholipid oxidation by HOCl in human LDL detected by LC-MS,” Free Radical Biology and Medicine, vol. 28, no. 5, pp. 673–682, 2000. View at Publisher · View at Google Scholar · View at Scopus
  208. S. Miyamoto, G. R. Martinez, D. Rettori, O. Augusto, M. H. G. Medeiros, and P. Di Mascio, “Linoleic acid hydroperoxide reacts with hypochlorous acid, generating peroxyl radical intermediates and singlet molecular oxygen,” Proceedings of the National Academy of Sciences of the United States of America, vol. 103, no. 2, pp. 293–298, 2006. View at Publisher · View at Google Scholar · View at Scopus
  209. A. Jerlich, L. Horakova, J. S. Fabjan, A. Giessauf, G. Jürgens, and R. J. Schaur, “Correlation of low-density lipoprotein modification by myeloperoxidase with hypochlorous acid formation,” International Journal of Clinical & Laboratory Research, vol. 29, no. 4, pp. 155–161, 1999. View at Publisher · View at Google Scholar · View at Scopus
  210. A. Jerlich, R. J. Schaur, A. R. Pitt, and C. M. Spickett, “The formation of phosphatidylcholine oxidation products by stimulated phagocytes,” Free Radical Research, vol. 37, no. 6, pp. 645–653, 2003. View at Publisher · View at Google Scholar · View at Scopus
  211. C. J. Albert, D. S. Anbukumar, M. C. Messner, and D. A. Ford, “Chromatographic methods for the analyses of 2-halofatty aldehydes and chlorohydrin molecular species of lysophosphatidylcholine,” Journal of Chromatography B: Analytical Technologies in the Biomedical and Life Sciences, vol. 877, no. 26, pp. 2768–2777, 2009. View at Publisher · View at Google Scholar · View at Scopus
  212. F.-F. Hsu, J. Turk, A. K. Thukkani, M. C. Messner, K. R. Wildsmith, and D. A. Ford, “Characterization of alkylacyl, alk-1-enylacyl and lyso subclasses of glycerophosphocholine by tandem quadrupole mass spectrometry with electrospray ionization,” Journal of Mass Spectrometry, vol. 38, no. 7, pp. 752–763, 2003. View at Publisher · View at Google Scholar · View at Scopus
  213. W. C. Byrdwell, “Atmospheric pressure chemical ionization mass spectrometry for analysis of lipids,” Lipids, vol. 36, no. 4, pp. 327–346, 2001. View at Publisher · View at Google Scholar · View at Scopus
  214. A. Kuksis, J.-P. Suomela, M. Tarvainen, and H. Kallio, “Lipidomic analysis of glycerolipid and cholesteryl ester autooxidation products,” Molecular Biotechnology, vol. 42, no. 2, pp. 224–268, 2009. View at Publisher · View at Google Scholar · View at Scopus
  215. C. Mesaros, S. H. Lee, and I. A. Blair, “Targeted quantitative analysis of eicosanoid lipids in biological samples using liquid chromatography-tandem mass spectrometry,” Journal of Chromatography B: Analytical Technologies in the Biomedical and Life Sciences, vol. 877, no. 26, pp. 2736–2745, 2009. View at Publisher · View at Google Scholar · View at Scopus
  216. J. van den Berg and C. Winterbourn, “Measurement of reaction products from hypochlorous acid and unsaturated lipids,” Methods in Enzymology, vol. 233, pp. 639–649, 1994. View at Google Scholar
  217. O. M. Panasenko, J. Amhold, J. Schiller, K. Arnold, and V. I. Sergienko, “Peroxidation of egg yolk phosphatidylcholine liposomes by hypochlorous acid,” Biochimica et Biophysica Acta—Lipids and Lipid Metabolism, vol. 1215, no. 3, pp. 259–266, 1994. View at Publisher · View at Google Scholar · View at Scopus
  218. J. Schiller, M. Müller, B. Fuchs, K. Arnold, and D. Huster, “31P NMR spectroscopy of phospholipids: from micelles to membranes,” Current Analytical Chemistry, vol. 3, no. 4, pp. 283–301, 2007. View at Publisher · View at Google Scholar · View at Scopus
  219. R. Servaty, J. Schiller, H. Binder, B. Kohlstrunk, and K. Arnold, “IR and NMR studies on the action of hypochlorous acid on chondroitin sulfate and taurine,” Bioorganic Chemistry, vol. 26, no. 1, pp. 33–43, 1998. View at Publisher · View at Google Scholar
  220. E. L. Thomas, M. B. Grisham, and M. M. Jefferson, “Preparation and characterization of chloramines,” Methods in Enzymology, vol. 132, pp. 569–585, 1986. View at Publisher · View at Google Scholar
  221. B. Fuchs, R. Süß, K. Teuber, M. Eibisch, and J. Schiller, “Lipid analysis by thin-layer chromatography—a review of the current state,” Journal of Chromatography A, vol. 1218, no. 19, pp. 2754–2774, 2011. View at Publisher · View at Google Scholar · View at Scopus
  222. B. Fuchs, J. Schiller, R. Süß et al., “Analysis of stem cell lipids by offline HPTLC-MALDI-TOF MS,” Analytical and Bioanalytical Chemistry, vol. 392, no. 5, pp. 849–860, 2008. View at Publisher · View at Google Scholar · View at Scopus
  223. H. Jin, T. S. Hallstrand, D. S. Daly et al., “A halotyrosine antibody that detects increased protein modifications in asthma patients,” Journal of Immunological Methods, vol. 403, no. 1-2, pp. 17–25, 2014. View at Publisher · View at Google Scholar · View at Scopus
  224. R. J. Goiffon, S. C. Martinez, and D. Piwnica-Worms, “A rapid bioluminescence assay for measuring myeloperoxidase activity in human plasma,” Nature Communications, vol. 6, article 6271, 9 pages, 2015. View at Publisher · View at Google Scholar · View at Scopus
  225. N. M. Domigan, A. C. Carr, J. G. Lewis, P. A. Elder, and C. C. Winterbourn, “A monoclonal antibody recognizing the chlorohydrin derivatives of oleic acid for probing hypochlorous acid involvement in tissue injury,” Redox Report, vol. 3, no. 2, pp. 111–117, 1997. View at Publisher · View at Google Scholar · View at Scopus