Table of Contents Author Guidelines Submit a Manuscript
Oxidative Medicine and Cellular Longevity
Volume 2016, Article ID 6043038, 12 pages
http://dx.doi.org/10.1155/2016/6043038
Review Article

Hydrogen Sulfide and Cellular Redox Homeostasis

1Institute of Pharmacy & Pharmacology, University of South China, Hengyang, Hunan 421001, China
2Hunan Province Cooperative Innovation Center for Molecular Target New Drug Study, Hengyang, Hunan 421001, China
3Department of Pharmacology, Yong Loo Lin School of Medicine, National University of Singapore, Singapore 117597

Received 26 September 2015; Revised 23 November 2015; Accepted 1 December 2015

Academic Editor: Rodrigo Franco

Copyright © 2016 Zhi-Zhong Xie et al. 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

Intracellular redox imbalance is mainly caused by overproduction of reactive oxygen species (ROS) or weakness of the natural antioxidant defense system. It is involved in the pathophysiology of a wide array of human diseases. Hydrogen sulfide (H2S) is now recognized as the third “gasotransmitters” and proved to exert a wide range of physiological and cytoprotective functions in the biological systems. Among these functions, the role of H2S in oxidative stress has been one of the main focuses over years. However, the underlying mechanisms for the antioxidant effect of H2S are still poorly comprehended. This review presents an overview of the current understanding of H2S specially focusing on the new understanding and mechanisms of the antioxidant effects of H2S based on recent reports. Both inhibition of ROS generation and stimulation of antioxidants are discussed. H2S-induced S-sulfhydration of key proteins (e.g., p66Shc and Keap1) is also one of the focuses of this review.

1. Introduction

In 1777, a young Swedish apothecary, Carl Wilhelm Scheele, treated ferrous sulfide with a mineral acid and noted a colorless gas with a characteristic odor of rotten eggs. He described it as “sulfuretted hydrogen.” The notoriety of hydrogen sulfide (H2S) had been considered as a toxic gas for several hundreds of years. The Permissible Exposure Limit (PEL) of H2S is 10 ppm and sudden exposure to >400 ppm can cause rapid death. The biological effects of H2S in physiological condition began around the turn of the 20th century. H2S is now recognized as the third “gasotransmitter” along with nitric oxide (NO) and carbon monoxide (CO) [1]. The desulfhydration of cysteine is considered as the major source of H2S in mammals. This process is catalyzed by cystathionine β-synthase (CBS) and cystathionine γ-lyase (CSE), two pyridoxal-5′-phosphate- (PLP-) dependent enzymes. CBS is primarily expressed in various regions of the brain and is essential to the production of H2S in the central nervous system [24], whereas CSE is mainly expressed in the cardiovascular system [5, 6]. Recently, 3-mercaptopyruvate sulfurtransferase (3-MST) was reported as the third enzyme for H2S production, which is localized to mitochondria and nerve endings [7, 8]. We and others proved that H2S exerted a wide range of biological functions including neuroprotection [9, 10], cardioprotection [11, 12], antihypertension [13], and osteoblastic protection [14]. The antioxidant effect of H2S has been most extensively investigated and was thought as the major mechanism underlying the effects of H2S. Here, we summarize the existing knowledge about the antioxidant effect of H2S, highlighting recent advances in our understanding of the ability of H2S to neutralize reactive oxygen species (ROS) in vivo.

2. Free Radical, Oxidative Stress, and Cellular Antioxidant Defenses

2.1. Free Radical and Oxidative Stress

A free radical is an unstable chemical species that contains one or more unpaired electrons in its outer orbital. In organisms, the highly reactive free radicals formed from metabolism might donate their unpaired electron to another molecule or pull an electron off a neighboring molecule. The term oxidative stress has been proposed indicating a disturbance in the equilibrium status of oxidant/antioxidant systems with a progressive accumulation of ROS in intact cells. ROS are short-lived and highly chemically reactive. At low concentrations, ROS serve as cellular signaling molecules [15]. However, at high concentrations, ROS may cause both beneficial and unbeneficial effects. In the late case, ROS may not only kill invading pathogens and microbes but also damage the components of the cell, including proteins, lipids, carbohydrates, and DNA [16]. Overwhelming evidence indicates that oxidative stress is involved in the pathophysiology of the wide array of human diseases, including cancer [17], cardiovascular disease [18], AIDS [19], diabetes mellitus [20], and neurodegenerative disorders such as aging, Parkinson’s disease, and Alzheimer’s disease [21, 22].

In human body, more than 95% free radicals belong to oxygen free radicals. Recent studies suggest that oxygen-free radicals play an essential role in the control of cell functions and signal transmission [23, 24]. The common oxygen free radicals consist of superoxide anion (), hydroxyl radical (), perhydroxyl radical (), alkoxyl radical (), alkyl peroxide radical (), and so on (Table 1). Among them, is very unstable and able to react spontaneously with itself producing hydrogen peroxide (H2O2) and molecular oxygen (O2) [25]. is the starter of chain reaction of oxygen free radicals. is the most reactive oxygen free radical and can react with any biological molecule [26]. is the protonated form of superoxide anion and exhibits higher reactivity than superoxide anion [27]. In addition, other reactive oxygen metabolites such as H2O2 and the singlet oxygen () can also be regarded as oxygen free radicals, although they are not true free radical species. H2O2 may cross the biological membranes and is one of the origins of highly reactive [28]. The singlet oxygen () also has higher reactivity [29] and can be formed directly by illumination () from molecular oxygen.

Table 1: The types of common oxygen-free radicals.
2.2. The Sources of ROS

ROS are widespread in living organisms. Actually, they are being continuously produced in vivo and many of them are necessary to carry out certain cellular and biological reactions [23]. When they were overproduced, cellular damage may happen [30, 31]. The origin of oxygen-free radicals may be generated exogenously or endogenously.

Exogenous sources are mainly generated by some stimulating factors. These include smoking, alcohol, certain drugs, air pollution, ionizing radiation, and hyperbaric oxygen poisoning. Compared with exogenous sources, endogenous sources play more important roles in the form of oxygen free radicals. Endogenous activities are the main sources of oxygen-free radicals in living organisms. The main endogenous sources are listed below (Figure 1, solid line arrows).

Figure 1: The main ROS generation and elimination pathways. ROS (including , , , , and H2O2) may be generated by exogenous (like smoking, , air pollution, etc.) and endogenous (like mitochondria, catecholamine, NOX, etc.) stimulating factors. can further react with H2O2 to generate through the Haber-Weiss reaction in the presence of ferric irons (shown as solid line arrows). Excessive is eliminated by SOD by catalyzing the dismutation of to H2O2 and O2. H2O2 can be further removed by the catalysis of CAT or GPx. The catalysis of GPx needs GSH as its cosubstrate and GSH is oxidized to GSSG. GSSG can be reduced to GSH again by GR utilizing NADPH. GSH can also react with oxygen free radical directly and form the thiyl radical () and later GSSG. Vitamin E and vitamin C may react with oxygen free radical and form less reactive radicals (shown as dotted line arrows). NADPH: nicotinamide-adenine dinucleotide phosphate; NOX: NADPH oxidase; XO: xanthine oxidase; SOD: superoxide dismutase; GSH: glutathione; GSSG: glutathione disulfide; GPx: glutathione peroxidase; GR: glutathione reductase.

(i) Mitochondrial Electron Transport. The oxygen-free radical is the by-products of cellular metabolism. Under normal physiological conditions, most oxygen in organisms will acquire four electrons and four protons and reduce to form water by the cytochrome c oxidase from electron transport system of mitochondrial. In this procedure, no oxygen-free radical will form at last. However, if the molecular oxygen undergos sequential univalent reduction, highly reactive , , and H2O2 would be formed [32]. Mitochondria are the major source of intracellular ROS. As the terminal electron acceptor of respiration, more than 90% oxygen is used to produce ATP in mitochondria and about 2% of the oxygen is transformed into ROS as respiratory chain by-products [33].

(ii) The Increase of Xanthine Oxidase (XO). There are about 10% of xanthine oxidases (XO) and 90% of xanthine dehydrogenase (XD) in endothelial cells. The xanthine dehydrogenase (XD) will be converted into xanthine oxidase (XO) during ischaemia [34]. In this condition, the adenosine triphosphate (ATP) could not release energy. Instead, it will be degraded into adenosine diphosphate (ADP), adenosine monophosphate (AMP), and hypoxanthine gradually. Upon reperfusion of the ischemic tissue, increased xanthine oxidase (XO) will convert the increased hypoxanthine to xanthine and then convert the formed xanthine to uric acid by using oxygen as electron acceptor. Oxygen is reduced and produced , , and H2O2 finally [35] (Figure 2).

Figure 2: Endogenous superoxide anion () formation pathways. NOX catalyzes the one-electron reduction of oxygen to produce by utilizing NADPH as an electron donor.    formation in the process of the XO-catalyzed conversion of hypoxanthine into xanthine or xanthine into uric acid.    formation within catecholamine autooxidation.

(iii) The Increase of Catecholamine. Sympathetic adrenomedullary system is an important stress regulation system in our bodies. Catecholamine produced by this system under an external stimulus has an important role in the adjustment of metabolism. Catecholamine can also be converted to oxygen-free radicals by autooxidation [36] (Figure 2). It is worth noting that too much catecholamine and their oxidation products, especially the superoxide anion radicals, will cause damage to the body.

(iv) NADPH Oxidase. Nicotinamide-adenine dinucleotide phosphate (NADPH) oxidase (NOX) is another important enzyme for intracellular ROS generation. It is mainly distributed in the plasma membrane surface of phagocyte and catalyzes the one-electron reduction of oxygen to produce superoxide-free radical by utilizing NADPH as an electron donor (Figure 2). The NOX system is dormant in normal, but it can be activated by some stimulating factors, such as leukotriene, endotoxin, complement, and calcium ion [37, 38]. Thereby, more oxygen (O2) will be quickly reduced to and H2O2. will be also formed by further metabolism [39].

(v) Catalysis of Transitional Metals. The transitional metals, such as iron and copper, can change their valence by donating an electron and thus catalyze the Haber-Weiss reaction [28] as shown in (1). In the presence of superoxide anions, ferritin-bound ferric iron in cells usually can be liberated as ferrous form, thereby increasing the amount of iron [40]. The generated iron can form in the presence of hydrogen peroxide. This is the main source of hydroxyl radicals.

In addition, the metabolism of arachidonic acid by cyclooxygenase [41, 42] or lipoxygenases [43, 44], cytochromes P450 of the microsomal electron transport system [45, 46], may also produce oxygen-free radicals.

2.3. Cellular Defenses of ROS

In living organisms, ROS are continuously produced because of the reduction of molecular oxygen. Although free radicals play an important role in some physiological reactions, such as cell signal transduction and regulation of muscle tone [23, 40], excessive free radicals would cause damage to the lipids, proteins, and DNA and give rise to cellular and metabolic disturbance [30]. There are enzymes and chemical scavengers that could be used to remove excessive oxygen-free radicals formed in a living body [47].

Superoxide dismutase (SOD) is a common antioxidant enzyme which contains copper, zinc, and manganese as cofactors [48]. SOD can catalyze the dismutation of to molecular oxygen (O2) and the lesser active species H2O2 at a higher rate than the spontaneous dismutation of . The formed H2O2 will be further decomposed to H2O and O2 or be used to form through the Haber-Weiss reaction, as shown in (1), and reduced to H2O finally (Figure 1, dotted line arrows).

Catalase (CAT) is another antioxidant enzyme that is widely distributed in tissues [49]. It could catalyze the degradation of H2O2 directly to water and prevent the secondary generation of other intermediate radicals. In addition, selenium-containing glutathione peroxidase (GPx) could also catalyze the reduction of H2O2 [50]. This reaction needs reduced glutathione (GSH) as cosubstrate and GSH will be oxidized to oxidized glutathione (GSSG). GSSG could also be reduced to GSH again by glutathione reductase (GR) utilizing NADPH.

There are also some nonenzymatic chemical antioxidants that play an important role in antioxidant, included glutathione (GSH), α-tocopherol (vitamin E), and ascorbic acid (vitamin C) [51]. As mentioned before, GSH can act as a cosubstrate in the reduction of H2O2 by GPx. GSH could also react with oxygen-free radical directly and form the thiyl radical and later GSSG [52]. Like GSH, vitamins E and C could also reduce oxygen-free radicals [53]. They would trap hydroxyl radicals and other reactive radicals and thus break radical chain reactions and form new less reactive radicals. These new formed radicals themselves could not be removed or make further conversion. Only with the help of GPx and other biological molecules, these new radicals can be transformed to nonreactive substances. So, excess supplement of vitamins and other chemical antioxidants is not necessary. Excess levels of vitamins cannot replace the position of enzymes in organisms [54]. On the contrary, excess chemical antioxidants may produce excess less reactive radicals by reacting with oxygen radicals. These excess radicals may cause damage to the body. Actually, chemical antioxidants usually go into effect with the cooperation of antioxidant enzymes [55].

3. Mechanisms for the Regulatory Effect of H2S on ROS In Vivo

3.1. Quenching Free Radicals as a Chemical Reductant

At 37°C and pH 7.4, more than 80% of H2S molecules dissolve in surface waters and dissociate into H+, , and ions. is powerful one-electron chemical reluctant and presents a remarkable capacity to scavenge ROS. In addition, H2S itself has also been recognized to be a poor reducing agent, which can react directly with and quenches the superoxide anion () [56, 57] and NO-free radicals like peroxynitrite [58] as well as other ROS in vitro. However, it should be noted that the physiological concentration of H2S in vivo is believed to be at the submicromolar range [59, 60] and such low concentration of H2S is not paralleled with its antioxidant effect. Moreover, in our previous work, NaHS pretreatment significantly inhibited H2O2-induced (50 μM, 2 h) mitochondrial ROS generation and protected human neuroblastoma SH-SY5Y cells against H2O2-induced injury even when it had been washed out before H2O2 administration. Similar effects were also found in MC3T3-E1 osteoblastic cells, and this antioxidant effect of H2S lasted for at least 18 h [14]. These results indicated that other mechanisms besides chemical reductant exist in the antioxidant effect of H2S. We speculate that H2S might act as a trigger which will be retired after starting the process of antioxidant action.

3.2. Scavenging Free Radicals In Vivo via Nonenzymatic Antioxidants

As we mentioned before, ROS is counterbalanced in the body by a net of antioxidants, including enzymatic and nonenzymatic antioxidants. GSH and thioredoxin (Trx-1) are two biologically important nonenzymatic antioxidants in animal cells and attracted increasing attention as cellular protectants against oxidative stress in vivo.

3.2.1. H2S Increases Intracellular Reduced Glutathione (GSH)

GSH, a tripeptide consisting of cysteine, glutamate, and glycine, is a major antioxidant in the cellular defense against oxidative stress and a decreased GSH/GSSG ratio is usually taken as indicating oxidative stress. In cells, GSH is synthesized from cysteine. There are 2 cysteine forms, oxidized form cystine and reductive form cysteine. Because of its redox instability, extracellular cysteine is mostly present in cystine, which can be transported into cells through cystine/glutamate antiport system , then reduced to cysteine, and used for GSH synthesis [61]. Glutamate is the key inhibitor of the system . Our previous study showed that NaHS at 100 μM promoted [3H]glutamate uptake in astrocytes via enhancing the trafficking of glial glutamate transporter GLT-1 (also named the excitatory amino acid transporters-2, EAAT2), enhanced cystine transport, and increased intracellular GSH synthesis finally [62] (Figure 3).

Figure 3: H2S increases intracellular GSH synthesis. Cellular GSH is mainly synthesized from cysteine. H2S increases EAAT2-mediated glutamate uptake, which thereby increases cystine transportation through cystine/glutamate antiport system (). Intracellular H2S is released into extracellular space and reduces cystine into cysteine, which would be efficiently imported into cells through a cysteine transporter distinct from system . These two pathways provide more substrate to produce GSH. H2S increases glutamate cysteine ligase (GCL) expression and promotes GSH synthesis.

Studies from other laboratories have also proven that H2S preserves the cellular GSH status and provides protection against oxidative damage in brain [63, 64], spinal cord [65], heart [66, 67], lung [68], kidney [69, 70], liver [71], gastrointestinal tract [72, 73], and so forth. Recently, Kimura et al. showed a different mechanism for H2S on intracellular GSH production. They reported that H2S produced in cells may be released into extracellular space and reduces cystine into cysteine, which thereby would be efficiently imported into cells through a cysteine transporter distinct from system and used for GSH synthesis [74] (Figure 3). Meanwhile, Jain et al. also demonstrated that H2S increased intracellular GSH production by upregulating the glutamate-cysteine ligase catalytic subunit (GCLC) and glutamate-cysteine ligase modifier subunit (GCLM) [75] (Figure 3).

3.2.2. H2S Increases Intracellular Trx-1

Classic thioredoxin (Trx-1) is a small (12 kDa) ubiquitous molecule containing a characteristic Cys-Gly-Pro-Cys motif and the oxidation-reduction of Trx-1 occurs at its two cysteine residues. It was reported that Trx-1 exerts extracellular and intracellular multifunctions in cell proliferation [76], apoptosis [77], and gene expressions [78]. Moreover, Trx-1 was also shown to scavenge ROS and protect cells against oxidative stress. Trx-1 reduces hydrogen peroxide via peroxiredoxin (Prx) and oxidized Trx-1 is reduced by thioredoxin reductase [79]. Antioxidant effects of Trx-1 can also be mediated indirectly (for more details, see [79]).

In 2008, Jha et al. reported that H2S protected murine liver against ischemia-reperfusion (I/R) injury through upregulation of intracellular Trx-1 along with an increase in hepatic tissue GSH/GSSG ratio [71]. Trx-1 was also proved to mediate the cardioprotective effects of H2S in the setting of ischemic-induced heart failure by Nicholson et al. [80]. They demonstrated that Na2S treatment not only significantly increased the gene and protein expression of Trx-1 but also efficiently improved cardiac dilatation, dysfunction, and hypertrophy in the ischemic heart failure mice. Moreover, they generated transgenic mice with a cardiac-specific overexpression of a dominant negative mutant of Trx-1 and found the cardioprotective effects of Na2S were Trx-1 dependent.

3.2.3. Potential Mechanisms of H2S on Nonenzymatic Antioxidants Production

Despite the potential role of H2S in the cellular antioxidant defense, studies on its antioxidant mechanism have been exceptionally limited. Recently, increasing evidence revealed that Nrf2 participated in the antioxidant effect of H2S by promoting cellular antioxidant gene expression.

Nuclear factor (erythroid-derived 2)-like 2, also known as nuclear factor-erythroid 2 (NF-E2) related factor 2 (Nrf2), is a transcription factor that regulates a wide variety gene expression. Nrf2 is found mostly in the cytoplasm as an inactive complex with Kelch-like ECH-associated protein 1 (Keap1) [81]. Under oxidative stressed conditions, Keap1 undergoes ubiquitination and promotes Nrf2 translocation to the nucleus, in which Nrf2 binds to promoters containing the antioxidant response element (ARE) sequence and inducing ARE-dependent gene expression [82]. ARE is a cis-acting regulatory element, which is found in promoter region of certain genes, such as Trx-1 [83], glutathione reductase [84], and thioredoxin-interacting protein (Txnip) [85]. Nrf2 can suppress the basal expression of Txnip, which binds redox-active cysteine residues of Trx-1 and inhibit its antioxidant function [85]. Nrf2 can also increase both expression and activity of glutathione reductase, which, as we mentioned above, promotes oxidized GSH recycle back to reduced GSH and increases GSH/GSSG ratio [86]. On the other hand, it was reported that H2S can S-sulfhydrated Keap1 at cysteine-151, which causes a conformational change in Keap1 and thereby leads to Nrf2 dissociation from Keap1. The activated Nrf2 nuclear finally translocates to nuclear and promotes antioxidant gene transcription, such as GCLM, GCLC, and glutathione reductase (GR) [87]. In addition, Calvert et al. also demonstrated that H2S increased the expression of Trx-1 and mediated cardioprotection through Nrf2 signaling [83]. Taken together, these results demonstrate that Nrf2 is the potential endogenous cardioprotective signal in the process of cellular nonenzymatic antioxidant generation induced by H2S (Figure 4).

Figure 4: Effect of H2S on intracellular enzymatic and nonenzymatic antioxidant production. H2S activates Nrf2, which translocates to nuclear, binds to ARE, and upregulates enzymatic and nonenzymatic antioxidant production. H2S stimulates NF-κB signaling, which further upregulates the expression of numerous genes including SOD, CAT, and GPx.
3.3. Scavenging Free Radicals In Vivo via Enzymatic Antioxidants

Another major mechanism for cells to maintain redox equilibrium is based on the clearance ability processed by cellular antioxidant enzymes. Superoxide dismutase (SOD), CAT, and GPx are three main antioxidant enzymes that defend against oxidative damage in vivo. There are three isoforms of mammalian SOD: the cytosolic copper/zinc-containing SOD (Cu/ZnSOD, SOD-1), the mitochondrial manganese-containing SOD (MnSOD, SOD-2), and the extracellular SOD (ecSOD, SOD-3). SOD catalyzes the dismutation of into H2O2, while CAT reacts with H2O2 to form water and molecular oxygen, and GPx detoxifies H2O2 in the presence of GSH, producing H2O and GSSG which is recycled to GSH by glutathione reductase in an NADPH-consuming process [88] (Figure 1, dotted line arrows). In 1995, Searcy et al. reported that H2S is a genuine substrate of SOD and can bind at the catalytic Cu center of SOD [89]. The binding of to SOD is very quick and the rate constant for binding is >107. When sulfide combined with SOD, there was a synergistic increase in the rate of superoxide anion scavenging. The measured by the pyrogallol technique is ~80 μM [89]. Recent studies also demonstrated that H2S could ameliorate cellular oxidative stress by improving activities of CAT [66, 9092] and GPx [9295].

The signal transduction pathways for H2S to promote endogenous enzymatic antioxidant defense are much less understood. NF-κB is a family of transcription factors and plays a pivotal role in inflammation. H2S was reported to attenuate inflammation via inhibition of NF-κB activation, which is associated with an array of diseases, such as hypoxia-induced neurotoxicity [96], cerebral ischemia [97], kidney injury [98], pulmonary fibrosis [99], and acute pancreatitis [100]. However, as a redox-sensitive transcription factor, NF-κB has also been considered as the most important factor on regulation of cellular antioxidant enzymes and was reported to be upregulated by H2S via substance P [101, 102]. Analyzing the gene sequences of mouse GPx and CAT, Zhou et al. [103] revealed the existence of binding sites for NF-κB at position - in the GPx gene and at the - and - in the CAT gene. Additionally, SOD was also proved to have binding site for NF-κB in its 5′-flanking region and the DNA binding activity of NF-κB was induced in response to oxidative stress [104]. Taken together, these observations suggest that NF-κB mediated signaling pathway is most likely attributable to the augmentation of endogenous antioxidant capacity of H2S in response to oxidative stress (Figure 4).

In addition to the activation of NF-κB, Nrf2 signaling cascade maybe another rational that accounts for the antioxidant effect of H2S. Dreger et al. [105] identified that an ARE element existed in the SOD1 and CAT promoter, which is not only essential but also sufficient for transcriptional regulation. In their study, antioxidative enzymes in cardiac myocytes were induced via Nrf2-dependent transcriptional activation of ARE sites. On the other hand, diallyl sulfide (DAS), a kind of sulfur-containing compound, was demonstrated to cause a significant increase in the activities of SOD, CAT, GPx, GR, glutathione-S-transferase (GST), and quinone reductase (QR) in rat kidney through the activation of Nrf2 to protect the cell against oxidative stress [106]. This indicates a possible role of H2S in ROS-interacting enzymes synthesis. However, there is no direct report to link the effect of H2S on Nrf2 signal pathway to Nrf2-induced antioxidative enzymes synthesis at present and further investigations are needed in future.

3.4. Inhibitory Effect on Mitochondrial Free Radicals Production

Besides the capacity of cellular antioxidant defense, sequential overproduction of ROS is another vital factor in response to oxidative stress. Mitochondria is the major source of intracellular ROS and leak from the electron transfer chain is thought to be the main route [107]. Mounting evidence shows that p66Shc plays predominant roles in mitochondrial redox signaling and its phosphorylation at serine-36 acts as a switch on mitochondrial ROS production [108, 109].

p66Shc is a 66 kD Src homologous-collagen homologue (Shc) adaptor protein, which is encoded by the shc1 gene and belongs to the ShcA family. There are two other Shc family members, p46Shc and p52Shc, and all these 3 isoforms share three common functionally identical domains: the C-terminal Src homology 2 domain (SH2), the central collagen homology domain (CH1), and the N-terminal phosphor-tyrosine-binding domain (PTB) [110]. Different from the other two isoforms, p66Shc has an additional N-terminal CH2 domain which contains a critical serine residue at the position 36 (Ser-36) and shows different functions from p46Shc and p52Shc. It was proved that p66Shc has a negative influence on the Ras-mediated signaling pathway [111] but is involved in mitochondrial redox signaling. In response to oxidative stress (UV exposure or H2O2 treatment), p66Shc is phosphorylated by protein kinase C-βII () at Ser-36. The activated p66Shc is then isomerized by the prolyl isomerase Pin1 and dephosphorylated by phosphatase A2 (PP2A) and finally translocates to mitochondria, where it binds to cytochrome c and transfers electrons from cytochrome c to molecular oxygen to product ROS [112, 113] (Figure 5). Migliaccio et al. reported that mice have a 30% increase in the life span [114]. Consistent with this report, Tomilov et al. also demonstrated that macrophages from mice appeared to have defect in the activation of the NADPH oxidase and therefore less superoxide production was observed [115].

Figure 5: Proposed model for the effect of H2S on p66Shc mediated mitochondrial ROS generation. (a) Showing the effect of H2S. p66Shc is activated by -dependent phosphorylation at serine-36 in the N-terminal CH2 domain. The phosphorylated p66Shc can be isomerized by Pin1 and dephosphorylated by PP2A. This, in turn, induces mitochondrial translocation of p66Shc and ROS production. H2S sulfhydrates p66Shc at cysteine-59, which locates in the same CH2 domain besides serine-36, disrupts the association between and p66Shc, inhibits -mediated p66Shc phosphorylation, and decreases mitochondria ROS generation finally. (b) Showing the structure of p66Shc and the conserved serine (Ser-36) and cysteine (Cys-59) residues in the CH2 domain.

Recently, our group demonstrated for the first time that H2S may inhibit mitochondrial ROS production via a p66Shc-dependent signal transduction. Protein S-sulfhydration had been proposed to emerge as a major functional alteration of proteins, such as the potassium channels (like KATP, IKca, and SKca) [116], PTP1B [117], NF-κB [118], and Keap1 [87]. We proved that H2S sulfhydrated p66Shc at cysteine-59, which resides in the proximity to the phosphorylation sites serine-36. S-sulfhydration of p66Shc further impaired the association of and p66Shc, attenuated H2O2-induced p66Shc phosphorylation, and reduced mitochondrial ROS generation [119]. This new finding provides new insights and clues to better understand the important role of the H2S in oxidative stress and oxidative stress related disease (Figure 5).

4. Challenges and Conclusions

The antioxidant activity of H2S discussed in this review illuminated the biochemical mechanisms of H2S on cellular redox homeostasis. However, the effects of H2S on redox status are highly divergent. H2S was also reported as a powerful prooxidant, which kills cancer cells in a ROS-dependent manner [57]. It was believed that the Janus-faced molecule serves as an antioxidant or a prooxidant depending on its local concentrations. At lower concentrations, H2S exerts beneficial effects like protective effects in the cardiovascular system as we mentioned before, while at higher concentrations, H2S exhibits a variety of deleterious/cytotoxic effects (for more details, see [120]).

It should also be noted that the concentration- and time-dependent effects of H2S are very complicated. H2S was reported to display opposite effects at different concentrations/periods. GYY4137, a slow-releasing H2S donor, yielded very low concentrations of H2S and was proved to kill cancer cells. NaHS, which releases higher concentrations of H2S in short period, however, only exhibited weaker anticanner effect [121]. This may imply that both H2S releasing speed and amount are important for its therapeutic effects. Therefore, the biological functions of H2S should be studied in different pathological situations with varied concentrations and treatment periods. Endogenous H2S generating enzyme activities should also be taken into consideration, as they may be activated/inhibited upon cellular oxidative stress.

In summary, we discussed the current understanding of the antioxidant effect of H2S in this paper. Obviously, H2S does not produce antioxidant effect via a single/simple mechanism. Multiple targets and signaling pathways are involved. H2S can stimulate cellular enzymatic or nonenzymatic antioxidants to scavenge free radicals. This may be secondary to a direct effect on antioxidants or an indirect action through activation of various signaling proteins. H2S may also inhibit mitochondria ROS production through sulfhydration of p66Shc or membrane/cytosol ROS generation via inhibition of NADPH. To a weak extent, H2S also quenches free radicals directly due to its chemical reducing property. Future studies to explore more action sites of H2S in different signaling proteins and mechanisms underlying concentration- and time-dependent effects of H2S are still warranted.

Abbreviations

3-MST:3-Mercaptopyruvate sulfurtransferase
ADP:Adenosine diphosphate
AMP:Adenosine monophosphate
ARE:Antioxidant response element
ATP:Adenosine triphosphate
CAT:Catalase
CBS:Cystathionine β-synthase
CH1:collagen homology domain 1
CO:carbon monoxide
CSE:Cystathionine -lyase
DAS:Diallyl sulfide
GCLC:Glutamate-cysteine ligase catalytic subunit
GCLM:Glutamate-cysteine ligase modifier subunit
GPx:Glutathione peroxidase
GR:Glutathione reductase
GSH:Reduced glutathione
GSSG:Oxidized glutathione
GST:Glutathione-S-transferase
I/R:Ischemia-reperfusion
Keap1:Kelch-like ECH-associated protein 1
NO:Nitric oxide
Nrf2:Nuclear factor-erythroid 2 (NF-E2) related factor 2
P.E.L:Permissible Exposure Limit
Pin1:Prolyl isomerase
PP2A:Dephosphorylated by phosphatase A2
Prx:Peroxiredoxin
PTB:The phosphor-tyrosine-binding domain
QR:Quinone reductase
ROS:Reactive oxygen species
Shc:Src homologous-collagen
SOD:Superoxide dismutase
Trx-1:Thioredoxin 1
XD:Xanthine dehydrogenase
XO:Xanthine oxidase.

Conflict of Interests

The authors declare no conflict of interests to this work.

Acknowledgments

This work was supported by the Construct Program of the Key Discipline in Hunan Province and by the NUHS B2B Research Grant (NUHSRO/2011/012/STB/B2B-08).

References

  1. R. Wang, “The gasotransmitter role of hydrogen sulfide,” Antioxidants & Redox Signaling, vol. 5, no. 4, pp. 493–501, 2003. View at Publisher · View at Google Scholar · View at Scopus
  2. E. P. Kotsyuba, “Cystathionine β-synthase in the central nervous system of the shore crab Hemigrapsus sanguineus,” Doklady Biological Sciences, vol. 437, no. 1, pp. 94–96, 2011. View at Publisher · View at Google Scholar · View at Scopus
  3. V. M. Chertok, A. E. Kotsiuba, and E. P. Kotsiuba, “Cystathionine beta-synthase in the structural elements of the human brain and spinal cord,” Tsitologiia, vol. 53, pp. 665–670, 2011. View at Google Scholar
  4. K. Robert, F. Vialard, E. Thiery et al., “Expression of the cystathionine β synthase (CBS) gene during mouse development and immunolocalization in adult brain,” Journal of Histochemistry and Cytochemistry, vol. 51, no. 3, pp. 363–371, 2003. View at Publisher · View at Google Scholar · View at Scopus
  5. B. Geng, J. Yang, Y. Qi et al., “H2S generated by heart in rat and its effects on cardiac function,” Biochemical and Biophysical Research Communications, vol. 313, no. 2, pp. 362–368, 2004. View at Publisher · View at Google Scholar · View at Scopus
  6. P. K. Mishra, N. Tyagi, U. Sen, S. Givvimani, and S. C. Tyagi, “H2S ameliorates oxidative and proteolytic stresses and protects the heart against adverse remodeling in chronic heart failure,” American Journal of Physiology—Heart and Circulatory Physiology, vol. 298, no. 2, pp. H451–H456, 2010. View at Publisher · View at Google Scholar · View at Scopus
  7. N. Shibuya, M. Tanaka, M. Yoshida et al., “3-Mercaptopyruvate sulfurtransferase produces hydrogen sulfide and bound sulfane sulfur in the brain,” Antioxidants & Redox Signaling, vol. 11, no. 4, pp. 703–714, 2009. View at Publisher · View at Google Scholar · View at Scopus
  8. Y. Mikami, N. Shibuya, Y. Kimura, N. Nagahara, Y. Ogasawara, and H. Kimura, “Thioredoxin and dihydrolipoic acid are required for 3-mercaptopyruvate sulfurtransferase to produce hydrogen sulfide,” Biochemical Journal, vol. 439, no. 3, pp. 479–485, 2011. View at Publisher · View at Google Scholar · View at Scopus
  9. L.-F. Hu, M. Lu, C. X. Tiong, G. S. Dawe, G. Hu, and J.-S. Bian, “Neuroprotective effects of hydrogen sulfide on Parkinson's disease rat models,” Aging Cell, vol. 9, no. 2, pp. 135–146, 2010. View at Publisher · View at Google Scholar · View at Scopus
  10. M. Lu, F.-F. Zhao, J.-J. Tang et al., “The neuroprotection of hydrogen sulfide against MPTP-induced dopaminergic neuron degeneration involves uncoupling protein 2 rather than ATP-sensitive potassium channels,” Antioxidants & Redox Signaling, vol. 17, no. 6, pp. 849–859, 2012. View at Publisher · View at Google Scholar · View at Scopus
  11. T.-T. Pan, Y. Q. Chen, and J.-S. Bian, “All in the timing: a comparison between the cardioprotection induced by H2S preconditioning and post-infarction treatment,” European Journal of Pharmacology, vol. 616, no. 1–3, pp. 160–165, 2009. View at Publisher · View at Google Scholar · View at Scopus
  12. T.-T. Pan, Z.-N. Feng, S. W. Lee, P. K. Moore, and J.-S. Bian, “Endogenous hydrogen sulfide contributes to the cardioprotection by metabolic inhibition preconditioning in the rat ventricular myocytes,” Journal of Molecular and Cellular Cardiology, vol. 40, no. 1, pp. 119–130, 2006. View at Publisher · View at Google Scholar · View at Scopus
  13. M. Lu, Y.-H. Liu, H. S. Goh et al., “Hydrogen sulfide inhibits plasma renin activity,” Journal of the American Society of Nephrology, vol. 21, no. 6, pp. 993–1002, 2010. View at Publisher · View at Google Scholar · View at Scopus
  14. Z.-S. Xu, X.-Y. Wang, D.-M. Xiao et al., “Hydrogen sulfide protects MC3T3-E1 osteoblastic cells against H2O2-induced oxidative damage-implications for the treatment of osteoporosis,” Free Radical Biology and Medicine, vol. 50, no. 10, pp. 1314–1323, 2011. View at Publisher · View at Google Scholar · View at Scopus
  15. P. D. Ray, B.-W. Huang, and Y. Tsuji, “Reactive oxygen species (ROS) homeostasis and redox regulation in cellular signaling,” Cellular Signalling, vol. 24, no. 5, pp. 981–990, 2012. View at Publisher · View at Google Scholar · View at Scopus
  16. J. J. Ahire, N. U. Mokashe, H. J. Patil, and B. L. Chaudhari, “Antioxidative potential of folate producing probiotic Lactobacillus helveticus CD6,” Journal of Food Science and Technology, vol. 50, no. 1, pp. 26–34, 2013. View at Publisher · View at Google Scholar · View at Scopus
  17. A. Glasauer and N. S. Chandel, “Targeting antioxidants for cancer therapy,” Biochemical Pharmacology, vol. 92, no. 1, pp. 90–101, 2014. View at Publisher · View at Google Scholar · View at Scopus
  18. M. P. Sumandea and S. F. Steinberg, “Redox signaling and cardiac sarcomeres,” Journal of Biological Chemistry, vol. 286, no. 12, pp. 9921–9927, 2011. View at Publisher · View at Google Scholar · View at Scopus
  19. K. M. Porter and R. L. Sutliff, “HIV-1, reactive oxygen species, and vascular complications,” Free Radical Biology and Medicine, vol. 53, no. 1, pp. 143–159, 2012. View at Publisher · View at Google Scholar · View at Scopus
  20. C. Abe, Y. Uto, A. Kawasaki et al., “Evaluation of the in vivo antioxidative activity of redox nanoparticles by using a developing chicken egg as an alternative animal model,” Journal of Controlled Release, vol. 182, no. 1, pp. 67–72, 2014. View at Publisher · View at Google Scholar · View at Scopus
  21. K. Abe and H. Kimura, “The possible role of hydrogen sulfide as an endogenous neuromodulator,” Journal of Neuroscience, vol. 16, no. 3, pp. 1066–1071, 1996. View at Google Scholar · View at Scopus
  22. T. Kiyoshima, N. Enoki, I. Kobayashi et al., “Oxidative stress caused by a low concentration of hydrogen peroxide induces senescence-like changes in mouse gingival fibroblasts,” International Journal of Molecular Medicine, vol. 30, no. 5, pp. 1007–1012, 2012. View at Publisher · View at Google Scholar · View at Scopus
  23. W. Dröge, “Free radicals in the physiological control of cell function,” Physiological Reviews, vol. 82, no. 1, pp. 47–95, 2002. View at Publisher · View at Google Scholar · View at Scopus
  24. V. J. Thannickal and B. L. Fanburg, “Reactive oxygen species in cell signaling,” American Journal of Physiology—Lung Cellular and Molecular Physiology, vol. 279, no. 6, pp. L1005–L1028, 2000. View at Google Scholar · View at Scopus
  25. I. Fridovich, “Superoxide radical: an endogenous toxicant,” Annual Review of Pharmacology and Toxicology, vol. 23, pp. 239–257, 1983. View at Publisher · View at Google Scholar · View at Scopus
  26. F.-C. Cheng, J.-F. Jen, and T.-H. Tsai, “Hydroxyl radical in living systems and its separation methods,” Journal of Chromatography B: Analytical Technologies in the Biomedical and Life Sciences, vol. 781, no. 1-2, pp. 481–496, 2002. View at Publisher · View at Google Scholar · View at Scopus
  27. B. H. J. Bielski and D. E. Cabelli, “Highlights of current research involving superoxide and perhydroxyl radicals in aqueous solutions,” International Journal of Radiation Biology, vol. 59, no. 2, pp. 291–319, 1991. View at Publisher · View at Google Scholar · View at Scopus
  28. J. P. Kehrer, “The Haber-Weiss reaction and mechanisms of toxicity,” Toxicology, vol. 149, no. 1, pp. 43–50, 2000. View at Publisher · View at Google Scholar · View at Scopus
  29. B. Epe, “Genotoxicity of singlet oxygen,” Chemico-Biological Interactions, vol. 80, no. 3, pp. 239–260, 1991. View at Publisher · View at Google Scholar · View at Scopus
  30. B. A. Freeman and J. D. Crapo, “Biology of disease: free radicals and tissue injury,” Laboratory Investigation, vol. 47, no. 5, pp. 412–426, 1982. View at Google Scholar · View at Scopus
  31. M. Atalay and D. E. Laaksonen, “Diabetes, oxidative stress and physical exercise,” Journal of Sports Science and Medicine, vol. 1, no. 1, pp. 1–14, 2002. View at Google Scholar · View at Scopus
  32. J. F. Turrens, “Mitochondrial formation of reactive oxygen species,” The Journal of Physiology, vol. 552, no. 2, pp. 335–344, 2003. View at Publisher · View at Google Scholar · View at Scopus
  33. S. Perrin, J. Cremer, P. Roll et al., “Hiv-1 infection and first line art induced differential responses in mitochondria from blood lymphocytes and monocytes: the ANRS EP45 ‘Aging’ study,” PLoS ONE, vol. 7, no. 7, Article ID e41129, 2012. View at Publisher · View at Google Scholar · View at Scopus
  34. J. Čejková, T. Ardan, M. Filipec, and A. Midelfart, “Xanthine oxidoreductase and xanthine oxidase in human cornea,” Histology and Histopathology, vol. 17, no. 3, pp. 755–760, 2002. View at Google Scholar · View at Scopus
  35. F. Lacy, D. A. Gough, and G. W. Schmid-Schönbein, “Role of xanthine oxidase in hydrogen peroxide production,” Free Radical Biology and Medicine, vol. 25, no. 6, pp. 720–727, 1998. View at Publisher · View at Google Scholar · View at Scopus
  36. J. W. Miller, J. Selhub, and J. A. Joseph, “Oxidative damage caused by free radicals produced during catecholamine autoxidation: protective effects of O-methylation and melatonin,” Free Radical Biology and Medicine, vol. 21, no. 2, pp. 241–249, 1996. View at Publisher · View at Google Scholar · View at Scopus
  37. C. R. Hoyal, E. Gozal, H. Zhou, K. Foldenauer, and H. J. Forman, “Modulation of the rat alveolar macrophage respiratory burst by hydroperoxides is calcium dependent,” Archives of Biochemistry and Biophysics, vol. 326, no. 1, pp. 166–171, 1996. View at Publisher · View at Google Scholar · View at Scopus
  38. O. T. G. Jones, “The mechanism of the production of superoxide by phagocytes,” Molecular and Chemical Neuropathology, vol. 19, no. 1-2, pp. 177–184, 1993. View at Publisher · View at Google Scholar · View at Scopus
  39. M. S. Cohen, B. E. Britigan, D. J. Hassett, and G. M. Rosen, “Phagocytes, O2 reduction, and hydroxyl radical,” Reviews of Infectious Diseases, vol. 10, no. 6, pp. 1088–1096, 1988. View at Publisher · View at Google Scholar · View at Scopus
  40. S.-X. Chen and P. Schopfer, “Hydroxyl-radical production in physiological reactions. A novel function of peroxidase,” European Journal of Biochemistry, vol. 260, no. 3, pp. 726–735, 1999. View at Publisher · View at Google Scholar · View at Scopus
  41. M. Bakovic and H. B. Dunford, “Intimate relation between cyclooxygenase and peroxidase activities of prostaglandin H synthase. Peroxidase reaction of ferulic acid and its influence on the reaction of arachidonic acid,” Biochemistry, vol. 33, no. 21, pp. 6475–6482, 1994. View at Publisher · View at Google Scholar
  42. R. Dworski, J. R. Sheller, and B. W. Christman, “Quantitative analysis of cyclooxygenase metabolites of arachidonic acid,” in Human Airway Inflammation, vol. 56 of Methods in Molecular Medicine, pp. 411–422, Humana Press, 2001. View at Publisher · View at Google Scholar
  43. K. J. Kwon, Y.-S. Jung, S. H. Lee, C.-H. Moon, and E. J. Baik, “Arachidonic acid induces neuronal death through lipoxygenase and cytochrome P450 rather than cyclooxygenase,” Journal of Neuroscience Research, vol. 81, no. 1, pp. 73–84, 2005. View at Publisher · View at Google Scholar · View at Scopus
  44. Y. Nakamura, M. Kozuka, K. Naniwa et al., “Arachidonic acid cascade inhibitors modulate phorbol ester-induced oxidative stress in female ICR mouse skin: differential roles of 5-lipoxygenase and cyclooxygenase-2 in leukocyte infiltration and activation,” Free Radical Biology and Medicine, vol. 35, no. 9, pp. 997–1007, 2003. View at Publisher · View at Google Scholar · View at Scopus
  45. K. Sugioka and M. Nakano, “A possible mechanism of the generation of singlet molecular oxygen in NADPH-dependent microsomal lipid peroxidation,” Biochimica et Biophysica Acta—Bioenergetics, vol. 423, no. 2, pp. 203–216, 1976. View at Publisher · View at Google Scholar · View at Scopus
  46. V. Fernandez, X. Barrientos, K. Kipreos, A. Valenzuela, and L. A. Videla, “Superoxide radical generation, NADPH oxidase activity, and cytochrome P-450 content of rat liver microsomal fractions in an experimental hyperthyroid state: relation to lipid peroxidation,” Endocrinology, vol. 117, no. 2, pp. 496–501, 1985. View at Publisher · View at Google Scholar · View at Scopus
  47. M. Valko, D. Leibfritz, J. Moncol, M. T. D. Cronin, M. Mazur, and J. Telser, “Free radicals and antioxidants in normal physiological functions and human disease,” International Journal of Biochemistry and Cell Biology, vol. 39, no. 1, pp. 44–84, 2007. View at Publisher · View at Google Scholar · View at Scopus
  48. R. Noor, S. Mittal, and J. Iqbal, “Superoxide dismutase—applications and relevance to human diseases,” Medical Science Monitor, vol. 8, no. 9, pp. RA210–RA215, 2002. View at Google Scholar · View at Scopus
  49. V. I. Lushchak and D. V. Gospodaryov, “Catalases protect cellular proteins from oxidative modification in Saccharomyces cerevisiae,” Cell Biology International, vol. 29, no. 3, pp. 187–192, 2005. View at Publisher · View at Google Scholar · View at Scopus
  50. C. V. B. Prasad, M. V. Kodliwadmath, and G. B. Kodliwadmath, “Erythrocyte glutathione peroxidase, glutathione reductase activities and blood glutathione content in leprosy,” Journal of Infection, vol. 56, no. 6, pp. 469–473, 2008. View at Publisher · View at Google Scholar · View at Scopus
  51. L. Ong-awyooth, S. Ong-ajyooth, K. Tiensong, and S. Nilwarangkur, “Reduced free radical scavengers and chronic renal failure,” Journal of the Medical Association of Thailand, vol. 80, no. 2, pp. 101–108, 1997. View at Google Scholar
  52. A. Maranzana and R. J. Mehlhorn, “Loss of glutathione, ascorbate recycling, and free radical scavenging in human erythrocytes exposed to filtered cigarette smoke,” Archives of Biochemistry and Biophysics, vol. 350, no. 2, pp. 169–182, 1998. View at Publisher · View at Google Scholar · View at Scopus
  53. J. C. J. Chao, M.-D. Yuan, P.-Y. Chen, and S.-W. Chien, “Vitamin C and E supplements improve the impaired antioxidant status and decrease plasma lipid peroxides in hemodialysis patients,” Journal of Nutritional Biochemistry, vol. 13, no. 11, pp. 653–663, 2002. View at Publisher · View at Google Scholar · View at Scopus
  54. W.-H. Cheng, B. A. Valentine, and X. G. Lei, “High levels of dietary vitamin E do not replace cellular glutathione peroxidase in protecting mice from acute oxidative stress,” Journal of Nutrition, vol. 129, no. 11, pp. 1951–1957, 1999. View at Google Scholar · View at Scopus
  55. K. E. Hill and R. F. Burk, “Influence of vitamin E and selenium on glutathione-dependent protection against microsomal lipid peroxidation,” Biochemical Pharmacology, vol. 33, no. 7, pp. 1065–1068, 1984. View at Publisher · View at Google Scholar · View at Scopus
  56. M. R. Al-Magableh, B. K. Kemp-Harper, H. H. Ng, A. A. Miller, and J. L. Hart, “Hydrogen sulfide protects endothelial nitric oxide function under conditions of acute oxidative stress in vitro,” Naunyn-Schmiedeberg's Archives of Pharmacology, vol. 387, no. 1, pp. 67–74, 2014. View at Publisher · View at Google Scholar · View at Scopus
  57. B. L. Predmore, D. J. Lefer, and G. Gojon, “Hydrogen sulfide in biochemistry and medicine,” Antioxidants and Redox Signaling, vol. 17, no. 1, pp. 119–140, 2012. View at Publisher · View at Google Scholar · View at Scopus
  58. M. Whiteman, L. Li, I. Kostetski et al., “Evidence for the formation of a novel nitrosothiol from the gaseous mediators nitric oxide and hydrogen sulphide,” Biochemical and Biophysical Research Communications, vol. 343, no. 1, pp. 303–310, 2006. View at Publisher · View at Google Scholar · View at Scopus
  59. J. Furne, A. Saeed, and M. D. Levitt, “Whole tissue hydrogen sulfide concentrations are orders of magnitude lower than presently accepted values,” American Journal of Physiology—Regulatory Integrative and Comparative Physiology, vol. 295, no. 5, pp. R1479–R1485, 2008. View at Publisher · View at Google Scholar · View at Scopus
  60. M. Ishigami, K. Hiraki, K. Umemura, Y. Ogasawara, K. Ishii, and H. Kimura, “A source of hydrogen sulfide and a mechanism of its release in the brain,” Antioxidants and Redox Signaling, vol. 11, no. 2, pp. 205–214, 2009. View at Publisher · View at Google Scholar · View at Scopus
  61. J. Lewerenz, S. J. Hewett, Y. Huang et al., “The cystine/glutamate antiporter system XC- in health and disease: from molecular mechanisms to novel therapeutic opportunities,” Antioxidants & Redox Signaling, vol. 18, no. 5, pp. 522–555, 2013. View at Publisher · View at Google Scholar
  62. M. Lu, L.-F. Hu, G. Hu, and J.-S. Bian, “Hydrogen sulfide protects astrocytes against H2O2-induced neural injury via enhancing glutamate uptake,” Free Radical Biology and Medicine, vol. 45, no. 12, pp. 1705–1713, 2008. View at Publisher · View at Google Scholar · View at Scopus
  63. A. S. A. Majid, A. M. S. A. Majid, Z. Q. Yin, and D. Ji, “Slow regulated release of H2S inhibits oxidative stress induced cell death by influencing certain key signaling molecules,” Neurochemical Research, vol. 38, no. 7, pp. 1375–1393, 2013. View at Publisher · View at Google Scholar · View at Scopus
  64. N. Tyagi, K. S. Moshal, U. Sen et al., “H2S protects against methionine-induced oxidative stress in brain endothelial cells,” Antioxidants & Redox Signaling, vol. 11, no. 1, pp. 25–33, 2009. View at Publisher · View at Google Scholar · View at Scopus
  65. V. Kesherwani, K. S. Nelson, and S. K. Agrawal, “Effect of sodium hydrosulphide after acute compression injury of spinal cord,” Brain Research, vol. 1527, pp. 222–229, 2013. View at Publisher · View at Google Scholar · View at Scopus
  66. C. Huang, J. Kan, X. Liu et al., “Cardioprotective effects of a novel hydrogen sulfide agent-controlled release formulation of S-propargyl-cysteine on heart failure rats and molecular mechanisms,” PLoS ONE, vol. 8, no. 7, Article ID e69205, 2013. View at Publisher · View at Google Scholar · View at Scopus
  67. B. Sojitra, Y. Bulani, U. K. Putcha et al., “Nitric oxide synthase inhibition abrogates hydrogen sulfide-induced cardioprotection in mice,” Molecular and Cellular Biochemistry, vol. 360, no. 1-2, pp. 61–69, 2012. View at Publisher · View at Google Scholar · View at Scopus
  68. C. Wang, H.-Y. Wang, Z.-W. Liu, Y. Fu, and B. Zhao, “Effect of endogenous hydrogen sulfide on oxidative stress in oleic acid-induced acute lung injury in rats,” Chinese Medical Journal, vol. 124, no. 21, pp. 3476–3480, 2011. View at Publisher · View at Google Scholar · View at Scopus
  69. A. Otunctemur, E. Ozbek, M. Dursun et al., “Protective effect of hydrogen sulfide on gentamicin-induced renal injury,” Renal Failure, vol. 36, no. 6, pp. 925–931, 2014. View at Publisher · View at Google Scholar · View at Scopus
  70. U. Sen, P. Basu, O. A. Abe et al., “Hydrogen sulfide ameliorates hyperhomocysteinemia-associated chronic renal failure,” American Journal of Physiology—Renal Physiology, vol. 297, no. 2, pp. F410–F419, 2009. View at Publisher · View at Google Scholar · View at Scopus
  71. S. Jha, J. W. Calvert, M. R. Duranski, A. Ramachandran, and D. J. Lefer, “Hydrogen sulfide attenuates hepatic ischemia-reperfusion injury: role of antioxidant and antiapoptotic signaling,” The American Journal of Physiology—Heart and Circulatory Physiology, vol. 295, no. 2, pp. H801–H806, 2008. View at Publisher · View at Google Scholar · View at Scopus
  72. C. Guo, F. Liang, W. Shah Masood, and X. Yan, “Hydrogen sulfide protected gastric epithelial cell from ischemia/reperfusion injury by Keap1 s-sulfhydration, MAPK dependent anti-apoptosis and NF-κB dependent anti-inflammation pathway,” European Journal of Pharmacology, vol. 725, pp. 70–78, 2014. View at Publisher · View at Google Scholar · View at Scopus
  73. J. Cui, L. Liu, J. Zou et al., “Protective effect of endogenous hydrogen sulfide against oxidative stress in gastric ischemia-reperfusion injury,” Experimental and Therapeutic Medicine, vol. 5, no. 3, pp. 689–694, 2013. View at Publisher · View at Google Scholar · View at Scopus
  74. Y. Kimura, Y.-I. Goto, and H. Kimura, “Hydrogen sulfide increases glutathione production and suppresses oxidative stress in mitochondria,” Antioxidants and Redox Signaling, vol. 12, no. 1, pp. 1–13, 2010. View at Publisher · View at Google Scholar · View at Scopus
  75. S. K. Jain, L. Huning, and D. Micinski, “Hydrogen sulfide upregulates glutamate-cysteine ligase catalytic subunit, glutamate-cysteine ligase modifier subunit, and glutathione and inhibits interleukin-1beta secretion in monocytes exposed to high glucose levels,” Metabolic Syndrome and Related Disorders, vol. 12, no. 5, pp. 299–302, 2014. View at Publisher · View at Google Scholar · View at Scopus
  76. W. A. Chutkow and R. T. Lee, “Thioredoxin regulates adipogenesis through thioredoxin-interacting protein (Txnip) protein stability,” The Journal of Biological Chemistry, vol. 286, no. 33, pp. 29139–29145, 2011. View at Publisher · View at Google Scholar · View at Scopus
  77. M.-L. Moreno, J. Escobar, A. Izquierdo-Álvarez et al., “Disulfide stress: a novel type of oxidative stress in acute pancreatitis,” Free Radical Biology and Medicine, vol. 70, pp. 265–277, 2014. View at Publisher · View at Google Scholar · View at Scopus
  78. Y. Luo, F. He, L. Hu et al., “Transcription factor Ets1 regulates expression of thioredoxin-interacting protein and inhibits insulin secretion in pancreatic β-cells,” PLoS ONE, vol. 9, no. 6, Article ID e99049, 2014. View at Publisher · View at Google Scholar · View at Scopus
  79. J. Nordberg and E. S. J. Arnér, “Reactive oxygen species, antioxidants, and the mammalian thioredoxin system,” Free Radical Biology and Medicine, vol. 31, no. 11, pp. 1287–1312, 2001. View at Publisher · View at Google Scholar · View at Scopus
  80. C. K. Nicholson, J. P. Lambert, J. D. Molkentin, J. Sadoshima, and J. W. Calvert, “Thioredoxin 1 is essential for sodium sulfide-mediated cardioprotection in the setting of heart failure,” Arteriosclerosis, Thrombosis, and Vascular Biology, vol. 33, no. 4, pp. 744–751, 2013. View at Publisher · View at Google Scholar · View at Scopus
  81. H. M. Leinonen, E. Kansanen, P. Pölönen, M. Heinäniemi, and A.-L. Levonen, “Role of the keap1-Nrf2 pathway in cancer,” Advances in Cancer Research, vol. 122, pp. 281–320, 2014. View at Publisher · View at Google Scholar · View at Scopus
  82. L. Gan and J. A. Johnson, “Oxidative damage and the Nrf2-ARE pathway in neurodegenerative diseases,” Biochimica et Biophysica Acta (BBA)—Molecular Basis of Disease, vol. 1842, no. 8, pp. 1208–1218, 2014. View at Publisher · View at Google Scholar · View at Scopus
  83. J. W. Calvert, S. Jha, S. Gundewar et al., “Hydrogen sulfide mediates cardioprotection through Nrf2 signaling,” Circulation Research, vol. 105, no. 4, pp. 365–374, 2009. View at Publisher · View at Google Scholar · View at Scopus
  84. B. Gao, A. Doan, and B. M. Hybertson, “The clinical potential of influencing Nrf2 signaling in degenerative and immunological disorders,” Clinical Pharmacology, vol. 6, no. 1, pp. 19–34, 2014. View at Publisher · View at Google Scholar · View at Scopus
  85. X. He and Q. Ma, “Redox regulation by nuclear factor erythroid 2-related factor 2: gatekeeping for the basal and diabetes-induced expression of thioredoxin-interacting protein,” Molecular Pharmacology, vol. 82, no. 5, pp. 887–897, 2012. View at Publisher · View at Google Scholar · View at Scopus
  86. C. J. Harvey, R. K. Thimmulappa, A. Singh et al., “Nrf2-regulated glutathione recycling independent of biosynthesis is critical for cell survival during oxidative stress,” Free Radical Biology and Medicine, vol. 46, no. 4, pp. 443–453, 2009. View at Publisher · View at Google Scholar · View at Scopus
  87. G. Yang, K. Zhao, Y. Ju et al., “Hydrogen sulfide protects against cellular senescence via s-sulfhydration of keap1 and activation of Nrf2,” Antioxidants and Redox Signaling, vol. 18, no. 15, pp. 1906–1919, 2013. View at Publisher · View at Google Scholar · View at Scopus
  88. S. Wassmann, K. Wassmann, and G. Nickenig, “Modulation of oxidant and antioxidant enzyme expression and function in vascular cells,” Hypertension, vol. 44, no. 4, pp. 381–386, 2004. View at Publisher · View at Google Scholar · View at Scopus
  89. D. G. Searcy, J. P. Whitehead, and M. J. Maroney, “Interaction of Cu,Zn superoxide dismutase with hydrogen sulfide,” Archives of Biochemistry and Biophysics, vol. 318, no. 2, pp. 251–263, 1995. View at Publisher · View at Google Scholar · View at Scopus
  90. X. Zhu, Z. Tang, B. Cong et al., “Estrogens increase cystathionine-γ-lyase expression and decrease inflammation and oxidative stress in the myocardium of ovariectomized rats,” Menopause, vol. 20, no. 10, pp. 1084–1091, 2013. View at Publisher · View at Google Scholar · View at Scopus
  91. Z. Fu, X. Liu, B. Geng, L. Fang, and C. Tang, “Hydrogen sulfide protects rat lung from ischemia-reperfusion injury,” Life Sciences, vol. 82, no. 23-24, pp. 1196–1202, 2008. View at Publisher · View at Google Scholar · View at Scopus
  92. Y.-D. Wen, H. Wang, S.-H. Kho et al., “Hydrogen sulfide protects HUVECs against hydrogen peroxide induced mitochondrial dysfunction and oxidative stress,” PLoS ONE, vol. 8, no. 2, Article ID e53147, 2013. View at Publisher · View at Google Scholar · View at Scopus
  93. Y.-Y. Liu, B. V. Nagpure, P. T.-H. Wong, and J.-S. Bian, “Hydrogen sulfide protects SH-SY5Y neuronal cells against d-galactose induced cell injury by suppression of advanced glycation end products formation and oxidative stress,” Neurochemistry International, vol. 62, no. 5, pp. 603–609, 2013. View at Publisher · View at Google Scholar · View at Scopus
  94. L. R. Benetti, D. Campos, S. A. Gurgueira et al., “Hydrogen sulfide inhibits oxidative stress in lungs from allergic mice in vivo,” European Journal of Pharmacology, vol. 698, no. 1–3, pp. 463–469, 2013. View at Publisher · View at Google Scholar · View at Scopus
  95. Y.-W. Su, C. Liang, H.-F. Jin et al., “Hydrogen sulfide regulates cardiac function and structure in adriamycin-induced cardiomyopathy,” Circulation Journal, vol. 73, no. 4, pp. 741–749, 2009. View at Publisher · View at Google Scholar · View at Scopus
  96. Q. Zhang, L. Yuan, D. Liu et al., “Hydrogen sulfide attenuates hypoxia-induced neurotoxicity through inhibiting microglial activation,” Pharmacological Research, vol. 84, pp. 32–44, 2014. View at Publisher · View at Google Scholar · View at Scopus
  97. Y. Wang, J. Jia, G. Ao et al., “Hydrogen sulfide protects blood-brain barrier integrity following cerebral ischemia,” Journal of Neurochemistry, vol. 129, no. 5, pp. 827–838, 2014. View at Publisher · View at Google Scholar · View at Scopus
  98. X. Chen, W. Xu, Y. Wang et al., “Hydrogen sulfide reduces kidney injury due to urinary-derived sepsis by inhibiting NF-κB expression, decreasing TNF-α levels and increasing IL-10 levels,” Experimental and Therapeutic Medicine, vol. 8, no. 2, pp. 464–470, 2014. View at Publisher · View at Google Scholar · View at Scopus
  99. H. Cao, X. Zhou, J. Zhang et al., “Hydrogen sulfide protects against bleomycin-induced pulmonary fibrosis in rats by inhibiting NF-kappaB expression and regulating Th1/Th2 balance,” Toxicology Letters, vol. 224, no. 3, pp. 387–394, 2014. View at Publisher · View at Google Scholar · View at Scopus
  100. A. D. Ang, J. Rivers-Auty, A. Hegde, I. Ishii, and M. Bhatia, “The effect of CSE gene deletion in caerulein-induced acute pancreatitis in the mouse,” The American Journal of Physiology—Gastrointestinal and Liver Physiology, vol. 305, no. 10, pp. G712–G721, 2013. View at Publisher · View at Google Scholar · View at Scopus
  101. M. Bhatia, J. N. Sidhapuriwala, S. Wei Ng, R. Tamizhselvi, and S. M. Moochhala, “Pro-inflammatory effects of hydrogen sulphide on substance P in caerulein-induced acute pancreatitis,” Journal of Cellular and Molecular Medicine, vol. 12, no. 2, pp. 580–590, 2008. View at Publisher · View at Google Scholar · View at Scopus
  102. R. Tamizhselvi, P. Shrivastava, Y.-H. Koh, H. Zhang, and M. Bhatia, “Preprotachykinin-A gene deletion regulates hydrogen sulfide-induced Toll-like receptor 4 signaling pathway in cerulein-treated pancreatic acinar cells,” Pancreas, vol. 40, no. 3, pp. 444–452, 2011. View at Publisher · View at Google Scholar · View at Scopus
  103. L. Z.-H. Zhou, A. P. Johnson, and T. A. Rando, “NFκB and AP-1 mediate transcriptional responses to oxidative stress in skeletal muscle cells,” Free Radical Biology and Medicine, vol. 31, no. 11, pp. 1405–1416, 2001. View at Publisher · View at Google Scholar · View at Scopus
  104. H. T. Kim, Y. H. Kim, J. W. Nam, H. J. Lee, H. M. Rho, and G. Jung, “Study of 5′-flanking region of human Cu/Zn superoxide dismutase,” Biochemical and Biophysical Research Communications, vol. 201, no. 3, pp. 1526–1533, 1994. View at Publisher · View at Google Scholar · View at Scopus
  105. H. Dreger, K. Westphal, A. Weller et al., “Nrf2-dependent upregulation of antioxidative enzymes: a novel pathway for proteasome inhibitor-mediated cardioprotection,” Cardiovascular Research, vol. 83, no. 2, pp. 354–361, 2009. View at Publisher · View at Google Scholar · View at Scopus
  106. S. Kalayarasan, P. N. Prabhu, N. Sriram, R. Manikandan, M. Arumugam, and G. Sudhandiran, “Diallyl sulfide enhances antioxidants and inhibits inflammation through the activation of Nrf2 against gentamicin-induced nephrotoxicity in Wistar rats,” European Journal of Pharmacology, vol. 606, no. 1–3, pp. 162–171, 2009. View at Publisher · View at Google Scholar · View at Scopus
  107. L. A. Sena and N. S. Chandel, “Physiological roles of mitochondrial reactive oxygen species,” Molecular Cell, vol. 48, no. 2, pp. 158–167, 2012. View at Publisher · View at Google Scholar · View at Scopus
  108. E. R. Galimov, “The role of p66shc in oxidative stress and apoptosis,” Acta Naturae, vol. 2, pp. 44–51, 2010. View at Google Scholar
  109. M. Gertz and C. Steegborn, “The lifespan-regulator p66Shc in mitochondria: redox enzyme or redox sensor?” Antioxidants and Redox Signaling, vol. 13, no. 9, pp. 1417–1428, 2010. View at Publisher · View at Google Scholar · View at Scopus
  110. G. Pelicci, L. Dente, A. De Giuseppe et al., “A family of Shc related proteins with conserved PTB, CH1 and SH2 regions,” Oncogene, vol. 13, no. 3, pp. 633–641, 1996. View at Google Scholar · View at Scopus
  111. K. S. Ravichandran, “Signaling via Shc family adapter proteins,” Oncogene, vol. 20, no. 44, pp. 6322–6330, 2001. View at Publisher · View at Google Scholar · View at Scopus
  112. P. Pinton, A. Rimessi, S. Marchi et al., “Protein kinase C β and prolyl isomerase 1 regulate mitochondrial effects of the life-span determinant p66Shc,” Science, vol. 315, pp. 659–663, 2007. View at Publisher · View at Google Scholar · View at Scopus
  113. M. Giorgio, E. Migliaccio, F. Orsini et al., “Electron transfer between cytochrome c and p66Shc generates reactive oxygen species that trigger mitochondrial apoptosis,” Cell, vol. 122, no. 2, pp. 221–233, 2005. View at Publisher · View at Google Scholar · View at Scopus
  114. E. Migliaccio, M. Giogio, S. Mele et al., “The p66shc adaptor protein controls oxidative stress response and life span in mammals,” Nature, vol. 402, no. 6759, pp. 309–313, 1999. View at Publisher · View at Google Scholar · View at Scopus
  115. A. A. Tomilov, V. Bicocca, R. A. Schoenfeld et al., “Decreased superoxide production in macrophages of long-lived p66Shc knock-out mice,” The Journal of Biological Chemistry, vol. 285, no. 2, pp. 1153–1165, 2010. View at Publisher · View at Google Scholar · View at Scopus
  116. A. K. Mustafa, G. Sikka, S. K. Gazi et al., “Hydrogen sulfide as endothelium-derived hyperpolarizing factor sulfhydrates potassium channels,” Circulation Research, vol. 109, no. 11, pp. 1259–1268, 2011. View at Publisher · View at Google Scholar · View at Scopus
  117. N. Krishnan, C. Fu, D. J. Pappin, and N. K. Tonks, “H2S-induced sulfhydration of the phosphatase PTP1B and its role in the endoplasmic reticulum stress response,” Science Signaling, vol. 4, article ra86, 2011. View at Publisher · View at Google Scholar · View at Scopus
  118. N. Sen, B. D. Paul, M. M. Gadalla et al., “Hydrogen sulfide-linked sulfhydration of NF-κB mediates its antiapoptotic actions,” Molecular Cell, vol. 45, no. 1, pp. 13–24, 2012. View at Publisher · View at Google Scholar · View at Scopus
  119. Z.-Z. Xie, M.-M. Shi, L. Xie et al., “Sulfhydration of p66Shc at Cysteine59 mediates the antioxidant effect of hydrogen sulfide,” Antioxidants and Redox Signaling, vol. 21, no. 18, pp. 2531–2542, 2014. View at Publisher · View at Google Scholar · View at Scopus
  120. C. Szabo, C. Ransy, K. Módis et al., “Regulation of mitochondrial bioenergetic function by hydrogen sulfide. Part I. Biochemical and physiological mechanisms,” British Journal of Pharmacology, vol. 171, no. 8, pp. 2099–2122, 2014. View at Publisher · View at Google Scholar · View at Scopus
  121. Z. W. Lee, J. Zhou, C.-S. Chen et al., “The slow-releasing Hydrogen Sulfide donor, GYY4137, exhibits novel anti-cancer effects in vitro and in vivo,” PLoS ONE, vol. 6, no. 6, Article ID e21077, 2011. View at Publisher · View at Google Scholar · View at Scopus