Nitric Oxide Inactivation Mechanisms in the Brain: Role in Bioenergetics and Neurodegeneration

Santos, Ricardo M.; Lourenço, Cátia F.; Ledo, Ana; Barbosa, Rui M.; Laranjinha, João

doi:https://doi.org/10.1155/2012/391914

International Journal of Cell Biology

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Volume 2012 | Article ID 391914 | https://doi.org/10.1155/2012/391914

Nitric Oxide Inactivation Mechanisms in the Brain: Role in Bioenergetics and Neurodegeneration

Ricardo M. Santos,¹Cátia F. Lourenço,¹Ana Ledo,¹Rui M. Barbosa,¹and João Laranjinha¹

Academic Editor: Juan P. Bolaños

Received27 Mar 2012

Accepted18 Apr 2012

Published10 Jun 2012

Abstract

During the last decades nitric oxide (^•NO) has emerged as a critical physiological signaling molecule in mammalian tissues, notably in the brain. ^•NO may modify the activity of regulatory proteins via direct reaction with the heme moiety, or indirectly, via S-nitrosylation of thiol groups or nitration of tyrosine residues. However, a conceptual understanding of how ^•NO bioactivity is carried out in biological systems is hampered by the lack of knowledge on its dynamics in vivo. Key questions still lacking concrete and definitive answers include those related with quantitative issues of its concentration dynamics and diffusion, summarized in the how much, how long, and how far trilogy. For instance, a major problem is the lack of knowledge of what constitutes a physiological ^•NO concentration and what constitutes a pathological one and how is ^•NO concentration regulated. The ambient ^•NO concentration reflects the balance between the rate of synthesis and the rate of breakdown. Much has been learnt about the mechanism of ^•NO synthesis, but the inactivation pathways of ^•NO has been almost completely ignored. We have recently addressed these issues in vivo on basis of microelectrode technology that allows a fine-tuned spatial and temporal measurement ^•NO concentration dynamics in the brain.

1. Introduction

Nitric oxide (^•NO) is a small and diffusible free radical synthesized by a family of nitric oxide synthases (NOS) that participates in a wide range of signaling pathways in biological tissues, mediating physiologic processes such as vasodilation, memory and learning, neuronal development, regulation of immune response, among many others [1–5]. In the brain, ^•NO is mainly synthesized in synaptic terminals by a neuronal NOS isoform, acting as a neuromodulator [3, 4]. The radical nature, small size, and hydrophobicity support the notion that ^•NO lacks specific interactions with receptors, and yet these properties confer to this molecule a great versatility concerning interactions with biological targets. The outcome of these interactions is dictated by ^•NO concentration dynamics, ranging from physiological to pathological effects leading to cell death. This dual role anticipates a tight regulation of ^•NO concentration dynamics under physiologic conditions.

The major aspects that characterize ^•NO neuroactivity and its regulation are discussed in this paper.

2. The Interactions of ^•NO with Biological Targets: Redox and Functional Impact

Nitric oxide is able to rapidly diffuse in tissue and interact with a variety of biological targets involved in relevant physiological processes. Two main mechanisms that stabilize the unpaired electron of ^•NO are its reaction with other free radicals and interactions with d-orbitals of transition metals [6]. Among the latter, the interactions of ^•NO with iron are the most relevant in biological systems due to the abundance of proteins containing iron, most notably hemeproteins, involved in numerous physiological processes. Essentially, ^•NO can interact with iron complexes by three ways: (a) binding to iron, (b) reaction with dioxygen iron complexes, and (c) reaction with high valent oxo-complexes [7]. ^•NO can bind to both ferrous and ferric heme proteins, but the binding to Fe(II) is generally faster and more reversible than to Fe(III) [8]. Actually, the majority of biologically relevant ^•NO reactions with heme proteins involve the reversible binding of ^•NO to ferrous iron in proteins, a process called nitrosylation [7]. For instance, the binding of ^•NO to ferrous heme activates the enzyme soluble guanylyl cyclase (sGC) [3], which is the best characterized signaling target of ^•NO and inhibits cytochrome c oxidase (CcO), a crucial enzyme for mitochondrial respiration [9]. The interaction between ^•NO and ferrous hemoglobin is also biologically relevant by binding to the deoxy-hemoglobin heme or as a means to degrade ^•NO via reaction with oxy-hemoglobin, resulting in the oxidation of the ferrous heme and formation of nitrate.

These interactions are relatively fast, exhibiting rate constants of M⁻¹ s⁻¹ [8]. Given the abundance of hemoglobin in the vasculature, they constitute the main pathway of ^•NO removal in that compartment and significantly contribute to shape the dynamics of ^•NO at the neighboring tissues [10].

A critical aspect of the interactions of ^•NO with hemeproteins able to transduce a transient ^•NO concentration change into a biological response is their different sensitivity for ^•NO. The most sensitive ^•NO physiologic signaling target is sGC with half-maximal activation at 10 nM [11], mediating most of the known ^•NO biological effects [3]. For higher ^•NO concentrations inhibition of CcO occurs, being half-maximal at ≈120 nM, under resting metabolic conditions and physiological O₂ tension [9, 12].

The indirect effects of ^•NO require it to react with molecular oxygen or superoxide anion radical () to produce reactive oxygen and nitrogen species (RONS) such as nitrogen dioxide (^•NO₂), nitrogen trioxide (N₂O₃), and peroxynitrite (ONOO⁻). ONOO⁻ and ^•NO₂ are potent oxidants (>1.0 V NHE) [13] and can both oxidize and nitrate protein residues and lipids. The product of ^•NO autooxidation, N₂O₃, is a mild oxidant and will preferably nitrosate nucleophiles such as amines and thiols [14, 15].

S-Nitrosation is a covalent posttranslational modification associated to ^•NO-dependent signaling, which refers to the incorporation of a nitroso group (–NO) to a thiol group (in cystein residues). There are several mechanisms by which S-nitrosation can occur, mainly through (a) involvement of N₂O₃, (b) direct interaction of ^•NO with a thiyl radical (radical-radical interaction), and (c) transfer of a nitroso group from a nitrosylated metal or nitrosothiol (transnitrosation) [16]. S-Nitrosation mediated by N₂O₃ somehow defines the microenvironment in which the modification predominantly occurs. Because the reaction of ^•NO with O₂ is slow, it requires high levels of both species, a condition favored by the proximity of sources of ^•NO production and by hydrophobic environment (where both species accumulate). Also, the life time of N₂O₃ is increased in hydrophobic compartments [7]. These factors limit S-nitrosation and confer selectivity to the reaction as only cysteine residues found within a particular microenvironment in a protein are prone to be nitrosated (reviewed by [17]).

Several proteins have been described as being regulated by S-Nitrosation and ensued physiologic and pathologic consequences described [18, 19]. To mention some, S-nitrosation of N-methyl-D-aspartate receptors (NMDAr) has been shown to inactivate the receptor, thereby possibly protecting against excessive NMDAr activation and consequent excitotoxicity [20]. SNitrosation of 2-amino-3-(5-methyl-3-oxo-1,2-oxazol-4-yl)propanoic acid receptor (AMPAr) regulatory proteins (stargazin and Nethylmaleimide-sensitive factor) may increase surface expression of the receptor [21, 22]. Other examples include nitrosation of caspases-3 and -8 and poly(ADP-ribose) polymerase [23–25], protecting against apoptosis. In turn, S-nitrosation of glyceraldehyde-3-phosphate dehydrogenase (GAPDH) inhibits its dehydrogenase activity and induces an acyl phosphatase activity in the enzyme, resulting in the uncoupling of glycolytic flux from ATP synthesis [26]. Nitrosated GAPDH can also translocate to the nucleus, enabling it to degrade selected target proteins and affect apoptosis [27].

The nitration of proteins and lipids by ^•NO-derived reactive species is a further posttranslational modification of proteins by which ^•NO can accomplish functional diversity in cellular processes. It is currently accepted that protein nitration is an in vivo protein modification that translates into functional alterations in physiological and pathological settings [28]. Nitration results from the addition of a nitro –NO₂ group to aromatic and aliphatic residues in proteins or to the aliphatic chain of fatty acids, mainly mediated by ONOO⁻ and ^•NO₂. In proteins, tyrosine residues are the key target for nitration by ONOO⁻ (reviewed in [29]). 3-Nitrotyrosine (3-NT) has been used as a marker of pathological events associated to oxidative stress. Indeed, 3-NT immunoreactivity has been found in early stages of several neurodegenerative disorders in human autopsy samples as well as in animal models (reviewed in [28, 30]).

Protein nitration is a very selective modification. Not all tyrosine residues present in a given protein can suffer nitration. Protein folding, the surrounding local environment (namely, the presence of glutamate residues), and the nitration agent all contribute to direct nitration towards specific tyrosine residues [31]. Examples of nitration targets with relevance in the context of the nervous system and neurodegeneration may include the following: (1) neurofilament L in human ALS neurons, preventing assembly and possibly axonal transport, both pathological hallmarks of ALS [32–34]; (2) tyrosine hydroxylase, the rate-limiting enzyme in catecholamine synthesis, causing loss of enzyme function in the MPTP-induced Parkinson’s disease model [35–37], affording a possible cause of dopamine deficiency prior to cell death; (3) nitration of Mn superoxide dismutase inactivates this mitochondrial antioxidant enzyme, with implications several disease states (reviewed in [38]); (4) Lewy bodies in Parkinson’s disease have been found to contain nitrated alfa-synuclein, which tends to form oligomers [39].

In sum, at low ^•NO concentrations, direct ^•NO interactions with transition metal centers via reversible binding are likely to predominate as a physiological signal transduction mechanism.

On the other hand, the actual concentration at which ^•NO-dependent nitrosative and nitrative chemistry occurs, either from a physiological or deleterious view point, is not known and likely depends on the particular tissue redox conditions. A rough estimate has been made in cellular preparations, indicating that nitrosative stress becomes significant when the ^•NO concentration reaches near-micromolar levels [5, 40].

From the lines of evidence shown above it becomes clear that the concentration dynamics of ^•NO (the profile of change in time and space) is an essential aspect of its biology. Nitric oxide signals, having different amplitude, time course, and spatial distribution may thus encode different signaling messages, possibly mediated by different biological targets. Paradoxically, in spite of being one of the most studied endogenous molecules during the last decades, the exceeding majority of studies are of qualitative and phenomenological nature, lacking the critical quantitative information on ^•NO dynamics. Under this scenario it is not a surprise that several dogmas have undermined the knowledge of ^•NO biological actions.

Therefore, the monitoring of ^•NO concentration profiles in vivo, allowing to unravel its endogenous concentration profiles and the major factors regulating its concentration, is a critical piece of knowledge to understand the mechanisms by which ^•NO affects cell and tissue function in the brain.

3. The Transient ^•NO Change from the Background and the Mechanisms That Regulate Its Profile

3.1. ^•NO Production in the Brain

The ^•NO signaling in CNS is intimately associated to the glutamate system. In glutamatergic synapses, ^•NO synthesis involves the stimulation of ionotropic glutamate receptors (iGluR), particularly NMDA subtype, and consequent influx of Ca²⁺ to the cytosol that, upon binding to calmodulin, activates neuronal isoform of NOS (nNOS). The α-splice variant of nNOS is particular in that it possesses an N-terminal PDZ motif [41], which allows the enzyme to bind to other PDZ-containing proteins, such as the synaptic density scaffold protein PSD-95 [42]. The functional impact of this association is very relevant, as PSD-95 simultaneously binds to the NR2 subunit of the NMDAr [43, 44], thus forming a supramolecular complex that places the Ca²⁺-dependent nNOS under the direct effect of Ca²⁺ influx through the activated NMDAr channel [45]. Upon Ca²⁺ influx, providing that substrates (L-arginine, O₂) and several other cofactors (NADPH, FMN, FAD, tetrahydrobiopterin, heme) are available, nNOS catalyses the conversion of L-arginine to L-citrulline and ^•NO [46, 47]. However, the regulation of ^•NO synthesis by nNOS goes beyond Ca²⁺ dynamics, also involving, among other factors, specific adaptor proteins [48] and posttranslational modifications [49, 50]. In addition to the diverse regulatory mechanisms associated to ^•NO synthesis, the distribution of nNOS within a particular volume is suggested to influence the ^•NO volume signaling [51]. In essence, the abovementioned notions suggest an intricate regulatory process for ^•NO production that may translate into distinct concentration dynamics.

3.1.1. Measurement of Nitric Oxide Concentration Dynamics In Vitro and In Vivo

The measurement of ^•NO in real time by electrochemical methods with microelectrodes inserted into the ^•NO diffusion field is an important tool to characterize ^•NO concentration dynamics [52]. Glutamate-dependent ^•NO production in hippocampus is of particular relevance because of the involvement of ^•NO in the regulation of plasticity, such as learning and memory, and cell death associated with neurodegeneration [53]. Electrochemical detection presents several advantages in relation to other methods to measure ^•NO in biological systems, as it allows direct and real-time measurement. Moreover, the small size of the carbon fiber microelectrodes affords their use in nervous tissue, with minimal perturbation of the natural environment, and confers high spatial resolution to the measurements [54, 55].

In hippocampal slices, chemically modified carbon fiber microelectrodes with suitable analytical properties for ^•NO-selective measurement [56] have been used to perform real-time recording of endogenous ^•NO concentration dynamics evoked by activation of ionotropic GluR. By using this methodological approach we were able to show that NMDA-evoked ^•NO concentration dynamics is heterogeneous along the trisynaptic loop in the rat hippocampus [57]. We also provided evidence that the AMPAr in addition to the NMDAr could contribute to the fine tuning of glutamate-dependent ^•NO production [58] and that NMDA-evoked ^•NO production inhibits tissue O₂ consumption for submicromolar concentrations [59].

The use of this approach has also allowed the characterization of endogenous ^•NO concentration dynamics produced in rat brain in vivo upon glutamatergic stimulation. In the hippocampus we found that both endogenous and synthetic agonists of ionotropic GluR (glutamate, NMDA, and AMPA) promoted transient increases of extracellular ^•NO concentration, although with different kinetics. Pharmacological modulation suggested that ^•NO overflow elicited by glutamate resulted from an integrated activation of both subtypes of ionotropic GluR [60]. Glutamate-evoked ^•NO concentration changes were further characterized along the hippocampal trisynaptic loop (CA1, CA3, and dentate gyrus), as well as in cerebral cortex and striatum, showing that while glutamate induced transitory increases in ^•NO levels in all regions, regional-specific concentration profiles were observed (unpublished data).

3.2. ^•NO Diffusion and Half-Life

Together with ^•NO production, the rates of diffusion and inactivation are key determinants of ^•NO concentration dynamics in tissues. However, unlike the mechanisms of ^•NO synthesis, the physiologic processes underlying the termination of ^•NO signals in vivo (inactivation) remain unclear, particularly in the brain. Inactivation of classical neurotransmitters (e.g., dopamine or glutamate) relies on their rapid removal from the extracellular space via intracellular uptake processes [61–63]. However, given the uncommon physicochemical properties of ^•NO, its consumption via chemical reactions is generally accepted as the most probable route of inactivation. Although several biochemical mechanisms have been proposed to fulfill that role, the exact extent of their effect on ^•NO concentration dynamics in brain tissue has remained uncertain. Another layer of complexity is added by the effect of diffusional processes on the signal. Although ^•NO has been frequently considered as a molecule that can freely diffuse in tissues [64–66], with a diffusion coefficient estimated in aqueous solution of to 4. cm²/s [67–69], it has been observed that ^•NO diffusion is hindered across the aortic wall [70].

Recently, we have obtained experimental data that allowed the characterization of ^•NO diffusion in the rat brain in vivo. The studies were conducted by using ^•NO-selective carbon fiber microelectrodes to monitor ^•NO increases following local application of small volumes (few nanoliters) of ^•NO solution from a micropipette located 200–350 μm away. These microelectrode/micropipette arrays were stereotaxically inserted in the brain of anesthetized rats [71].

The resulting electrochemical signals were fitted to an equation that describes the diffusion of a compound and takes into account a first-order kinetics of inactivation. This approach allowed the estimation of the ^•NO diffusion coefficient and half-life in tissue. We found that ^•NO is highly diffusible and short lived in the brain, having an effective diffusion coefficient () of 2. cm²/s and a half-life of 0.64 s in the rat cortex.

We have also investigated possible pathways of ^•NO diffusion by testing the concepts of free, hindered, and enhanced diffusion. The D_NO obtained in agarose gel, a model used to evaluate ^•NO-free diffusion, was cm²/s, only 14% higher than the in vivo , suggesting that ^•NO could freely diffuse in the brain. Accordingly, we found that ^•NO diffusion in brain tissue is distinct from a molecule of similar size that remains in the extracellular space (nitrite), but importantly, our data indicated that ^•NO diffusion is hindered by conditions that mimic intracellular macromolecular crowding [71].

These latter lines of evidence suggest that neither ^•NO diffusion through the extracellular space nor a homogeneous diffusion in the tissue through brain cells provides a reasonable conceptual explanation for the similarity between the obtained in vivo and the D_NO found in agarose gel. Thus, as previously suggested for O₂ [72, 73], it is likely that ^•NO diffusion in nervous tissue is facilitated by certain physiological processes. A likely candidate is ^•NO partition in hydrophobic media, such as cell membranes and myelin sheaths, which may constitute low-resistance pathways that facilitate ^•NO diffusion in nervous tissue, resulting in an increased diffusion rate.

Together with diffusion, the quantification of ^•NO half-life in the brain is also important to better understand the dynamics of ^•NO, produced during brain function. ^•NO half-life is a kinetic parameter essential for the definition of its basal concentrations and diffusion radius. Some studies have estimated the ^•NO half-life in biological tissues in the range between 5 and 15 s [66]. Studies performed on isolated cell preparations of brain and liver extrapolated values for in vivo of around 100 ms [74, 75], in accordance with the half-life obtained in heart muscle [76]. In intact brain tissue, a half-life of 10 ms was reported in acute cerebellar slices for [^•NO] below 10 nM [77] which was 60 fold slower in organotypic cerebellar slices [78]. Although variability exists in the data, these works support the notion that ^•NO is a short-lived messenger, in agreement with the biological necessity to maintain ^•NO levels within the physiological range. Our in vivo approach, based on the fitting of a diffusion/inactivation equation to the signals of exogenously applied ^•NO in vivo in the rat brain cortex, allowed the estimation of a half-life of 0.64 s in that brain region, thus providing quantitative experimental evidence for a sub-second ^•NO half-life in vivo.

3.3. Mechanisms of ^•NO Inactivation

Several studies have found O₂-dependent mechanisms of ^•NO consumption/inactivation in in vitro preparations but the direct reaction between ^•NO and O₂ is too slow to account for significant ^•NO consumption if one considers the low concentration of the reactants in vivo (particularly ^•NO). Nevertheless, the favored partition of these molecules in the hydrophobic phase of cell membranes greatly accelerates the reaction, possibly accounting for ^•NO consumption in tissues [79].

As mentioned above, ^•NO direct biological activity may play out through the reaction with transition metals, in particular the iron contained in hemeproteins. One such target for ^•NO is Cytochrome c oxidase (CcO), the terminal complex of the mitochondrial respiratory chain. In the mid-1990s, ^•NO was shown to bind to and inhibit CcO [80] and block mitochondrial respiration in preparations as diverse as isolated mitochondria [81] synaptosomes [82], and primary cell cultures [83, 84].

The initial assessment of ^•NO interaction with CcO suggested an inhibition mechanism based on the high-affinity, reversible binding of ^•NO to the enzyme’s binuclear active site, in competition with O₂. [81, 82, 85]. In accordance with this model that prevails under high enzyme turnover conditions, ^•NO binds to the fully reduced binuclear center (heme a₃/Cu_B) and its removal from the active binuclear sites returns CcO to a fully active state.

A second low-affinity inhibitory site has been proposed for the fully oxidized enzyme—the Cu_B in the binuclear center-rendering CcO inactive [86, 87]. This is an uncompetitive mechanism of inhibition of CcO by ^•NO. Contrary to the simple on/off mechanism observed in the competitive model, bound ^•NO reduces the enzyme and is itself oxidized to . Enzyme inhibition is reverted by dissociation of upon further reduction [88, 89]. This uncompetitive inhibition mechanism is favored by high [O₂] and low turnover and its main biological role seems to be to consume ^•NO, thus shaping ^•NO concentration dynamics in the tissue [90, 91].

In mitochondria, ^•NO can also be consumed by the nearly diffusion-limited reaction with [92], generated as a byproduct of cellular respiration. However, the physiologic relevance of this reaction is questionable, since dismutation by MnSOD greatly decreases concentration (in spite of the favoured competition of ^•NO over SOD to ) to values in the pM range under physiologic conditions [7, 93].

Several heme-containing enzymes catalyze redox reactions that can consume ^•NO in dispersed preparations. Among others, a flavoheme protein in several mammalian cell lines [94], lipoxygenases, prostaglandin H synthase and cycloxygenase-1 in platelets [95–97], peroxidases [98], and cytochrome P450 oxidoreductase [99] have been identified.

Proteins from the globin family are other likely candidates to participate in ^•NO inactivation in brain tissue due to their rapid reaction with ^•NO ( M⁻¹ s⁻¹). In several brain regions, neurons express neuroglobin (Ngb), cytoglobin, and also hemoglobin [100–102]. The exact physiologic functions of these proteins in the brain tissue are not clear. It was observed that the overexpression of Ngb protects the brain against ischemic damage [103] and cells overexpressing Ngb are more resistant to ^•NO cytotoxicity, suggesting a possible role of ^•NO scavenging in the neuroprotective mechanism of Ngb. However, given the low intraneuronal concentration of these proteins (<1 μM), the function of Ngb as a robust ^•NO scavenger would require its association with a putative met-Ngb reductase to rapidly regenerate ferrous heme upon reaction with ^•NO. Yet, this functional association has not been reported [104]. Neuronal hemoglobin appears to have a role in intracellular oxygen storage or transport but insufficient data exists regarding its capacity to metabolize ^•NO in neurons [102]. Conversely, it is widely accepted that hemoglobin is the major ^•NO sink in the vasculature, due to its high concentration in erythrocytes (ca. 20 mM) and high reaction rate with ^•NO [105]. The effectiveness of this reaction on the regulation of ^•NO concentration in the extravascular compartment has been disputed since erythrocytic packing of hemoglobin and intravascular flow can decrease the effectiveness of hemoglobin scavenging of ^•NO by 3-4 orders of magnitude [105–107].

The uncertainty regarding how ^•NO is inactivated in the brain in physiologic conditions is related to difficulties in its direct measurement in intact tissue. A study on ^•NO inactivation in cerebellar slices of rat brain found that ^•NO was inactivated by an unknown mechanism that could not be explained by any known mechanism of ^•NO consumption [77].

3.3.1. Pathways of ^•NO Inactivation In Vivo

A strategy to the study of the mechanisms that govern ^•NO inactivation in vivo has included the recordings of ^•NO signals by ^•NO-selective microelectrodes, following local application of small volumes of exogenous ^•NO in the brain [10]. The decay of ^•NO signals obtained by means of this approach was very sensitive to experimental conditions impairing vascular function in vivo. First, global ischemia induced a 90% decrease in the ^•NO signals decay rate constant (k), suggesting that ^•NO inactivation is nearly abolished during this condition. Second, the k values of ^•NO signals decay were 3–5-fold higher in vivo than in brain slices of cortex and hippocampus, which lack functional vasculature. Finally, impairing the microcirculation in the brain in vivo by inducing hemorrhagic shock induced an average 50% decrease in k. Comparatively, modulation of O₂ tension in the brain in vivo, either by inducing hypoxia or hyperoxia, caused only small changes in ^•NO decay (20%), thus demonstrating that scavenging by circulating red blood cells constitutes the major ^•NO inactivation pathway in the brain (Figure 1).

Figure 1

The major pathways of ^•NO production and inactivation in the brain. (a) ^•NO is synthesized following calcium entrance into the postsynaptic density (upon glutamate activation of NMDA receptors). Calcium activates nNOS by promoting Calmodulin (CaM) binding to the enzyme. ^•NO rapidly diffuses to neighboring tissue, being inactivated both by O₂-dependent mechanisms and by scavenging by circulating erythrocytes (RBCs). (b) Typical electrochemical signals obtained using microelectrodes in the rat brain in vivo and in agarose gel following local application of small volumes (few nL) of ^•NO solution. First-order decay constant values (k) were used to quantify the decay profiles. (c) Anoxia, induced by a nitrite lethal dose, induced a 20% decrease in k (k2), in contrast with a large decrease in following cardiac arrest, suggesting that the major route of ^•NO inactivation in the brain in vivo is by circulating RBCs scavenging (k1). Adapted from [10].

The ^•NO half-life in tissue is thereby expected to be dependent on the vascular density, which may be tuned to meet specific local signaling requirements. Accordingly, using microelectrode arrays that allow monitoring ^•NO in four brain sites simultaneously, we observed that the probability of ^•NO detection following its local application is apparently related with the local vascular density [10].

4. The Functional Impact of ^•NO in Brain Tissue

4.1. ^•NO as a Neuromodulator

sGC is the best characterized signaling target for ^•NO and is often considered a receptor-like molecule for ^•NO in cells for the role of ^•NO as a neuromodulator is mainly mediated by its binding to sGC, leading to transient increases in cGMP.

The most widespread mechanism associated with cGMP is the activation of the cGMP-dependent protein kinase (PKG). Several substrates for PKG have been identified and many of its actions are exerted at the level of phosphatases, thereby affecting the levels of phosphorylation of effector proteins [108]. Other mechanism able to mediate ^•NO signaling effects downstream sGC is the cGMP activation of cyclic nucleotide-gated (CNG) ion channels [109] and hyperpolarization-activated cyclic nucleotide-modulated (HCN) channels [110]. CNG and HCN are nonselective cation channels that allow the passage of several ions, including Na⁺, K⁺, and Ca²⁺. For instance, studies reported that, in neurons expressing these ionic channels, the ^•NO-cGMP pathway cause a pre- or postsynaptic membrane depolarization (depending on the location of the channels) thereby modulating neuronal excitability [3].

It is noteworthy that the actions of ^•NO through the ^•NO-cGMP pathway obey no general rules. Despite employing the same transduction mechanism (cGMP), the physiological outcomes are tissue/cell specific since different cell populations may arbor different cGMP targets. Thus, the great variability of cGMP targets among different populations of neurons seems to explain the wide range of reported ^•NO effects in the nervous system. To cite some examples, ^•NO has been implicated in the modulation of neuronal excitability, synaptic plasticity, modulation of neurotransmitter release, regulation of rhythmic activity, and neurovascular coupling [3, 4, 46, 111].

4.2. Regulation of Mitochondrial Respiration

The average [O₂] in capillaries is 30 μM and typically cells experience an intracellular concentration of O₂ of around 3 μM [112]. The high affinity of CcO for its substrate guarantees sustained mitochondrial phosphorylation with a large safety margin regarding O₂ [113]. ^•NO will compete with O₂ for binding to the active site of CcO, inhibiting respiration, raising the enzyme’s K_m and limiting O₂ usage even under normoxic conditions.

The physiological and/or pathophysiological impact of ^•NO inhibition of CcO will depend on the fraction of enzyme that is effectively inhibited and if this decreases O₂ consumption and oxidative phosphorylation [114]. The overall electron flow in the respiratory chain is typically regulated by complex I in state 4 respiring mitochondria and under these conditions, a fractional inhibition of CcO by ^•NO produces no net change on O₂ consumption, contrary to what occurs in state 3 respiring mitochondria [115, 116]. An immediate consequence of decreased O₂ consumption is the increase in O₂ availability and increased tissue oxygenation at sites farther away from blood vessels [74], an effect that may act in synergy with ^•NO-induced vasodilatiion. Alternatively, increased [O₂] may render it available to participate in signaling pathways such as the activation of hypoxia-inducible factor [117].

A key notion which has emerged in the literature is that mitochondrial cell signaling cascades are intimately linked to ^•NO regulation of CcO function [118]. The interaction of ^•NO with CcO may inhibit enzyme activity without producing a net effect in cellular respiration: steady-state and kinetic modeling [119] have revealed that the ^•NO-CcO interaction can lead to an accumulation of reduced cytochromes upstream of CcO without producing a net effect on cellular respiration, but with consequences in redox signaling pathways such as increased mitochondrial production RONS, notably and H₂O₂ [114, 120, 121], both of which can impact downstream signaling cascades.

The situation changes dramatically when inhibition of CcO is severe and persistent-excessive inhibition of mitochondrial respiration results in bioenergetics dysfunction and cellular damage, conditions associated with aging and neurodegeneration. Under such conditions, excess may react with ^•NO yielding ONOO⁻, which unlike ^•NO can irreversibly block all complexes of the mitochondrial respiratory chain through oxidation and nitration chemistry [122–124]. In 2005, Shiva et al. proposed the term nitroxia to describe this pathological situation resulting from a deregulation of the ^•NO-CcO signaling pathway with increased production of RONS leading to mitochondrial and cellular oxidation and nitration chemistry [125].

4.3. Neurovascular Coupling

^•NO has been suggested as a mediator of the neurovascular coupling, the active mechanism enlarging vessel diameter in response to the rising of metabolic demands imposed by neuronal activity [126]. Indeed, ^•NO appears well suited to mediate this process as it is a potent vasodilator, is released during enhanced neuronal activity, and, as previously discussed, is also highly diffusible. During the years, the role of ^•NO in neurovascular coupling has been strengthened by the observation that the increase in cerebral blood flow dependent on neuronal activation is repressed by NOS inhibitors [127–130]. However, contradictory reports have also shown the lack of effect of NOS inhibitors, pointing towards a lack of ^•NO-mediated effect associated to neurovascular coupling [131–133]. As a matter of fact, although it is plausible that neuronal-derived ^•NO is involved in the regulation of cerebral blood flow, concrete evidence is still missing, as well as the elucidation of the underlying mechanism [134]. Recently, by using an experimental approach that allowed the simultaneous measurement of ^•NO concentration dynamics and cerebral blood flow changes in vivo upon glutamatergic activation in hippocampus we were able to establish the temporal, amplitude, and spatial association of both events. Furthermore, the coupling between neuronal activation and local cerebral blood flow changes mediated by neuronal-derived ^•NO occurs in the hippocampus regardless of the intermediacy of other cellular players such as astrocytes (unpublished data).

The mechanism of neuronal-derived ^•NO, via volume signaling, mediating neurovascular coupling, may be a noncanonical fashion to underlie a process of vital importance for the brain to preserve its structural and functional integrity [135]. However, the dual interaction of ^•NO concentration dynamics and vasculature assists the hypothesis of a highly and intrinsically controlled mechanism to match blood supply with the metabolic demands imposed by increased neuronal activity. While ^•NO triggers the increase in cerebral blood flow, in turn, the increase in the cerebral blood flow, by way of hemoglobin-dependent inactivation of ^•NO, helps to shape the ^•NO signal.

4.4. Neurodegeneration

A key tenet of ^•NO bioactivity is that besides participating in important physiological functions as those previously mentioned, it has also been implicated in pathological processes associated with several neurodegenerative disorders, such as Alzheimer’s disease (AD), Parkinson’s disease (PD), amyotrophic lateral sclerosis (ALS), Huntington’s disease (HD), and ischemic brain injury (reviewed by [111, 136]. The pathological role of ^•NO involves pathways that are only partially different from those underlying its physiological actions but which are associated to other stress conditions. In AD, the three NOS isoforms are suggested to operate as central mediators of amyloid-β (Aβ) action, contributing to the maintenance, self-perpetuation, and progression of the disease [137], although data regarding changes in NOS in AD are highly inconsistent [138]. In cell-free assays, Aβ peptides were shown to strongly inhibit constitutive NOS (eNOS and nNOS) [139]. Conversely, other reports have shown Aβ-dependent enhancement of nNOS activity [140], and memory impairment appears to be correlated with the increase in nNOS expression and ^•NO levels [141].

A larger consensus exists regarding the inducible isoform of NOS, which seems to be overexpressed in AD [138]. Various studies have reported that Aβ stimulates microglial and astrocytic ^•NO production [142–144]. Moreover, modifications of iNOS expression are suggested to importantly contribute to AD progression. The ablation of iNOS from a transgenic mouse model of AD protected the AD-like mice from cerebral plaque formation and increased Aβ levels, astrocytosis, and microgliosis [145]. Moreover, astrocytic-derived ^•NO triggers tau hyperphosphorylation in hippocampal neurons [146] and Aβ-mediated inhibition of NMDAr-dependent LTP requires iNOS activity [147].

The majority of neurotoxic effects of ^•NO supporting the development of AD pathological mechanisms are due to indirect reactions of ^•NO, promoting posttranslational protein modifications, namely, nitration and S-nitrosation. Indeed, high levels of nitrotyrosine have been found in brains from AD patients [148–151]. Nitrated proteins were described to be associated with Aβ deposition [150], and recently Aβ itself was shown to be a target for ^•NO bioactivity. Nitrated Aβ is characterized by an accelerated aggregation rate, being detected in the core of plaques of APP/PS1 mice and AD brains [152]. Also tau protein and synaptophysin are potential targets for nitration with relevant consequences in terms of AD progression [153].

Furthermore, lines of evidence suggest that a number of proteins are S-nitrosated in AD. An example with important impact in neurodegeneration is the S-nitrosation of endoplasmic reticulum (ER) chaperone protein-dissulphide isomerase (PDI). The modification of an active cysteine in the PDI promotes the inhibition of both isomerase and chaperone activities, resulting in abnormal accumulation of misfolded and polyubiquitinated proteins, ER stress, and ultimately in cell death [154, 155]. Also dynamin-related protein 1 (Drp1) is a target for S-nitrosation, being hyperactivated, a mechanism suggested to underlie Aβ-related mitochondrial fission and neuronal injury [156].

Finally, it should be remarked that ^•NO may also have a protective role in the development of AD pathology. Under physiological conditions, endothelium-derived ^•NO evidenced a protective action against Aβ accumulation through direct modulation of Aβ, APP, and BACE-1 levels [157].

5. Novel Perspectives on the Mechanisms Underlying Deregulation of ^•NO Dynamics in Disease

As mentioned in the sections above, the excessive activation of NOSs is commonly regarded as the main mechanism leading to the buildup of cytotoxic ^•NO concentrations in pathological conditions ranging from AD, PD, multiple sclerosis (MS) to ischemic damage [158, 159]. Despite the view of the excessive ^•NO production in neurodegeneration (although the quantitation in vivo requires refinenments), the notions presented in the previous sections of this paper also highlight the role of the pathways of ^•NO diffusion and inactivation in the regulation of ^•NO levels in brain tissue. Accordingly, a pathological change of the mechanisms controlling diffusion and inactivation might also cause a deregulation in ^•NO concentration dynamics with consequences for tissue homeostasis. Indeed, given the recently found importance of the vasculature on the regulation of ^•NO inactivation in vivo [10], there are several pathological situations in which a vascular impairment might greatly account for deregulation of ^•NO levels, including ischemia-reperfusion, AD, and MS.

It is known that, in the brain of AD patients, vascular dysfunction appears in the early stages of the disease, which manifests as a characteristic oligemia in some brain regions [160]. This condition might contribute to increase ^•NO concentration due to lowered inactivation.

Conversely, the blood brain barrier breakdown that occurs in MS [161] might contribute to increase ^•NO inactivation, thereby lowering ^•NO concentration. But, alterations in inactivation might also be beneficial in some circumstances. We observed a great decrease in ^•NO inactivation rate in the brain during global ischemia [10], which might potentiate ^•NO accumulation in the affected tissue, formed from either residual NOS activity or NOS-independent ^•NO synthesis mechanisms, such as ischemic reduction of nitrite [162]. Interestingly, preischemic administration of ^•NO donors or nitrite in vivo decreases brain ischemia/reperfusion infarct volume in models of focal ischemia [162]. The vasodilatory action of ^•NO may explain its neuroprotective role during ischemia by enhancing microcirculation in the regions adjacent to the affected area (penumbra). Thus, it is possible that the impairment of ^•NO inactivation in the brain region affected by ischemia is protective by increasing local ^•NO availability and consequently enhancing microcirculation in the adjacent tissue.

Acknowledgment

This work was supported by FCT (Portugal) Grants PTDC/SAU-NEU/108992/2008, PTDC/SAU-NEU/103538/2008, and PTDC/SAU-BEB/103228/2008.

References

J. W. Coleman, “Nitric oxide in immunity and inflammation,” International Immunopharmacology, vol. 1, no. 8, pp. 1397–1406, 2001.
View at: Publisher Site | Google Scholar
R. F. Furchgott, “Endothelium-derived relaxing factor: discovery, early studies, and identification as nitric oxide,” Bioscience Reports, vol. 19, no. 4, pp. 235–251, 1999.
View at: Google Scholar
J. Garthwaite, “Concepts of neural nitric oxide-mediated transmission,” European Journal of Neuroscience, vol. 27, no. 11, pp. 2783–2802, 2008.
View at: Publisher Site | Google Scholar
J. R. Steinert, T. Chernova, and I. D. Forsythe, “Nitric oxide signaling in brain function, dysfunction, and dementia,” Neuroscientist, vol. 16, no. 4, pp. 435–452, 2010.
View at: Publisher Site | Google Scholar
D. D. Thomas, L. A. Ridnour, J. S. Isenberg et al., “The chemical biology of nitric oxide: implications in cellular signaling,” Free Radical Biology & Medicine, vol. 45, no. 1, pp. 18–31, 2008.
View at: Google Scholar
B. G. Hill, B. P. Dranka, S. M. Bailey, J. R. Lancaster, and V. M. Darley-Usmar, “What part of NO don't you understand? Some answers to the cardinal questions in nitric oxide biology,” Journal of Biological Chemistry, vol. 285, no. 26, pp. 19699–19704, 2010.
View at: Publisher Site | Google Scholar
D. A. Wink and J. B. Mitchell, “Chemical biology of nitric oxide: insights into regulatory, cytotoxic, and cytoprotective mechanisms of nitric oxide,” Free Radical Biology and Medicine, vol. 25, no. 4-5, pp. 434–456, 1998.
View at: Publisher Site | Google Scholar
C. E. Cooper, “Nitric oxide and iron proteins,” Biochimica et Biophysica Acta, vol. 1411, no. 2-3, pp. 290–309, 1999.
View at: Publisher Site | Google Scholar
C. E. Cooper and C. Giulivi, “Nitric oxide regulation of mitochondrial oxygen consumption II: molecular mechanism and tissue physiology,” American Journal of Physiology, vol. 292, no. 6, pp. C1993–C2003, 2007.
View at: Publisher Site | Google Scholar
R. M. Santos, C. F. Lourenço, F. Pomerleau et al., “Brain nitric oxide inactivation is governed by the vasculature,” Antioxidants and Redox Signaling, vol. 14, no. 6, pp. 1011–1021, 2011.
View at: Publisher Site | Google Scholar
B. Roy and J. Garthwaite, “Nitric oxide activation of guanylyl cyclase in cells revisited,” Proceedings of the National Academy of Sciences of the United States of America, vol. 103, no. 32, pp. 12185–12190, 2006.
View at: Publisher Site | Google Scholar
T. C. Bellamy, C. Griffiths, and J. Garthwaite, “Differential sensitivity of guanylyl cyclase and mitochondrial respiration to nitric oxide measured using clamped concentrations,” Journal of Biological Chemistry, vol. 277, no. 35, pp. 31801–31807, 2002.
View at: Publisher Site | Google Scholar
W. A. Pryor and G. L. Squadrito, “The chemistry of peroxynitrite: a product from the reaction of nitric oxide with superoxide,” American Journal of Physiology, vol. 268, no. 5, pp. L699–L722, 1995.
View at: Google Scholar
D. A. Wink, R. W. Nims, J. F. Derbyshire et al., “Reaction kinetics for nitrosation of cysteine and glutathione in aerobic nitric oxide solutions at neutral pH. Insights into the fate and physiological effects of intermediates generated in the NO/O₂ reaction,” Chemical Research in Toxicology, vol. 7, no. 4, pp. 519–525, 1994.
View at: Google Scholar
D. A. Wink, J. A. Cook, S. Y. Kim et al., “Superoxide modulates the oxidation and nitrosation of thiols by nitric oxide-derived reactive intermediates. Chemical aspects involved in the balance between oxidative and nitrosative stress,” Journal of Biological Chemistry, vol. 272, no. 17, pp. 11147–11151, 1997.
View at: Publisher Site | Google Scholar
A. Martínez-Ruiz, S. Cadenas, and S. Lamas, “Nitric oxide signaling: classical, less classical, and nonclassical mechanisms,” Free Radical Biology and Medicine, vol. 51, no. 1, pp. 17–29, 2011.
View at: Publisher Site | Google Scholar
J. S. Stamler, E. J. Toone, S. A. Lipton, and N. J. Sucher, “(S)NO signals: translocation, regulation, and a consensus motif,” Neuron, vol. 18, no. 5, pp. 691–696, 1997.
View at: Publisher Site | Google Scholar
D. Seth and J. S. Stamler, “The SNO-proteome: causation and classifications,” Current Opinion in Chemical Biology, vol. 15, no. 1, pp. 129–136, 2011.
View at: Publisher Site | Google Scholar
M. W. Foster, D. T. Hess, and J. S. Stamler, “Protein S-nitrosylation in health and disease: a current perspective,” Trends in Molecular Medicine, vol. 15, no. 9, pp. 391–404, 2009.
View at: Publisher Site | Google Scholar
Y. B. Choi, L. Tenneti, D. A. Le et al., “Molecular basis of NMDA receptor-coupled ion channel modulation by S- nitrosylation,” Nature Neuroscience, vol. 3, no. 1, pp. 15–21, 2000.
View at: Publisher Site | Google Scholar
Y. Huang, H. Y. Man, Y. Sekine-Aizawa et al., “S-nitrosylation of N-ethylmaleimide sensitive factor mediates surface expression of AMPA receptors,” Neuron, vol. 46, no. 4, pp. 533–540, 2005.
View at: Publisher Site | Google Scholar
B. Selvakumar, R. L. Huganir, and S. H. Snyder, “S-nitrosylation of stargazin regulates surface expression of AMPA-glutamate neurotransmitter receptors,” Proceedings of the National Academy of Sciences of the United States of America, vol. 106, no. 38, pp. 16440–16445, 2009.
View at: Publisher Site | Google Scholar
Y. M. Kim, C. A. Bombeck, and T. R. Billiar, “Nitric oxide as a bifunctional regulator of apoptosis,” Circulation Research, vol. 84, no. 3, pp. 253–256, 1999.
View at: Google Scholar
Y. M. Kim, R. V. Talanian, and T. R. Billiar, “Nitric oxide inhibits apoptosis by preventing increases in caspase-3- like activity via two distinct mechanisms,” Journal of Biological Chemistry, vol. 272, no. 49, pp. 31138–31148, 1997.
View at: Publisher Site | Google Scholar
O. Sidorkina, M. G. Espey, K. M. Miranda, D. A. Wink, and J. Laval, “Inhibition of poly(ADP-ribose) polymerase (PARP) by nitric oxide and reactive nitrogen oxide species,” Free Radical Biology and Medicine, vol. 35, no. 11, pp. 1431–1438, 2003.
View at: Publisher Site | Google Scholar
G. C. Brown and V. Borutaite, “Nitric oxide and mitochondrial respiration in the heart,” Cardiovascular Research, vol. 75, no. 2, pp. 283–290, 2007.
View at: Publisher Site | Google Scholar
M. R. Hara and S. H. Snyder, “Nitric oxide-GAPDH-Siah: a novel cell death cascade,” Cellular and Molecular Neurobiology, vol. 26, no. 4–6, pp. 527–538, 2006.
View at: Google Scholar
H. Ischiropoulos, “Protein tyrosine nitration—an update,” Archives of Biochemistry and Biophysics, vol. 484, no. 2, pp. 117–121, 2009.
View at: Publisher Site | Google Scholar
R. Radi, G. Peluffo, M. N. Alvarez, M. Naviliat, and A. Cayota, “Unraveling peroxynitrite formation in biological systems,” Free Radical Biology and Medicine, vol. 30, no. 5, pp. 463–488, 2001.
View at: Publisher Site | Google Scholar
C. Szabó, H. Ischiropoulos, and R. Radi, “Peroxynitrite: biochemistry, pathophysiology and development of therapeutics,” Nature Reviews Drug Discovery, vol. 6, no. 8, pp. 662–680, 2007.
View at: Publisher Site | Google Scholar
H. Ischiropoulos, “Biological tyrosine nitration: a pathophysiological function of nitric oxide and reactive oxygen species,” Archives of Biochemistry and Biophysics, vol. 356, no. 1, pp. 1–11, 1998.
View at: Publisher Site | Google Scholar
D. Liu, F. Bao, J. Wen, and J. Liu, “Mutation of superoxide dismutase elevates reactive species: comparison of nitration and oxidation of proteins in different brain regions of transgenic mice with amyotrophic lateral sclerosis,” Neuroscience, vol. 146, no. 1, pp. 255–264, 2007.
View at: Publisher Site | Google Scholar
K. A. Trumbull and J. S. Beckman, “A role for copper in the toxicity of zinc-deficient superoxide dismutase to motor neurons in amyotrophic lateral sclerosis,” Antioxidants and Redox Signaling, vol. 11, no. 7, pp. 1627–1639, 2009.
View at: Publisher Site | Google Scholar
J. P. Crow, J. B. Sampson, Y. Zhuang, J. A. Thompson, and J. S. Beckman, “Decreased zinc affinity of amyotrophic lateral sclerosis, associated superoxide dismutase mutants leads to enhanced catalysis of tyrosine nitration by peroxynitrite,” Journal of Neurochemistry, vol. 69, no. 5, pp. 1936–1944, 1997.
View at: Google Scholar
T. R. Larsen, A. S. Söderling, K. Caidahl, P. Roepstorff, and J. B. Gramsbergen, “Nitration of soluble proteins in organotypic culture models of Parkinson's disease,” Neurochemistry International, vol. 52, no. 3, pp. 487–494, 2008.
View at: Publisher Site | Google Scholar
J. Ara, S. Przedborski, A. B. Naini et al., “Inactivation of tyrosine hydroxylase by nitration following exposure to peroxynitrite and 1-methyl-4-phenyl-1,2,3,6-tetrahydropyridine (MPTP),” Proceedings of the National Academy of Sciences of the United States of America, vol. 95, no. 13, pp. 7659–7663, 1998.
View at: Publisher Site | Google Scholar
S. C. Daubner, T. Le, and S. Wang, “Tyrosine hydroxylase and regulation of dopamine synthesis,” Archives of Biochemistry and Biophysics, vol. 508, no. 1, pp. 1–12, 2011.
View at: Publisher Site | Google Scholar
F. Yamakura and H. Kawasaki, “Post-translational modifications of superoxide dismutase,” Biochimica et Biophysica Acta, vol. 1804, no. 2, pp. 318–325, 2010.
View at: Publisher Site | Google Scholar
D. Y. Choi, J. Zhang, and G. Bing, “Aging enhances the neuroinflammatory response and α-synuclein nitration in rats,” Neurobiology of Aging, vol. 31, no. 9, pp. 1649–1653, 2010.
View at: Publisher Site | Google Scholar
D. D. Thomas, M. G. Espey, L. A. Ridnour et al., “Hypoxic inducible factor 1α, extracellular signal-regulated kinase, and p53 are regulated by distinct threshold concentrations of nitric oxide,” Proceedings of the National Academy of Sciences of the United States of America, vol. 101, no. 24, pp. 8894–8899, 2004.
View at: Publisher Site | Google Scholar
H. Tochio, Q. Zhang, P. Mandal, M. Li, and M. Zhang, “Solution structure of the extended neuronal nitric oxide synthase PDZ domain complexed with an associated peptide,” Nature Structural Biology, vol. 6, no. 5, pp. 417–421, 1999.
View at: Publisher Site | Google Scholar
J. E. Brenman, D. S. Chao, S. H. Gee et al., “Interaction of nitric oxide synthase with the postsynaptic density protein PSD-95 and α1-syntrophin mediated by PDZ domains,” Cell, vol. 84, no. 5, pp. 757–767, 1996.
View at: Publisher Site | Google Scholar
H. C. Kornau, L. T. Schenker, M. B. Kennedy, and P. H. Seeburg, “Domain interaction between NMDA receptor subunits and the postsynaptic density protein PSD-95,” Science, vol. 269, no. 5231, pp. 1737–1740, 1995.
View at: Google Scholar
M. Niethammer, E. Kim, and M. Sheng, “Interaction between the C terminus of NMDA receptor subunits and multiple members of the PSD-95 family of membrane-associated guanylate kinases,” Journal of Neuroscience, vol. 16, no. 7, pp. 2157–2163, 1996.
View at: Google Scholar
K. S. Christopherson, B. J. Hillier, W. A. Lim, and D. S. Bredt, “PSD-95 assembles a ternary complex with the N-methyl-D-aspartic acid receptor and a bivalent neuronal NO synthase PDZ domain,” Journal of Biological Chemistry, vol. 274, no. 39, pp. 27467–27473, 1999.
View at: Publisher Site | Google Scholar
J. Garthwaite and C. L. Boulton, “Nitric oxide signaling in the central nervous system,” Annual Review of Physiology, vol. 57, pp. 683–706, 1995.
View at: Google Scholar
D. S. Bredt, C. E. Glatt, P. M. Hwang, M. Fotuhi, T. M. Dawson, and S. H. Snyder, “Nitric oxide synthase protein and mRNA are discretely localized in neuronal populations of the mammalian CNS together with NADPH diaphorase,” Neuron, vol. 7, no. 4, pp. 615–624, 1991.
View at: Publisher Site | Google Scholar
S. R. Jaffrey, A. M. Snowman, M. J. L. Eliasson, N. A. Cohen, and S. H. Snyder, “CAPON: a protein associated with neuronal nitric oxide synthase that regulates its interactions with PSD95,” Neuron, vol. 20, no. 1, pp. 115–124, 1998.
View at: Publisher Site | Google Scholar
A. Burette, U. Zabel, R. J. Weinberg, H. H. H. W. Schmidt, and J. G. Valtschanoff, “Synaptic localization of nitric oxide synthase and soluble guanylyl cyclase in the hippocampus,” Journal of Neuroscience, vol. 22, no. 20, pp. 8961–8970, 2002.
View at: Google Scholar
P. I. Nedvetsky, W. C. Sessa, and H. H. H. W. Schmidt, “There's NO binding like NOS binding: protein-protein interactions in NO/cGMP signaling,” Proceedings of the National Academy of Sciences of the United States of America, vol. 99, no. 26, pp. 16510–16512, 2002.
View at: Publisher Site | Google Scholar
A. Philippides, S. R. Ott, P. Husbands, T. A. Lovick, and M. O'Shea, “Modeling cooperative volume signaling in a plexus of nitric oxide synthase-expressing neurons,” Journal of Neuroscience, vol. 25, no. 28, pp. 6520–6532, 2005.
View at: Publisher Site | Google Scholar
R. M. Barbosa, C. F. Lourenço, R. M. Santos et al., “Chapter 20 in vivo real-time measurement of nitric oxide in anesthetized rat brain,” Methods in Enzymology, vol. 441, pp. 351–367, 2008.
View at: Publisher Site | Google Scholar
J. Laranjinha and A. Ledo, “Coordination of physiologic and toxic pathways in hippocampus by nitric oxide and mitochondria,” Frontiers in Bioscience, vol. 12, no. 3, pp. 1094–1106, 2007.
View at: Publisher Site | Google Scholar
J. L. Peters, L. H. Miner, A. C. Michael, and S. R. Sesack, “Ultrastructure at carbon fiber microelectrode implantation sites after acute voltammetric measurements in the striatum of anesthetized rats,” Journal of Neuroscience Methods, vol. 137, no. 1, pp. 9–23, 2004.
View at: Publisher Site | Google Scholar
J. A. Stamford, F. Crespi, and C. A. Marsden, “5—in vivo voltammetric methods for monitoring monoamine release and metabolism,” in Monitoring Neuronal Activity, J. A. Stamford, Ed., pp. 113–145, Oxford University Press, Oxford, UK, 1992.
View at: Google Scholar
R. M. Santos, C. F. Lourenço, A. P. Piedade et al., “A comparative study of carbon fiber-based microelectrodes for the measurement of nitric oxide in brain tissue,” Biosensors and Bioelectronics, vol. 24, no. 4, pp. 704–709, 2008.
View at: Publisher Site | Google Scholar
A. Ledo, R. M. Barbosa, G. A. Gerhardt, E. Cadenas, and J. Laranjinha, “Concentration dynamics of nitric oxide in rat hippocampal subregions evoked by stimulation of the NMDA glutamate receptor,” Proceedings of the National Academy of Sciences of the United States of America, vol. 102, no. 48, pp. 17483–17488, 2005.
View at: Publisher Site | Google Scholar
J. G. Frade, R. M. Barbosa, and J. Laranjinha, “Stimulation of NMDA and AMPA glutamate receptors elicits distinct concentration dynamics of nitric oxide in rat hippocampal slices,” Hippocampus, vol. 19, no. 7, pp. 603–611, 2009.
View at: Publisher Site | Google Scholar
A. Ledo, R. Barbosa, E. Cadenas, and J. Laranjinha, “Dynamic and interacting profiles of ^∗NO and O₂ in rat hippocampal slices,” Free Radical Biology & Medicine, vol. 48, no. 8, pp. 1044–1050, 2010.
View at: Google Scholar
C. F. LourençO, R. Santos, R. M. Barbosa, G. Gerhardt, E. Cadenas, and J. Laranjinha, “In vivo modulation of nitric oxide concentration dynamics upon glutamatergic neuronal activation in the hippocampus,” Hippocampus, vol. 21, no. 6, pp. 622–630, 2011.
View at: Publisher Site | Google Scholar
N. C. Danbolt, “Glutamate uptake,” Progress in Neurobiology, vol. 65, no. 1, pp. 1–105, 2001.
View at: Publisher Site | Google Scholar
J. D. Elsworth and R. H. Roth, “Dopamine synthesis, uptake, metabolism, and receptors: relevance to gene therapy of Parkinson's disease,” Experimental Neurology, vol. 144, no. 1, pp. 4–9, 1997.
View at: Publisher Site | Google Scholar
A. S. Horn, “Dopamine uptake: a review of progress in the last decade,” Progress in Neurobiology, vol. 34, no. 5, pp. 387–400, 1990.
View at: Publisher Site | Google Scholar
J. Wood and J. Garthwaite, “Models of the diffusional spread of nitric oxide: implications for neural nitric oxide signalling and its pharmacological properties,” Neuropharmacology, vol. 33, no. 11, pp. 1235–1244, 1994.
View at: Publisher Site | Google Scholar
J. R. Lancaster Jr., “Simulation of the diffusion and reaction of endogenously produced nitric oxide,” Proceedings of the National Academy of Sciences of the United States of America, vol. 91, no. 17, pp. 8137–8141, 1994.
View at: Publisher Site | Google Scholar
J. R. Lancaster, “A tutorial on the diffusibility and reactivity of free nitric oxide,” Nitric Oxide, vol. 1, no. 1, pp. 18–30, 1997.
View at: Publisher Site | Google Scholar
A. Denicola, J. M. Souza, R. Radi, and E. Lissi, “Nitric oxide diffusion in membranes determined by fluorescence quenching,” Archives of Biochemistry and Biophysics, vol. 328, no. 1, pp. 208–212, 1996.
View at: Publisher Site | Google Scholar
I. G. Zacharia and W. M. Deen, “Diffusivity and solubility of nitric oxide in water and saline,” Annals of Biomedical Engineering, vol. 33, no. 2, pp. 214–222, 2005.
View at: Publisher Site | Google Scholar
T. Malinski, Z. Taha, S. Grunfeld, S. Patton, M. Kapturczak, and P. Tomboulian, “Diffusion of nitric oxide in the aorta wall. Monitored in situ by porphyrinic microsensors,” Biochemical and Biophysical Research Communications, vol. 193, no. 3, pp. 1076–1082, 1993.
View at: Publisher Site | Google Scholar
X. Liu, P. Srinivasan, E. Collard, P. Grajdeanu, J. L. Zweier, and A. Friedman, “Nitric oxide diffusion rate is reduced in the aortic wall,” Biophysical Journal, vol. 94, no. 5, pp. 1880–1889, 2008.
View at: Publisher Site | Google Scholar
R. M. Santos, C. F. Loureno, G. A. Gerhardt, E. Cadenas, J. Laranjinha, and R. M. Barbosa, “Evidence for a pathway that facilitates nitric oxide diffusion in the brain,” Neurochemistry International, vol. 59, no. 1, pp. 90–96, 2011.
View at: Publisher Site | Google Scholar
T. B. Bentley and R. N. Pittman, “Influence of temperature on oxygen diffusion in hamster retractor muscle,” American Journal of Physiology, vol. 272, no. 3, pp. H1106–H1112, 1997.
View at: Google Scholar
B. D. Sidell, “Intracellular oxygen diffusion: the roles of myoglobin and lipid at cold body temperature,” The Journal of Experimental Biology, vol. 201, no. 8, pp. 1119–1128, 1998.
View at: Google Scholar
D. D. Thomas, X. Liu, S. P. Kantrow, and J. R. Lancaster, “The biological lifetime of nitric oxide: implications for the perivascular dynamics of NO and O₂,” Proceedings of the National Academy of Sciences of the United States of America, vol. 98, no. 1, pp. 355–360, 2001.
View at: Google Scholar
C. Griffiths and J. Gartwaite, “The shaping of nitric oxide signals by a cellular sink,” Journal of Physiology, vol. 536, no. 3, pp. 855–862, 2001.
View at: Publisher Site | Google Scholar
M. Kelm and J. Schrader, “Control of coronary vascular tone by nitric oxide,” Circulation Research, vol. 66, no. 6, pp. 1561–1575, 1990.
View at: Google Scholar
C. N. Hall and J. Garthwaite, “Inactivation of nitric oxide by rat cerebellar slices,” Journal of Physiology, vol. 577, no. 2, pp. 549–567, 2006.
View at: Publisher Site | Google Scholar
C. N. Hall and D. Attwell, “Assessing the physiological concentration and targets of nitric oxide in brain tissue,” Journal of Physiology, vol. 586, no. 15, pp. 3597–3615, 2008.
View at: Publisher Site | Google Scholar
X. Liu, M. J. S. Miller, M. S. Joshi, D. D. Thomas, and J. R. Lancaster, “Accelerated reaction of nitric oxide with O₂ within the hydrophobic interior of biological membranes,” Proceedings of the National Academy of Sciences of the United States of America, vol. 95, no. 5, pp. 2175–2179, 1998.
View at: Publisher Site | Google Scholar
X. J. Zhao, V. Sampath, and W. S. Caughey, “Infrared characterization of nitric oxide bonding to bovine heart cytochrome c oxidase and myoglobin,” Biochemical and Biophysical Research Communications, vol. 204, no. 2, pp. 537–543, 1994.
View at: Publisher Site | Google Scholar
M. W. J. Cleeter, A. M. Cooper, B. M. Darley-Usmar, D. Moncada, and A. H. V. Schapira, “Reversible inhibition of cytochrome c oxidase, the terminal enzyme of the mitochondrial respiratory chain, by nitric oxide,” The FEBS Letters, vol. 345, no. 1, pp. 50–54, 1994.
View at: Publisher Site | Google Scholar
G. C. Brown, “Nanomolar concentrations of nitric oxide reversibly inhibit synaptosomal respiration by competing with oxygen at cytochrome oxidase,” The FEBS Letters, vol. 356, no. 2-3, pp. 295–298, 1994.
View at: Publisher Site | Google Scholar
J. P. Bolanos, S. Peuchen, S. J. R. Heales, J. M. Land, and J. B. Clark, “Nitric oxide-mediated inhibition of the mitochondrial respiratory chain in cultured astrocytes,” Journal of Neurochemistry, vol. 63, no. 3, pp. 910–916, 1994.
View at: Google Scholar
B. Mitrovic, “Nitric oxide as a potential pathological mechanism in demyelination: its differential effects on primary glial cells in vitro,” Neuroscience, vol. 61, no. 3, pp. 575–585, 1994.
View at: Publisher Site | Google Scholar
M. Schweizer and C. Richter, “Nitric oxide potently and reversibly deenergizes mitochondria at low oxygen tension,” Biochemical and Biophysical Research Communications, vol. 204, no. 1, pp. 169–175, 1994.
View at: Publisher Site | Google Scholar
J. Torres, C. E. Cooper, and M. T. Wilson, “A common mechanism for the interaction of nitric oxide with the oxidized binuclear centre and oxygen intermediates of cytochrome c oxidase,” Journal of Biological Chemistry, vol. 273, no. 15, pp. 8756–8766, 1998.
View at: Publisher Site | Google Scholar
J. Torres, V. Darley-Usmar, and M. T. Wilson, “Inhibition of cytochrome c oxidase in turnover by nitric oxide: mechanism and implications for control of respiration,” Biochemical Journal, vol. 312, no. 1, pp. 169–173, 1995.
View at: Google Scholar
C. E. Cooper, J. Torres, M. A. Sharpe, and M. T. Wilson, “Nitric oxide ejects electrons from the binuclear centre of cytochrome c oxidase by reacting with oxidised copper: a general mechanism for the interaction of copper proteins with nitric oxide?” The FEBS Letters, vol. 414, no. 2, pp. 281–284, 1997.
View at: Publisher Site | Google Scholar
J. Torres, M. A. Sharpe, A. Rosquist, C. E. Cooper, and M. T. Wilson, “Cytochrome c oxidase rapidly metabolises nitric oxide to nitrite,” The FEBS Letters, vol. 475, no. 3, pp. 263–266, 2000.
View at: Publisher Site | Google Scholar
F. Antunes, A. Boveris, and E. Cadenas, “On the biologic role of the reaction of NO with oxidized cytochrome C oxidase,” Antioxidants and Redox Signaling, vol. 9, no. 10, pp. 1569–1579, 2007.
View at: Publisher Site | Google Scholar
M. Palacios-Callender, V. Hollis, M. Mitchison, N. Frakich, D. Unitt, and S. Moncada, “Cytochrome c oxidase regulates endogenous nitric oxide availability in respiring cells: a possible explanation for hypoxic vasodilation,” Proceedings of the National Academy of Sciences of the United States of America, vol. 104, no. 47, pp. 18508–18513, 2007.
View at: Publisher Site | Google Scholar
W. H. Koppenol, “100 years of peroxynitrite chemistry and 11 years of peroxynitrite biochemistry,” Redox Report, vol. 6, no. 6, pp. 339–341, 2001.
View at: Publisher Site | Google Scholar
S. Alvarez, L. B. Valdez, T. Zaobornyj, and A. Boveris, “Oxygen dependence of mitochondrial nitric oxide synthase activity,” Biochemical and Biophysical Research Communications, vol. 305, no. 3, pp. 771–775, 2003.
View at: Publisher Site | Google Scholar
P. R. Gardner, L. A. Martin, D. Hall, and A. M. Gardner, “Dioxygen-dependent metabolism of nitric oxide in mammalian cells,” Free Radical Biology and Medicine, vol. 31, no. 2, pp. 191–204, 2001.
View at: Publisher Site | Google Scholar
V. B. O'Donnell, B. Coles, M. J. Lewis, B. C. Crews, L. J. Marnett, and B. A. Freeman, “Catalytic consumption of nitric oxide by prostaglandin H synthase-1 regulates platelet function,” Journal of Biological Chemistry, vol. 275, no. 49, pp. 38239–38244, 2000.
View at: Publisher Site | Google Scholar
V. B. O'Donnell, K. B. Taylor, S. Parthasarathy et al., “15-Lipoxygenase catalytically consumes nitric oxide and impairs activation of guanylate cyclase,” Journal of Biological Chemistry, vol. 274, no. 29, pp. 20083–20091, 1999.
View at: Publisher Site | Google Scholar
P. C. Williams, M. J. Coffey, B. Coles et al., “In vivo aspirin supplementation inhibits nitric oxide consumption by human platelets,” Blood, vol. 106, no. 8, pp. 2737–2743, 2005.
View at: Publisher Site | Google Scholar
H. M. Abu-Soud and S. L. Hazen, “Nitric oxide is a physiological substrate for mammalian peroxidases,” Journal of Biological Chemistry, vol. 275, no. 48, pp. 37524–37532, 2000.
View at: Publisher Site | Google Scholar
C. N. Hall, R. G. Keynes, and J. Garthwaite, “Cytochrome P450 oxidoreductase participates in nitric oxide consumption by rat brain,” Biochemical Journal, vol. 419, no. 2, pp. 411–418, 2009.
View at: Publisher Site | Google Scholar
T. Burmester, B. Welch, S. Reinhardt, and T. Hankeln, “A verteblrate globin expressed in the brain,” Nature, vol. 407, no. 6803, pp. 520–523, 2000.
View at: Publisher Site | Google Scholar
P. P. A. Mammen, J. M. Shelton, Q. Ye et al., “Cytoglobin is a stress-responsive hemoprotein expressed in the developing and adult brain,” Journal of Histochemistry and Cytochemistry, vol. 54, no. 12, pp. 1349–1361, 2006.
View at: Publisher Site | Google Scholar
D. W. Schelshorn, A. Schneider, W. Kuschinsky et al., “Expression of hemoglobin in rodent neurons,” Journal of Cerebral Blood Flow and Metabolism, vol. 29, no. 3, pp. 585–595, 2009.
View at: Publisher Site | Google Scholar
Y. Sun, K. Jin, A. Peel, X. Ou Mao, L. Xie, and D. A. Greenberg, “Neuroglobin protects the brain from experimental stroke in vivo,” Proceedings of the National Academy of Sciences of the United States of America, vol. 100, no. 6, pp. 3497–3500, 2003.
View at: Publisher Site | Google Scholar
M. Brunori and B. Vallone, “A globin for the brain,” The FASEB Journal, vol. 20, no. 13, pp. 2192–2197, 2006.
View at: Publisher Site | Google Scholar
X. Liu, M. J. S. Miller, M. S. Joshi, H. Sadowska-Krowicka, D. A. Clark, and J. R. Lancaster, “Diffusion-limited reaction of free nitric oxide with erythrocytes,” Journal of Biological Chemistry, vol. 273, no. 30, pp. 18709–18713, 1998.
View at: Publisher Site | Google Scholar
J. C. Liao, T. W. Hein, M. W. Vaughn, K. T. Huang, and L. Kuo, “Intravascular flow decreases erythrocyte consumption of nitric oxide,” Proceedings of the National Academy of Sciences of the United States of America, vol. 96, no. 15, pp. 8757–8761, 1999.
View at: Publisher Site | Google Scholar
A. J. Hobbs, M. T. Gladwin, R. P. Patel, D. L. H. Williams, and A. R. Butler, “Haemoglobin: NO transporter, NO inactivator or NOne of the above?” Trends in Pharmacological Sciences, vol. 23, no. 9, pp. 406–411, 2002.
View at: Publisher Site | Google Scholar
J. Schlossmann and F. Hofmann, “cGMP-dependent protein kinases in drug discovery,” Drug Discovery Today, vol. 10, no. 9, pp. 627–634, 2005.
View at: Publisher Site | Google Scholar
U. B. Kaupp and R. Seifert, “Cyclic nucleotide-gated ion channels,” Physiological Reviews, vol. 82, no. 3, pp. 769–824, 2002.
View at: Google Scholar
K. B. Craven and W. N. Zagotta, “CNG and HCN channels: two peas, one pod,” Annual Review of Physiology, vol. 68, pp. 375–401, 2006.
View at: Publisher Site | Google Scholar
F. X. Guix, I. Uribesalgo, M. Coma, and F. J. Muñoz, “The physiology and pathophysiology of nitric oxide in the brain,” Progress in Neurobiology, vol. 76, no. 2, pp. 126–152, 2005.
View at: Publisher Site | Google Scholar
E. Gnaiger and A. V. Kuznetsov, “Mitochondrial respiration at low levels of oxygen and cytochrome c,” Biochemical Society Transactions, vol. 30, no. 2, pp. 252–258, 2002.
View at: Google Scholar
R. Rossignol, B. Faustin, C. Rocher, M. Malgat, J. P. Mazat, and T. Letellier, “Mitochondrial threshold effects,” Biochemical Journal, vol. 370, no. 3, pp. 751–762, 2003.
View at: Publisher Site | Google Scholar
M. Palacios-Callender, M. Quintero, V. S. Hollis, R. J. Springe, and S. Moncada, “Endogenous NO regulates superioxide production at low oxygen concentrations by modifying the redox state of cytochrome c oxidase,” Proceedings of the National Academy of Sciences of the United States of America, vol. 101, no. 20, pp. 7630–7635, 2004.
View at: Publisher Site | Google Scholar
B. Ventura, M. L. Genova, C. Bovina, G. Formiggini, and G. Lenaz, “Control of oxidative phosphorylation by Complex I in rat liver mitochondria: implications for aging,” Biochimica et Biophysica Acta, vol. 1553, no. 3, pp. 249–260, 2002.
View at: Publisher Site | Google Scholar
A. K. Groen, R. J. Wanders, H. V. Westerhoff, R. van der Meer, and J. M. Tager, “Quantification of the contribution of various steps to the control of mitochondrial respiration,” Journal of Biological Chemistry, vol. 257, no. 6, pp. 2754–2757, 1982.
View at: Google Scholar
T. Hagen, C. T. Taylor, F. Lam, and S. Moncada, “Redistribution of intracellular oxygen in hypoxia by nitric oxide: effect on HIF1α,” Science, vol. 302, no. 5652, pp. 1975–1978, 2003.
View at: Publisher Site | Google Scholar
S. Moncada and J. D. Erusalimsky, “Does nitric oxide modulate mitochondrial energy generation and apoptosis?” Nature Reviews Molecular Cell Biology, vol. 3, no. 3, pp. 214–220, 2002.
View at: Publisher Site | Google Scholar
M. G. Mason, P. Nicholls, M. T. Wilson, and C. E. Cooper, “Nitric oxide inhibition of respiration involves both competitive (heme) and noncompetitive (copper) binding to cytochrome c oxidase,” Proceedings of the National Academy of Sciences of the United States of America, vol. 103, no. 3, pp. 708–713, 2006.
View at: Publisher Site | Google Scholar
P. Brookes and V. M. Darley-Usmar, “Hypothesis: the mitochondrial NO· signaling pathway, and the transduction of nitrosative to oxidative cell signals: an alternative function for cytochrome c oxidase,” Free Radical Biology and Medicine, vol. 32, no. 4, pp. 370–374, 2002.
View at: Publisher Site | Google Scholar
P. S. Brookes, A. L. Levonen, S. Shiva, P. Sarti, and V. M. Darley-Usmar, “Mitochondria: regulators of signal transduction by reactive oxygen and nitrogen species,” Free Radical Biology and Medicine, vol. 33, no. 6, pp. 755–764, 2002.
View at: Publisher Site | Google Scholar
J. Murray, S. W. Taylor, B. Zhang, S. S. Ghosh, and R. A. Capaldi, “Oxidative damage to mitochondrial complex I due to peroxynitrite: identification of reactive tyrosines by mass spectrometry,” Journal of Biological Chemistry, vol. 278, no. 39, pp. 37223–37230, 2003.
View at: Publisher Site | Google Scholar
I. V. Turko, L. Li, K. S. Aulak, D. J. Stuehr, J. Y. Chang, and F. Murad, “Protein tyrosine nitration in the mitochondria from diabetic mouse heart: implications to dysfunctional mitochondria in diabetes,” Journal of Biological Chemistry, vol. 278, no. 36, pp. 33972–33977, 2003.
View at: Publisher Site | Google Scholar
K. S. Aulak, T. Koeck, J. W. Crabb, and D. J. Stuehr, “Dynamics of protein nitration in cells and mitochondria,” American Journal of Physiology, vol. 286, no. 1, pp. H30–H38, 2004.
View at: Google Scholar
S. Shiva, J. Y. Oh, A. L. Landar et al., “Nitroxia: the pathological consequence of dysfunction in the nitric oxide-cytochrome c oxidase signaling pathway,” Free Radical Biology and Medicine, vol. 38, no. 3, pp. 297–306, 2005.
View at: Publisher Site | Google Scholar
C. Iadecola, “Regulation of the cerebral microcirculation during neural activity: is nitric oxide the missing link?” Trends in Neurosciences, vol. 16, no. 6, pp. 206–214, 1993.
View at: Google Scholar
F. M. Faraci and K. R. Breese, “Nitric oxide mediates vasodilatation in response to activation of N- methyl-D-aspartate receptors in brain,” Circulation Research, vol. 72, no. 2, pp. 476–480, 1993.
View at: Google Scholar
W. Meng, J. R. Tobin, D. W. Busija, and C. Iadecola, “Glutamate-induced cerebral vasodilation is mediated by nitric oxide through N-methyl-D-aspartate receptors,” Stroke, vol. 26, no. 5, pp. 857–862, 1995.
View at: Google Scholar
D. A. Pelligrino, R. L. Gay, V. L. Baughman, and Q. Wang, “NO synthase inhibition modulates NMDA-induced changes in cerebral blood flow and EEG activity,” American Journal of Physiology, vol. 271, no. 3, pp. H990–H995, 1996.
View at: Google Scholar
N. Akgören, M. Fabricius, and M. Lauritzen, “Importance of nitric oxide for local increases of blood flow in rat cerebellar cortex during electrical stimulation,” Proceedings of the National Academy of Sciences of the United States of America, vol. 91, no. 13, pp. 5903–5907, 1994.
View at: Publisher Site | Google Scholar
K. Adachi, S. Takahashi, P. Melzer et al., “Increases in local cerebral blood flow associated with somatosensory activation are not mediated by NO,” American Journal of Physiology, vol. 267, no. 6, pp. H2155–H2162, 1994.
View at: Google Scholar
J. H. Greenberg, N. W. Sohn, and P. J. Hand, “Nitric oxide and the cerebral-blood-flow response to somatosensory activation following deafferentation,” Experimental Brain Research, vol. 129, no. 4, pp. 541–550, 1999.
View at: Google Scholar
Q. Wang, T. Kjaer, M. B. Jorgensen et al., “Nitric oxide does not act as a mediator coupling cerebral blood flow to neural activity following somatosensory stimuli in rats,” Neurological Research, vol. 15, no. 1, pp. 33–36, 1993.
View at: Google Scholar
D. R. Harder, C. Zhang, and D. Gebremedhin, “Astrocytes function in matching blood flow to metabolic activity,” News in Physiological Sciences, vol. 17, no. 1, pp. 27–31, 2002.
View at: Google Scholar
H. Girouard and C. Iadecola, “Neurovascular coupling in the normal brain and in hypertension, stroke, and Alzheimer disease,” Journal of Applied Physiology, vol. 100, no. 1, pp. 328–335, 2006.
View at: Publisher Site | Google Scholar
A. B. Knott and E. Bossy-Wetzel, “Nitric oxide in health and disease of the nervous system,” Antioxidants and Redox Signaling, vol. 11, no. 3, pp. 541–554, 2009.
View at: Publisher Site | Google Scholar
A. P. Fernandez, A. Pozo-Rodrigalvarez, J. Serrano, and R. Martinez-Murillo, “Nitric oxide: target for therapeutic strategies in alzheimer's disease,” Current Pharmaceutical Design, vol. 16, no. 25, pp. 2837–2850, 2010.
View at: Google Scholar
A. Law, S. Gauthier, and R. Quirion, “Say NO to Alzheimer's disease: the putative links between nitric oxide and dementia of the Alzheimer's type,” Brain Research Reviews, vol. 35, no. 1, pp. 73–96, 2001.
View at: Publisher Site | Google Scholar
G. Venturini, M. Colasanti, T. Persichini et al., “Beta-amyloid inhibits NOS activity by subtracting NADPH availability,” The FASEB Journal, vol. 16, no. 14, pp. 1970–1972, 2002.
View at: Google Scholar
M. Y. Stepanichev, M. V. Onufriev, A. A. Yakovlev et al., “Amyloid-β (25–35) increases activity of neuronal NO-synthase in rat brain,” Neurochemistry International, vol. 52, no. 6, pp. 1114–1124, 2008.
View at: Publisher Site | Google Scholar
I. D. Limón, A. Díaz, L. Mendieta et al., “Amyloid-β25-35 impairs memory and increases NO in the temporal cortex of rats,” Neuroscience Research, vol. 63, no. 2, pp. 129–137, 2009.
View at: Publisher Site | Google Scholar
M. N. Wallace, J. G. Geddes, D. A. Farquhar, and M. R. Masson, “Nitric oxide synthase in reactive astrocytes adjacent to β-amyloid plaques,” Experimental Neurology, vol. 144, no. 2, pp. 266–272, 1997.
View at: Publisher Site | Google Scholar
K. T. Akama and L. J. Van Eldik, “β-Amyloid stimulation of inducible nitric-oxide synthase in astrocytes is interleukin-1β- and tumor necrosis factor-α (TNFα)-dependent, and involves a TNFα receptor-associated factor- and NFκB-inducing kinase- dependent signaling mechanism,” Journal of Biological Chemistry, vol. 275, no. 11, pp. 7918–7924, 2000.
View at: Publisher Site | Google Scholar
F. Rossi and E. Bianchini, “Synergistic induction of nitric oxide by β-amyloid and cytokines in astrocytes,” Biochemical and Biophysical Research Communications, vol. 225, no. 2, pp. 474–478, 1996.
View at: Publisher Site | Google Scholar
C. Nathan, N. Calingasan, J. Nezezon et al., “Protection from Alzheimer's-like disease in the mouse by genetic ablation of inducible nitric oxide synthase,” Journal of Experimental Medicine, vol. 202, no. 9, pp. 1163–1169, 2005.
View at: Publisher Site | Google Scholar
E. T. Saez, M. Pehar, M. Vargas, L. Barbeito, and R. B. Maccioni, “Astrocytic nitric oxide triggers tau hyperphosphorylation in hippocampal neurons,” In Vivo, vol. 18, no. 3, pp. 275–280, 2004.
View at: Google Scholar
Q. Wang, M. J. Rowan, and R. Anwyl, “β-amyloid-mediated inhibition of NMDA receptor-dependent long-term potentiation induction involves activation of microglia and stimulation of inducible nitric oxide synthase and superoxide,” Journal of Neuroscience, vol. 24, no. 27, pp. 6049–6056, 2004.
View at: Publisher Site | Google Scholar
K. Van Dyke, “The possible role of peroxynitrite in Alzheimer's disease: a simple hypothesis that could be tested more thoroughly,” Medical Hypotheses, vol. 48, no. 5, pp. 375–380, 1997.
View at: Publisher Site | Google Scholar
T. Koppal, J. Drake, S. Yatin et al., “Peroxynitrite-induced alterations in synaptosomal membrane proteins: insight into oxidative stress in Alzheimer's disease,” Journal of Neurochemistry, vol. 72, no. 1, pp. 310–317, 1999.
View at: Publisher Site | Google Scholar
R. Sultana, H. F. Poon, J. Cai et al., “Identification of nitrated proteins in Alzheimer's disease brain using a redox proteomics approach,” Neurobiology of Disease, vol. 22, no. 1, pp. 76–87, 2006.
View at: Publisher Site | Google Scholar
S. R. Danielson and J. K. Andersen, “Oxidative and nitrative protein modifications in Parkinson's disease,” Free Radical Biology and Medicine, vol. 44, no. 10, pp. 1787–1794, 2008.
View at: Publisher Site | Google Scholar
M. P. Kummer, M. Hermes, A. Delekarte et al., “Nitration of tyrosine 10 critically enhances amyloid beta aggregation and plaque formation,” Neuron, vol. 71, no. 5, pp. 833–844, 2011.
View at: Google Scholar
M. R. Reynolds, R. W. Berry, and L. I. Binder, “Site-specific nitration and oxidative dityrosine bridging of the τ protein by peroxynitrite: implications for Alzheimer's disease,” Biochemistry, vol. 44, no. 5, pp. 1690–1700, 2005.
View at: Publisher Site | Google Scholar
T. Uehara, T. Nakamura, D. Yao et al., “S-Nitrosylated protein-disulphide isomerase links protein misfolding to neurodegeneration,” Nature, vol. 441, no. 7092, pp. 513–517, 2006.
View at: Publisher Site | Google Scholar
T. Nakamura and S. A. Lipton, “S-nitrosylation of critical protein thiols mediates protein misfolding and mitochondrial dysfunction in neurodegenerative diseases,” Antioxidants and Redox Signaling, vol. 14, no. 8, pp. 1479–1492, 2011.
View at: Publisher Site | Google Scholar
D. H. Cho, T. Nakamura, J. Fang et al., “β-Amyloid-related mitochondrial fission and neuronal injury,” Science, vol. 324, no. 5923, pp. 102–105, 2009.
View at: Publisher Site | Google Scholar
S. A. Austin, A. V. Santhanam, and Z. S. Katusic, “Endothelial nitric oxide modulates expression and processing of amyloid precursor protein,” Circulation Research, vol. 107, no. 12, pp. 1498–1502, 2010.
View at: Publisher Site | Google Scholar
V. L. Dawson and T. M. Dawson, “Nitric oxide in neurodegeneration,” Progress in Brain Research, vol. 118, pp. 215–229, 1998.
View at: Google Scholar
S. Moncada and J. P. Bolaños, “Nitric oxide, cell bioenergetics and neurodegeneration,” Journal of Neurochemistry, vol. 97, no. 6, pp. 1676–1689, 2006.
View at: Publisher Site | Google Scholar
E. P. Meyer, A. Ulmann-Schuler, M. Staufenbiel, and T. Krucker, “Altered morphology and 3D architecture of brain vasculature in a mouse model for Alzheimer's disease,” Proceedings of the National Academy of Sciences of the United States of America, vol. 105, no. 9, pp. 3587–3592, 2008.
View at: Publisher Site | Google Scholar
A. Minagar and J. S. Alexander, “Blood-brain barrier disruption in multiple sclerosis,” Multiple Sclerosis, vol. 9, no. 6, pp. 540–549, 2003.
View at: Publisher Site | Google Scholar
K. H. Jung, K. Chu, S. Y. Ko et al., “Early intravenous infusion of sodium nitrite protects brain against in vivo ischemia-reperfusion injury,” Stroke, vol. 37, no. 11, pp. 2744–2750, 2006.
View at: Publisher Site | Google Scholar

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Copyright © 2012 Ricardo M. Santos 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.

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Nitric Oxide Inactivation Mechanisms in the Brain: Role in Bioenergetics and Neurodegeneration

Abstract

1. Introduction

2. The Interactions of •NO with Biological Targets: Redox and Functional Impact

3. The Transient •NO Change from the Background and the Mechanisms That Regulate Its Profile

3.1. •NO Production in the Brain

3.1.1. Measurement of Nitric Oxide Concentration Dynamics In Vitro and In Vivo

3.2. •NO Diffusion and Half-Life

3.3. Mechanisms of •NO Inactivation

3.3.1. Pathways of •NO Inactivation In Vivo

4. The Functional Impact of •NO in Brain Tissue

4.1. •NO as a Neuromodulator

4.2. Regulation of Mitochondrial Respiration

4.3. Neurovascular Coupling

4.4. Neurodegeneration

5. Novel Perspectives on the Mechanisms Underlying Deregulation of •NO Dynamics in Disease

Acknowledgment

References

Copyright

2. The Interactions of ^•NO with Biological Targets: Redox and Functional Impact

3. The Transient ^•NO Change from the Background and the Mechanisms That Regulate Its Profile

3.1. ^•NO Production in the Brain

3.2. ^•NO Diffusion and Half-Life

3.3. Mechanisms of ^•NO Inactivation

3.3.1. Pathways of ^•NO Inactivation In Vivo

4. The Functional Impact of ^•NO in Brain Tissue

4.1. ^•NO as a Neuromodulator

5. Novel Perspectives on the Mechanisms Underlying Deregulation of ^•NO Dynamics in Disease