Abstract
Parkinson’s Disease (PD) is a neurodegenerative disorder characterized, in part, by the loss of dopaminergic neurons within the nigral-striatal pathway. Multiple lines of evidence support a role for reactive nitrogen species (RNS) in degeneration of this pathway, specifically nitric oxide (NO). This review will focus on how RNS leads to loss of dopaminergic neurons in PD and whether RNS accumulation represents a central signal in the degenerative cascade. Herein, we provide an overview of how RNS accumulates in PD by considering the various cellular sources of RNS including nNOS, iNOS, nitrate, and nitrite reduction and describe evidence that these sources are upregulating RNS in PD. We document that over 1/3 of the proteins that deposit in Lewy Bodies, are post-translationally modified (S-nitrosylated) by RNS and provide a broad description of how this elicits deleterious effects in neurons. In doing so, we identify specific proteins that are modified by RNS in neurons which are implicated in PD pathogenesis, with an emphasis on exacerbation of synucleinopathy. How nitration of alpha-synuclein (aSyn) leads to aSyn misfolding and toxicity in PD models is outlined. Furthermore, we delineate how RNS modulates known PD-related phenotypes including axo-dendritic-, mitochondrial-, and dopamine-dysfunctions. Finally, we discuss successful outcomes of therapeutics that target S-nitrosylation of proteins in Parkinson’s Disease related clinical trials. In conclusion, we argue that targeting RNS may be of therapeutic benefit for people in early clinical stages of PD.
Introduction
Parkinson’s disease (PD) is the most common movement disorder affecting over 10 million individuals worldwide1. PD is characterized by the degeneration of brain cell populations, most notably the dopaminergic neurons emanating from the substantia nigra. Nigrostriatal degeneration correlates with a decline in motor control generally resulting in bradykinesia, rigidity, or tremors. In addition, many non-motor symptoms such as constipation, fatigue or dementia may be concomitant. The neuronal loss in PD is preceded by many phenotypes discussed herein, with a focus on axo-dendritic defects, mitochondrial dysfunction, and synucleinopathy. In this review, we describe how these phenotypes can be attributed to increases in reactive nitrogen species (RNS). We first discuss how RNS is upregulated in PD, we then discuss the effects of RNS on dopaminergic neurons, and then we describe how unchecked RNS leads to aSyn misfolding and Lewy body deposition. In conclusion, we provide an argument that reducing nitrosative stress early in disease may represent a means of delaying phenotypic progression in PD and protecting cells from degeneration.
Sources of reactive nitrogen species in PD
Nitrosative stress results primarily from the over-production of nitrogen based free radicals: nitric oxide (NO−) and nitrogen dioxide (NO2−). These atoms possess unbalanced valence electrons and are therefore highly reactive and prone to filling their outer valance shell with other atoms or molecules. This can lead to production of secondary free radicals such as peroxynitrite (ONOO−) and hydroxide anion (OH−), as well as toxic non-radicals such as hydrogen peroxide (H2O2), dinitrogen dioxide (N2O2), and nitrous acid (HNO2) (Fig. 1). Although many of these are present in healthy neurons, several events can lead to their overproduction which, ultimately damages cellular components leading to neuronal dysfunction and increased severity and area of affliction in a time dependent manner2,3,4. It has been reported that PD patients have elevated RNS as indicated from increased levels of nitrite/nitrate in cerebral spinal fluid5 and blood6. More specifically, in PD it has been reported that white blood cell-neutrophils have higher expression of nNOS and an increased ability to produce excess NO7. In fact, Kouti et al. reported that serum levels of nitric oxide positively correlated with increased UPDRS scores (Universal Parkinson’s disease rating scale) and duration of disease regardless of sex or age6; however, these findings are contentious8,9.
Various formulas showing the production of reactive nitrogen species are displayed (a). The known reactions between RNS and thiols are also shown (b). A cartoon depicting the primary effects of various RNS and their intermediates (c). This figure was created using Biorender.
Increased enzymatic activity of NOS is elevated in the PD brain
Neuronal nitric oxide synthetase (nNOS) is the primary source of nitric oxide (NO) production in neurons. nNOS is a 161 kda enzyme encoded by the NOS1 gene. Each nNOS has an oxygenase and reductase domain connected by a linker that is responsible for calmodulin binding. The generation of NO occurs in two-steps, both requiring oxygen, NADPH, and an nNOS dimer (zinc facilitates the dimerization of nNOS, enabling nNOS activity). First, intracellular Ca2+ catalyzes the binding of nNOS to calmodulin and, in the presence of heme, hydroxylates L-arginine to N-hydroxy-L-arginine. In this step, co-factors FAD and FMN aid the electron transfer from the NADPH by the nNOS to the heme. Second, N-hydroxy-L-arginine is oxidized to L-citrulline and NO with the aid of L-arginine and co-factor BH4 (Fig. 2). There are at least four splice variants of nNOS: nNOSα, nNOSβ, nNOSγ, and nNOSμ. nNOSα is the most dominant variant, primarily found in neurons. nNOS contains a PDZ domain which allows its interaction with other PDZ-domain containing proteins, thus influencing the cellular localization of NOS. As such, nNOS is often localized at the synaptic membrane due to its PDZ-interaction with PSD95 and PFK-M, for example.
NOS may be activated by various ions, proteins, or enzymes. To produce nitric oxide, NOS requires oxygen, NADPH and L-arginine. The reductase (containing FMN) and oxygenase (heme-containing) domain are bound by calmodulin (CaM). To produce nitric oxide, oxygen and NADPH enter the reductase domain facilitating the transfer of the electron from the FAD, to the FMN, to the heme. This electron, along with oxygen, is needed to convert L-arginine into N-hydroxyl-L-arginine (monooxygenase reaction I). Next, a second monooxygenase reaction involving an electron, oxygen molecule and co-factor BH4 occurs to convert N-hydroxyl-L-arginine to L-citrulline and nitric oxide (NO). BH4 is oxidized to BH2, which can then be reduced back to BH4, balancing NOS dimers in an on (coupled)/off (uncoupled) state. NOS subunits are held together by zinc (Zn) ions that bind the oxygenase domains. Output from NOS includes L-citrulline, water, NADP and nitric oxide. This figure was created using Biorender.
Post-mortem analysis of midbrain samples revealed that nNOS expression is increased in brain regions of PD patients relative to controls10. nNOS activity is also upregulated in animal models of PD11,12. Similarly, in weaver mice where the spontaneous depletion of dopaminergic neurons occurs, nNOS is increased in the substantia nigra but not in other brain regions13. Together these findings implicate nNOS activity in PD pathogenesis. nNOS activity is highly regulated by post-translational modifications and interacting proteins. For example, the phosphorylation of Ser847 is inhibitory, while de-phosphorylation of Ser847 stimulates nNOS activity14. Perhaps it is not surprising that docosahexaenoic acid, a supplement that phosphorylates nNOS (i.e., inhibits nNOS activity) protects dopaminergic neurons from MPTP toxicity in rodent models of PD15. In addition, while a number of nNOS interacting proteins have been identified, HSP90 (heat-shock protein 90) has been demonstrated to be an important regulator of protein homeostasis and plays a specific role in preventing aSyn aggregation16 ascribing it significance in PD. While these findings seem to suggest that HSP90 may have a protective role in PD, HSP90 has also been shown to interact with and amplify nNOS activity17 thereby contributing to RNS. In cell models of PD, HSP90 inhibitors have been shown to protect against PD-related phenotype induction by preventing neurite loss and even aSyn aggregation18,19. Likewise, knockdown of nNOS using siRNAs protects dopamine neurons in cell and animal models of PD20. Together these findings suggest that nNOS is upregulated in PD and that suppression of nNOS activity may prevent PD pathogenesis.
Another relevant isoform of NOS is inducible nitric oxide synthase (iNOS), which is expressed by glial cells such as astrocytes and macrophages. iNOS is an enzyme ~131 kDa in size, encoded by the NOS2 gene. Like nNOS, iNOS consists of two domains; an oxygenase and reductase domain which facilitates the binding of calmodulin and the subsequent production of NO through a series of electron transport events. Its activity is regulated by protein interactions (e.g., kalirin), substrate and co-factor availability (cationic amino acid transporter L-arginine). Unlike the constitutive expression of nNOS in neurons, iNOS is stimulated, hence the term “inducible”. An operative distinction between iNOS and nNOS is the ability of iNOS to bind to calmodulin at much lower concentrations of calcium making NO production from iNOS tenfold that of nNOS-NO production21.
Elevated levels of iNOS have been found post-mortem in multiple neurodegenerative diseases including Parkinson’s-patient brains22. In support of this observation, there is heightened iNOS expression in multiple animal models of PD using 6-OHDA23, MPTP24, and even aSyn oligomers25 whereas mice lacking iNOS are resistant to many PD-inducing stressors26. Moreover, glial cells readily populate brain regions with active neurodegeneration, increasing the potential for high NO levels that can further exacerbate toxicity in surrounding cells.
Nitrate reduction as a means of RNS generation
Independently of NOS family members, nitrate (NO3−) and nitrite (NO2−) can be reduced to NO or other RNS. Nitrates and nitrites are commonly sourced from diet, most notably vegetables. The reduction of NO3− to NO2− is most frequently catalyzed by the gastro-intestinal microbiome which uses NO2− to produce energy and, in turn, generates nitrogen oxide by-products that can be absorbed into the body via the GI-tract. Alternatively, the reduction of NO3− can be catalyzed by mammalian NO3− reductases (e.g., Xanthine oxidase)27 or in mitochondria at complex III/ubiquinol complex28. NO2−, utilized as an NO reserve, is circulated throughout the body and further reduced to NO with the help of enzymes (eg. xanthine oxidoreductase, aldehyde oxidase), carrier proteins (e.g., deoxyhemoglobin, neuroglobin), or co-factors (e.g., ascorbic acid) in various tissues. Indeed, dietary NO3− increases NO2− availability to the brain29 where high levels of ascorbate might facilitate the conversion of NO2− to NO30. It has been further hypothesized that NO2− reduction in the brain may replace NOS-derived NO production when NOS is compromised, as in states of hypoxia or ischemia31. This event may occur at mitochondria32. NO may further react with other nitrogen oxide, oxide, or superoxide radicals to produce the potent nitrating agents ONOO−, N2O3, or NO2. Whether dietary-derived NO3− or NO2− contribute significantly to NO in the brain remains unclear, yet a link between gut microbiome and phenotypic PD-onset has recently been proposed33,34.
It is reported that PD patients have altered gut microbial ecosystems relative to healthy controls. More specifically, PD patients have decrease short chain fatty acids (causing decreased vitamin levels) as well as small intestinal bacterial overgrowth, which perpetuates oxidative and nitrosative stress in the gut. Patients also have increased levels of gut-aSyn relative to healthy controls, and this is observed years before motor symptoms arise35. Indeed, in the last decade several groups have put forth studies that support the theory that PD originates in the gut and that overtime pathology spreads into the brain. This is believed to be possible through the connectivity of the enteric neurons located in the gastrointestinal wall and the central nervous system. The theory postulates that external stressors stimulate an immune response in the gut, which triggers and seeds pathology from the enteric system to the brain via the vagal nerve33. In support of this, evidence suggests that pathological (or misfolded) aSyn inoculated into the duodenum can spread from the gut into the brain of rodents36 and that severing the vagal nerve inhibits this phenomenon37. Furthermore, oral administration of the pesticide rotenone triggers synucleinopathy, which spreads from the GI into the brain of inoculated mice34. This indicates that toxins that elicit an oxidative stress response in the gut are capable of triggering PD related synucleinopathy. A study by Sampson et al. suggested that gut microbiota may dictate PD-motor phenotypes; as PD-patient fecal transplants into germ free animals triggered locomotor deficits, whereas fecal transplants from healthy human donors had no effect on locomotor function. In the same study, Sampson et al. demonstrated that synucleinopathy itself was markedly reduced in germ-free mice despite aSyn overexpression38. As gut-brain connectivity is bi-directional, it is plausible that PD pathologies might also spread from the CNS into the gut. Indeed, 6-OHDA induced nigral-striatal brain lesions caused a reduction in fecal output39, further asserting a relationship between the gut and brain. Moreover, transgenic human-aSyn and MPTP-induced murine models of PD display GI-dysfunction such as constipation in parallel with aSyn accumulation40. Fecal transplantation to MPTP-induced PD mice reduced PD-phenotypes41 suggesting that unidirectional gut-to-brain communication predominates with respect to the influence on motor phenotypes. It is therefore interesting to speculate as to whether NO3− or NO2− imbalance in the gut contributes to the spread of synucleinopathy from the enteric nervous system to the central nervous system.
RNS-induced pre-degenerative dysfunction of dopaminergic neurons
NO-mediated alterations axo-dendritic function
As discussed above, nNOS contains a PDZ domain that confers binding capacity to many post-synaptic density-proteins (e.g., PSD93/95, PFK-M, CAPON, and syntrophin) and is therefore regionally distributed along synaptic spines. This localization is key to its canonical function, which is to promote NO-mediated second messenger signaling. In this way, NO reacts with guanylyl cyclase to produce cyclic guanosine monophosphate which is important for regulating neuronal dynamics including outgrowth and synaptic plasticity42. In addition, NO has a major role in regulating synaptic activity through s-nitrosylation and/or transnitrosylation of proteins43,44,45. In the healthy state, NO protects neurons from hyperexcitability by s-nitrosylating and inhibiting NMDARs (SNO-NMDAR)46. Choi et al. were the first to describe the mechanism whereby NO inhibits the NMDAR via s-nitrosylation of cysteine 399 on the NMDAR-subunit NR2A46. NO has also been shown to protect neurons from hyperexcitability by regulating AMPAR expression, a major component of ionotropic glutamate signaling. AMPAR surface expression is increased (SNO-Stargazin) or decreased (SNO-Thorase) in response to S-nitrosylation of respective regulatory proteins47,48. Moreover, in neurons NO itself can act as a neurotransmitter; regulating calcium signaling49, stimulating extracellular vesicle release and endocytosis50, and is even involved with learning and memory formation through its activation of CREB51 and retrograde transmission from the post- to pre-synaptic terminal, stimulating neurotransmitter release and long-term potentiation52. However, when in excess, as is the case in PD-neurons, NO alters axo-dendritic function impairing synaptic signaling, vesicular trafficking, and dopamine homeostasis (Fig. 3).
This schematic highlights the major phenotypes that arise as a consequence of RNS in PD. This includes axo-dendritic defects (a), mitochondrial defects (b) and dopamine-induced defects (c) discussed in this review. This figure was created using Biorender.
The aberrant s-nitrosylation of synaptic proteins is believed to lead to the dysregulation of synaptic activity in PD-neurons. While the exact effects of superfluous NO or its derivatives on synaptic function in PD have not been fully elucidated, there is evidence that excess NO alters axo-dendritic function, specifically impairing neurite length through the S-nitrosylation of protein disulfide isomerase or microtubule associated protein 1b, and causing synaptic spine loss through the hyperactivity of Cyclic-dependent kinase 5 (CDK5) following CDK5 S-nitrosylation53,54. These axo-dendritic impairments alter network connectivity, which is associated with cognitive decline and even neuronal death. NO also regulates NMDAR-excitotoxicity55 that can be further exacerbated by SNO-Src and SNO-SHP-256,57. Src, a family of proteins tyrosine kinases, was found to be activated by autophosphorylation and S-nitrosylation leading to the phosphorylation of NMDAR subunit NR2B and the subsequent increase of NMDAR activity. Additionally, NMDAR excitotoxicity is also regulated by SHP-2, a Src homology-2 domain containing phosphatase. SHP-2 has been shown to promote cell survival via ERK1/2 pathway, while nitrosylation of SHP-2 inhibits its phosphatase activity. Indeed, NMDAR-dependent calcium influx triggers nNOS to generate NO thereby compounding the effects of SNO-Src and SNO-SHP-2 and further contributing to NMDAR-mediated excitotoxicity. Moreover, NO has been shown to induce the synthesis of NO per se58, indicating that the superfluous levels of NO in PD might lead to a vicious loop of NO production.
Recent evidence suggests another important function of NO is to regulate intracellular trafficking of vesicles and cargo. We and others have shown that PD patient derived dopaminergic neurons are particularly susceptible to nitrosative stress59,60. These studies demonstrated that low doses of agrochemicals, which had no effect on isogenic control neurons, caused the nitration of tubulin and impaired KIF5b transport of mitochondria in neurons harboring aSyn mutations61. Moreover, Redondo et al. show that NO reduces KIF5A and KIF21B expression in neurons62, suggesting that an upregulation of NO in PD would cause a reduction of anterograde trafficking. The loss of kinesin-driven axonal transport would likely have many consequences for neurons such as (1) energetic deficits given that cells would have impairments in transport of metabolic enzymes. This defect would particularly affect energy production at the synapse where there exists a large energetic demand. We can speculate that another consequence of decreased transport in neurons would be (2) reduced neurotransmitter production, given that enzymes that synthesize neurotransmitters are required to be trafficked to the synapse via vesicles. The latter defect may be exacerbated by the S-nitrosylation of VMAT2 (vesicular monoamine transporter)63, which has been shown to be important for the transport of enzymes responsible for dopamine synthesis (e.g., tyrosine hydroxylase and AADC) as well as important for storing dopamine in vesicles to protect dopamine from oxidation and degradation. Ultimately, Redondo et al. show that the loss of kinesin proteins led to a reduction in axonal length and neuron survival62.
Effects of NO on mitochondrial function in neurons
In a healthy system NO has been ascribed a role in regulating mitochondrial function. In 1994, Brown and Cooper provided evidence that NO alters mitochondrial respiration. They showed that in isolated synaptosomes low levels of NO compete with oxygen to inhibit or activate cytochrome c, respectively64. Since mitochondria cluster to regions where the demand for ATP is heightened, such as the synapse, it is possible that NO regulates mitochondrial oxygen consumption in order to maintain ATP supply. This regulation would be particularly important in the context of substantia-nigral dopaminergic neurons given their complex arborization and pace-making activity. Moreover, substantia-nigral dopaminergic neurons have fast spiking Ca2+ transients that increase the intracellular concentration of Ca2+ that is subsequently buffered, in part, by mitochondria. Not only does this put mitochondria at risk for Ca2+ overload leading to excitotoxicity and/or apoptosis, but Ca2+ that is not buffered may further stimulate nNOS-generated NO. Together, mitochondrial- NO reacts with superoxide produced by mitochondria to promote the production of the highly toxic ONOO−. Studies have shown that ONOO− can impair mitochondrial-ATP synthesis through inhibition of mitochondrial respiratory complexes, mitochondrial polarization, and detoxifying enzymes in addition to promoting mitophagy65,66.
Many mitochondrial-related proteins are reported to be S-nitrosylated, both endogenously and in response to stimuli. Indeed, Chang et al. used the biotin-switch LC-MS/MS method to detect S-nitrosylated proteins in isolated rat brain-derived mitochondria identifying s-nitrosylated mitochondrial targets that include: pyruvate dehydrogenase, succinyl-CoA ligase, complex I, VDAC (voltage dependent anion channel), and prohibitin (PHB)67. Still others have performed various SNO-capture methods (SNOSID, SNOTrap, Phenylmercury (MRC)) on whole brain extracts or primary cultured neurons to generate global lists of SNO-modified proteins. While the implications of each of these modifications have not been fully elucidated, the exuberant increase in RNS in PD would likely increase the number of mitochondrial targets nitrosylated in the disease setting. Studies indicate that the S-nitrosylation of the electron transport chain, the citric acid cycle, carnitine/acylcarnitine transporter and the nitration of HSP90 impairs metabolism68,69. Together, these studies suggest that RNS-altered mitochondrial targets leads to a loss of function. On the other hand, the nitrosylation of voltage-dependent anion channel 1, a component of the mitochondrial permeability transition pore, is believed to trigger the opening of the channel leading to a gain of function67. Consequently, this leads to Ca2+ dyshomeostasis and mitochondrial depolarization, cytochrome c release and apopotosome formation, permeabilization of the outer mitochondrial membrane as well as causing the hyperproduction and release of O2− and H2O2 leading to other free radical damage70. It has, however, been reported that the effects of NO on VDAC is concentration dependent: low doses of NO block the channel, while high doses of NO open the channel71. While we have just described some of the deleterious effect of RNS on mitochondrial proteins, the specific effects in PD remain poorly characterized.
In addition to mitochondrial proteins that can be nitrosylated, extra-mitochondrial proteins that affect mitochondrial function are susceptible to nitrosylation or nitration leading to altered mitochondrial dynamics. For instance, while nitrosylation of CREB may enhance its ability to bind DNA and leads to the upregulation of mitochondrial-biogenesis genes72, the nitration of PPAR has been shown to impede the expression of mitochondrial proteins73. Parkin (i.e., Park2) is an E3 ubiquitin ligase that is believed to play an important role in directing misfolded proteins for degradation via the ubiquitin-protease system74 and helps regulate mitochondrial dynamics through mitochondrial biogenesis, import of mitochondrial proteins and mitophagy (targeting mitochondria to phagosomes)75. In humans, Parkin mutations are associated with autosomal recessive familial PD. Moreover, SNO-Parkin is more present in PD patients and in rotenone or MPTP-treated mice than controls76,77. SNO-Parkin leads to mitochondrial depolarization whereas SNO-PINK1 decreases Parkin translocation to mitochondrial membranes, disrupting mitophagy78,79. In addition, the S-nitrosylation of the mitochondrial chaperone protein PHB has actually been shown to be neuroprotective against stress evoked by oxygen and glucose deprivation80; however, PHB’s expression is reportedly reduced in PD patient brains81 suggesting PD neurons are more susceptible to this stress. In PD patient brain tissue and cellular models of PD, S-nitrosylation of peroxiredoxin (PrxII) decreases peroxidase activity causing H2O2 to accumulate, exasperating oxidative stress82.
Effects of NO on dopamine homeostasis in neurons
The unique susceptibility of dopaminergic neurons to nitrosative stress, may relate to dopamine synthesis and catabolism. Indeed, the dopamine synthesizing enzyme tyrosine hydroxylase can be inactivated by tyrosine nitration, reducing intracellular dopamine levels83,84. In addition, NO also catalyzes the auto-oxidation of dopamine (via quinones and semiquinones)85 causing protein-, lipid-, or DNA- dopamine-adducts that can lead to neurodegeneration. What’s more, dopamine itself can react with many RNS including nitric dioxide, nitrogen dioxide and dinitrogen trioxide forming 6-nitrosodopamine which can further react with RNS to produce 6-nitrodopamine which can then produce other radicals and RNS86. Together these findings suggest that dopaminergic neurons are vulnerable to nitrosative stress due, in part, to the presence of dopamine per se. RNS-altered dopamine may dysregulate dopamine homeostasis and further intensify RNS.
The effects of RNS on mitochondria also has specific implications for dopaminergic neurons since the breakdown of dopamine by the mitochondrial localized enzyme monoamine oxidase produces the metabolite 3,4-dihydroxyphenylacetic acid (DOPAC) whose interaction with NO can impair mitochondrial respiration87. The combination of DOPAC and NO was shown to also cause a decrease in glutathione88. Glutathione, a thiol-reducing agent and antioxidant responsible for the breakdown of H2O2, is known to be dysregulated in PD patients. Indeed, decreasing glutathione synthesis in dopamine cells causes the inhibition of mitochondrial complex I in either a NO- or ONOO−-dependent manner, depending on whether the treatment was acute or chronic, respectively89,90. While the nature of the interaction between NO, DOPAC and complex I remains elusive, it is likely to play a part in the early decline of dopaminergic neurons in PD.
Role of RNS in protein misfolding and Lewy Body deposition
Alpha-Synuclein protofibril formation in PD
Many causal aSyn mutations have been identified (A30P, A53T, E46K, G51D, duplication, and triplication) in PD patients. While familial forms of PD only account for about 10% of cases, the presence of aSyn in Lewy-bodies of sporadic PD cases highlights its importance to multiple disease stratifications. Although the processes driving Lewy body formation are not well understood, much is known about how aSyn fibrillization contributes to Lewy Body pathology. aSyn is a 14 kDa protein consisting of three domains: the amino-terminus, the non-amyloid β-component (NAC), and the carboxyl-terminal domain. In solution, aSyn exists primarily as an unstructured random-coil. Since the amino-terminus is amphipathic, consisting of seven KTKEGV repeat sequences, aSyn reconfigures into an α-helical form when bound to anionic phospholipid membranes. Although the function of aSyn remains poorly characterized, most evidence supports functions at the synapse, regulating vesicle storage, dopamine synthesis and neurotransmission. When misfolded, aSyn represents the major component of β-sheet-rich cytoplasmic inclusions within Lewy bodies, which accumulate prior to neurodegeneration in PD. Prior to deposition into Lewy bodies, aSyn protofibrils (or oligomers) accumulate. In PD, aSyn oligomers are conformationally self-templating and able to cross-seed with other structural conformers of aSyn91. What’s more, oligomers actively recruit other proteins into aggregates92. aSyn oligomers can also propagate between cells through synaptically linked regions of the brain93,94, exo-endocytosis95, tunneling nanotubes96 or by receptor mediation (e.g., Lag3)97 leading to the pathological spread of synucleinopathy. aSyn oligomers can also permeabilize lipid membranes98, trigger mitochondrial dysfunction99, proteostatic stress100,101,102, and impair synaptic function103. Although the pathological progression of aSyn and Lewy Body pathology can be variable, the patterning is typically predictive: beginning in the medulla, continuing into the midbrain, and finally infecting the cortex104. It remains controversial whether aSyn per-se or mature Lewy bodies ultimately trigger cell death. While Lewy-bodies appear to trigger cell death by blocking intracellular-transport as well as impairing mitochondrial and synaptic function, they may develop in response to sequestration of aSyn oligomers that are highly toxic.
RNS potentiates aSyn misfolding and pathological deposition
Nitration of aSyn can potentiate aSyn-oligomer formation. Oxidative modification to tyrosine can occur in one of two ways: a hydrogen atom in the 3′ position of a tyrosine ring can be replaced with a nitro-group (3-Nitro-Tyrosine (3NT)), or tyrosines can react with each other to form 3,3′-dityrosine crosslinks. Exposure of aSyn to nitrating agents can encourage o,o′-dityrosine crosslinking between the N-domain tyrosine (Y39) and C-terminal tyrosines (Y125, Y133, Y136) to generate aSyn-dimers that are more prone to oligomer formation105,106,107,108. Perhaps unsurprisingly, mutated aSyn (A30P and A53T) has an increased propensity for dityrosine cross-linking107. Additionally, tyrosines play an important role in aSyn-vesicle binding while nitration impairs this interaction (making the charge more negative at the N-terminal domain, or causing a conformational change when the C-terminal domain is nitrated) thereby increasing the amount of aSyn in a random coil or beta-sheet conformation and thus shifting equilibrium toward oligomer formation105,106,109. It has also been suggested that nitrated aSyn promotes the seeding of aSyn-oligomers from cell-to-cell110.
There exists evidence that nitration of aSyn can also potentiate fibril formation. In cells exposed to ONOO−, formation of aSyn aggregates is dependent on nitro-tyrosine adduct formation111, supporting the notion that that protein nitration may serve as a biomarker of PD. Indeed, nitrated aSyn is almost exclusively found in the insoluble protein fraction making aSyn more resistant to degradation, more compact, and more stable112,113. Moreover, mutating aSyn-tyrosine Y39 residue to phenylalanine reduces the ability of aSyn to fibrilize105,113. Many studies have also demonstrated that nitrating-aSyn through the addition of nitrating agents (eg. ONOO− or TMN) promotes non-amyloidogenic β-sheet oligomers and dimers, as opposed to fibrils105,112,113,114. In this way, it has been suggested that nitration of aSyn might occur post-fibril-formation and function to stabilize aSyn in its new form. Taken together, these studies suggest that tyrosine nitration can augment fibril formation by promoting dityrosine crosslinking capable of seeding pathology and may in addition represent a post-fibril modification that functions to stabilize fibrils.
In PD patients, aSyn itself was shown to be at least one target of nitration in PD-patient brain samples. Indeed, higher RNS and nitrated aSyn in PD-patient serum levels correlates with worsened PD-related outcomes115. Moreover, nitrated aSyn was specifically identified within Lewy-body-like and insoluble inclusions116. Overexpression of aSyn in HEK293 cells lead to intracellular inclusions following exposure to a NO donor and oxidizing agents or ONOO−111,117. Likewise, in mice treated with MPTP, which causes the degeneration of dopaminergic neurons, immunoprecipitation of aSyn and subsequent western-blot analysis indicated that aSyn was nitrated as early as 4 h following MPTP treatment117. Despite the fact that very few proteins undergo nitration, increased levels of nitrated-aSyn in PD patients suggests that nitration might be linked to PD-pathology.
Nitrated-aSyn likely has many functional consequences. An in vitro assay by Mishizen-Eberz et al. demonstrated that nitrated aSyn fibrils were able to be cleaved by calpain1 just as un-nitrated aSyn-fibrils were. However, the authors noted that the cleaved fibrils from nitrated-aSyn formed uniquely structured fragments which were wider and had a more exposed NAC domain relative to the cleavage of un-nitrated aSyn fibrils. In addition, the nitrated-aSyn fragments promoted the recruitment of soluble aSyn into its aggregate118, suggesting that the nitration of aSyn might seed pathology more efficiently than non-nitrated aSyn fibril-fragments. Moreover, nitration of aSyn has been shown to increase the rate of fibrillization and simultaneously slow the rate of proteolytic degradation (e.g., cleavage by calpain1)106. In addition, when cells and mice were exposed to aSyn or nitrated-aSyn, the nitrated aSyn was more toxic as it causes dopamine-cells to degenerate and mice to perform more poorly on behavioral motor-coordination assays119.
Increased aSyn correlates with increases in RNS
There exists evidence that strongly suggests a positive-feedback correlation between aSyn and RNS. Several reports have determined that aSyn accumulation leads to increased NO generation and s-nitrosylation of proteins implicated in PD pathogenesis. In brains of sporadic PD patients with diffuse Lewy bodies, s-nitrosylation of Parkin120, p53120, PTEN, and DJ-1121 have been reported that result from an interlinked mechanism of trans-nitrosylation leading to degeneration of nigral neurons. aSyn overexpressing transgenic mice show elevated levels of S-nitrosylated Parkin and PINK1 and defects in mitochondrial quality control79, whereas aSyn-knockout cells and mice are resistant to the deleterious effects of RNS elicited by exposure to MPP+ or LPS122. That parkin is heavily nitrosylated in models of aSyn overexpression is perhaps not surprising given reports that Parkin cysteine oxidation is linked to redox balance in human midbrain123 and that Parkin suppresses unfolded protein stress-induced cell death124. Studies from human stem-cell-derived dopaminergic neurons have shown that neurons harboring the endogenous aSyn-A53T mutation have increased kinetics of NO synthesis and are more susceptible to RNS-toxins59,61. Moreover, mutant aSyn (A53T and E46K) neurons have increased basal levels of S-nitrosylated proteins relative to isogenic controls. In fact, when considering reports on the constituents of Lewy Bodies125, one third of the proteins deposited are modified by S-nitrosylation (Table 1). With respect to protein nitration, Tapias et al. showed that inoculation of aSyn preformed fibrils into mice and nonhuman primate brains caused an accumulation of 3NT-modified proteins, particularly in dopaminergic neurons25. Together, these findings suggest crosstalk between aSyn and RNS with respect to pathological deposition of protein aggregates in PD.
Targeting RNS as a PD therapy
Reducing RNS by targeting NOS
Upregulating proteins that interact with or inhibit nNOS activity may represent a means of mitigating PD pathogenesis. The specific nNOS inhibitor 7-nitroindazole protects against dopaminergic neuron depletion in animals treated with 6OHDA126 or MPTP12, even preventing motor impairments such as apomorphine induced contralateral rotations127 and catalepsy12. nNOS inhibition by Nwnitro-L-arginine methyl ester can reduce NO accumulation in human induced pluripotent stem cell (hiPSC)-derived PD neurons (harboring the A53T-SNCA mutation) protecting neurons from mitochondrial dysfunction61 and rescuing axodendritic pathology128. Likewise, treatment with docosahexaenoic acid causes the phosphorylation of nNOS that in turn decreases nNOS activity preventing PD-like motor deficits in MPTP treatment in mice15. While inhibiting NOS may seem to be an obvious therapy, this is complicated by the fact that nitric oxide is integral for physiological function, particularly for the vascular system. In addition, NO inhibition has been shown to be related to insulin resistance and can cause other adverse side effects.
As an alternative to NOS inhibition, gene silencing by interfering RNAs (iRNAs) could degrade RNAs that are integral for NOS synthesis. iRNAs are delivered to cells through viral (e.g., nanoparticle or liposomes) non-viral vectors (e.g., adeno-associated virus or retrovirus). Similar to the protection from PD-phenotypes exhibited by nNOS knockout mice129, striatal inoculation of iRNA targeting-nNOS reduced 6-OHDA toxicity by preventing dopaminergic neuron degeneration and behavioral impairments in rats20. Clinical trials are ongoing that employ the use of iRNAs for PD, thus specific targeting of NOS in the SNpc to decrease RNS may be feasible in the future.
Antioxidants to reduce RNS
Some studies have shown that scavenging RNS may also be one way to attenuate PD pathologies. One way to accomplish this is to inhibit NADPH oxidase (NOX), which is responsible for the formation of O2− and, subsequently, the formation of ONOO−. In vitro experiments by Schildknecht et al. showed that the NOX inhibitor GTK136901 reduced the amount of ONOO−, prevented alpha-synuclein nitration, and protected human dopaminergic cells from ONOO− toxicity130. Similarly, minocyclin, a scavenger of ONOO− [194], has also been shown to reduce ONOO− in a LPS model of PD, preventing 3-NT immunoreactivity131. Moreover, minocyclin has also been shown to prevent 6-OHDA and MPTP dopaminergic neuronal degeneration though its inhibition of iNOS-produced NO132,133. Together, these findings suggest a dual-role mechanism of action for minocyclin (1) scavenging ONOO− and (2) inhibiting iNOS in glial cells. Indeed, a number of other NOX inhibitors are being studied for their therapeutic potential in PD134.
There has been some interest in repurposing the drugs simvastatin (i.e., Zocor) or dimethyl fumarate (i.e., Tecfidera) for PD. These drugs are relevant as they function to activate NRF2 which upregulates antioxidant response enzymes to mitigate ROS/RNS135,136. NRF2 is released from its repressor (KEAP1) allowing NRF2 to translocate to the nucleus and transcribe >800 genes, including phase i enzymes involved in the metabolic detoxification pathway and phase ii conjugation enzymes that metabolize functional groups. Particularly important to the regulation of RNS, NRF2 activity upregulates enzymes such as thioredoxin and GCLC, the rate limiting enzyme in glutathione synthesis. Glutathione can react with NO to form GSNO which acts as an NO reserve. Glutathione also regulates GSNO(R) reductase (i.e., AHD5) which, together with thioredoxin, reduces protein S-nitrosothiol groups (Fig. 4). Studies suggest that both simvastatin and dimethyl fumarate are neuroprotective in animal models of PD137,138,139,140,141. Indeed, dimethyl fumarate can rescue antioxidant enzyme expression as well as increase neuritic arborization and complexity in hiPSC-derived dopamine neurons harboring the A53T aSyn mutation128. While results from the Simvastatin clinical trial have yet to be reported and trials using dimethyl fumarate have yet to commence, there is reason to be hopeful that a drug targeting RNS may be effective for PD therapy.
Two major de-nitrosylation pathways reduce s-nitrosocysteine in cells: the thioredoxin reductase (Trx) family of redox sensors that includes Glutaredoxin (Grx), and the indirect S-nitrosoglutathione reductase (GSNOR) system. a Trx removes the s-nitrosyl-group from the protein-SNO (either through Trx-mediated trans-nitrosylation or Trx-disulfide-bond formation within the protein-SNO) and then b generates a disulfide bond, freeing HON or NO + H+. Alternatively, the GSNOR system c first requires that glutathione (GSH) react with the s-nitrosocysteine of an S-nitrosylated protein, transferring the nitrosyl-group to the thiol of the cysteinyl-group of GSH generating GSNO. d Next, the enzyme S-nitrosoglutathione reductase (GSNOR) and co-enzyme NADH catalyzes the conversion of GSNO to an N-hydrosulfinamide (GSNOH) intermediate and subsequently to glutathione-disulfide (protein-GSSG) and hydroxylamine (not shown). e Protein-GSSG is then reduced to GSH through the activity of glutathione reductase (GR) and co-enzyme NADPH. f The Grx member of the Trx family has two modes of SNO reduction. Grx can form an oxidized Grx intermediate (Grx-SNO) on one cysteine residue following transfer of the nitrosyl-group from protein-SNO. This can either be reduced though the GSH pathway described above (mono-thiol reaction) or through the traditional Trx system (diol-thiol reaction) by producing a disulfide bond. g The now oxidized Grx is reduced by two GSH molecules to restore the cycle. This figure was created using Biorender.
Additional clinical trials have aimed to improve the antioxidant response in PD, including the study of lithium, hydrogen, Deferiprone and N-acetylcysteine. The aforementioned drugs exhibit neuroprotective actions in PD models; reducing oxidative/nitrosative stress, aSyn aggregation or nitration, and activating anti-apoptotic pathways142,143,144,145,146,147,148,149,150. While early findings from clinical trials show that the protective effects of hydrogen and deferiprone did not reach statistical significance151,152,153, N-acetylcysteine (NAC) shows promising efficacy. NAC is a membrane-permeable form of cysteine, a precursor for glutathione. In vitro studies using PFFs to induce synucleinopathy in primary neurons showed that treatment with NAC reduced aSyn aggregates and oxidative stress154. Likewise, many animal models of PD show that oral administration of NAC rescued dopaminergic neuron loss, reduced oxidative stress, and improved motor outcomes154,155,156,157. To date, clinical trials investigating the effectiveness of NAC demonstrate that the oral coupled with intravenous administration of NAC increases the expression of the dopamine transporter and shows modest improvement in UPDRS scores in PD patients158,159. While these results suggest NAC-treatment may be one potential strategy for reducing RNS in PD, the limited bioavailability of oral NAC in brain tissue and need for intravenous administration may limit its widespread use.
Targeting alternative de-nitrosylating proteins
Since the nitrosylation of proteins has deleterious effects with immediate implications for PD, targeting this modification may offer therapeutic benefit. For example, S-nitrosylation of peroxireductase (Prx2) has been shown to impair the H2O2 reductase capacity of Prx2, resulting in increased oxidative stress. SNO-Prx2 has been found to be more abundant in PD models than controls82. In light of this, preventing this and other SNO-modifications might be an important step in mitigating PD pathology. Sunico et al. identified that the overexpression of sulfiredoxin (Srxn1), an enzyme responsible for the de-nitrosylation of SNO-Prx2, protected dopaminergic neurons from the effects of paraquat/maneb treatment in both mice and hiPSC-derived dopaminergic neurons120.
Perhaps the most well-studied protein for its nitrosylated/de-nitrosylated function in PD is Parkin. The oxidation of Parkin leads to its aggregation which reduces its ability to act as a redox sponge123. Recent reports indicate that the protein DJ-1 regulates SNO-parkin (and the S-nitrosylation of other proteins) via trans-nitrosylation78,121 as recently reviewed by Sircar and colleagues160. Moreover, inactivating DJ-1 mimics PD-related mitochondrial dysfunction78. Besides regulating SNO-Parkin, SNO-Dj-1 itself also represents a potential PD therapeutic target since DJ-1 plays a role in activating the antioxidant response, cellular metabolism, cell survival, and redox homeostasis160. However, the specific function of SNO-Dj-1 vs. de-nitrosylated Dj-1 have yet to be elucidated. Future research that identifies supplementary de-nitrosylating proteins may provide valuable information for the removal of SNO-modification and rescuing PD pathology.
In summary, the effects of RNS in PD are multifaceted. Herein, we describe the sources of RNS in neurons and provide evidence that RNS is implicated in PD. Accumulating evidence suggest that RNS exacerbates the rate of disease progression by promoting aSyn misfolding and accelerating deposition of aSyn aggregates. The sheer number of s-nitrosylated proteins that deposit in Lewy Body aggregates suggests that RNS, once triggered, is accelerating not only aSyn aggregation but the aggregation of many proteins critical to neuronal survival and function. This culminates in (1) axo-dendritic pathology coupled to loss of synaptic function, (2) impaired mitochondrial dynamics coupled with altered energy homeostasis, and (3) impaired dopamine metabolism, all of which contribute to further RNS imbalance. Thus, reducing or controlling RNS accumulation early in disease etiology may have multimodal benefits to people with PD. This is supported by positive outcomes in clinical trials for NAC showing rescue of dopamine levels and improved function in patient cohorts. While NAC use is limited by its poor bioavailability in brain tissue, these results may indicate that de-nitrosylating proteins of the Trx family such as (Grx, Srxn1and Prx2) may represent a new class of disease modifying targets against PD. Future studies should explore whether de-nitrosylating proteins are targetable and effective in diseased populations.
Data availability
Data sharing is not applicable to this article as no datasets were generated or analyzed during the current study.
Code availability
Code sharing is not applicable to this article as no datasets were generated or analyzed during the current study.
Change history
19 September 2022
A Correction to this paper has been published: https://doi.org/10.1038/s41531-022-00390-z
References
Statistics, https://www.parkinson.org/Understanding-Parkinsons/Statistics (2022).
Pang, S. Y. Y. et al. The interplay of aging, genetics and environmental factors in the pathogenesis of Parkinson’s disease. Transl. Neurodegener. 8, 1–11 (2019).
Collier, T. J., Kanaan, N. M. & Kordower, J. H. Aging and Parkinson’s disease: different sides of the same coin? Mov. Disord. 32, 983–990 (2017).
Grimm, A. & Eckert, A. Brain aging and neurodegeneration: from a mitochondrial point of view. J. Neurochem. 143, 418–431 (2017).
Santos-Lobato, B. L. et al. Levodopa-induced dyskinesias in Parkinson's disease increase cerebrospinal fluid nitric oxide metabolites' levels. J. Neural. Transm. (Vienna) 129, 55–63 (2022).
Kouti, L. et al. Nitric oxide and peroxynitrite serum levels in Parkinson’s disease: correlation of oxidative stress and the severity of the disease. Eur. Rev. Med. Pharmacol. Sci. 17, 964–970 (2013).
Gatto, E. M. et al. Circulating plasma factors in Parkinson’s disease enhance nitric oxide release of normal human neutrophils. J. Neurol. Sci. 165, 66–70 (1999).
Shukla, R., Rajani, M., Srivastava, N., Barthwal, M. K. & Dikshit, M. Nitrite and malondialdehyde content in cerebrospinal fluid of patients with Parkinson’s disease. Int. J. Neurosci. 116, 1391–1402 (2006).
Tuncel, D., Inanc Tolun, F. & Toru, I. Serum insulin-like growth factor-1 and nitric oxide levels in Parkinson’s disease. Mediators Inflamm. 2009, 132464 (2009).
Eve, D. J. et al. Basal ganglia neuronal nitric oxide synthase mRNA expression in Parkinson’s disease. Mol. Brain Res. 63, 62–71 (1998).
Joniec, I. et al. Age- and sex-differences in the nitric oxide synthase expression and dopamine concentration in the murine model of Parkinson’s disease induced by 1-methyl-4-phenyl-1,2,3,6-tetrahydropyridine. Brain Res. 1261, 7–19 (2009).
Watanabe, Y., Kato, H. & Araki, T. Protective action of neuronal nitric oxide synthase inhibitor in the MPTP mouse model of Parkinson’s disease. Metab. Brain Dis. 23, 51–69 (2008).
Cavalcanti-Kwiatkoski, R., Raisman-Vozari, R., Ginestet, L. & Del Bel, E. Altered expression of neuronal nitric oxide synthase in weaver mutant mice. Brain Res. 1326, 40–50 (2010).
Komeima, K., Hayashi, Y., Naito, Y. & Watanabe, Y. Inhibition of nNOS by calcium/calmodulin-dependent protein kinase IIα through Ser847 phosphorylation in NG108-15 neuronal cells. J. Biol. Chem. 275, 28139–28143 (2000).
Parlak, H. et al. Neuronal nitric oxide synthase phosphorylation induced by docosahexaenoic acid protects dopaminergic neurons in an experimental model of Parkinson’s disease. Folia Histochem. Cytobiol. 56, 27–37 (2018).
Falsone, S. F., Kungl, A. J., Rek, A., Cappai, R. & Zangger, K. The molecular chaperone Hsp90 modulates intermediate steps of amyloid assembly of the Parkinson-related protein alpha-synuclein. J. Biol. Chem. 284, 31190–31199 (2009).
Peng, H. M. et al. Dynamic cycling with Hsp90 stabilizes neuronal nitric oxide synthase through calmodulin-dependent inhibition of ubiquitination. Biochemistry 48, 8483–8490 (2009).
Liu, J. et al. Rab11a and HSP90 regulate recycling of extracellular alpha-synuclein. J. Neurosci. 29, 1480–1485 (2009).
Putcha, P. et al. Brain-permeable small-molecule inhibitors of Hsp90 prevent alpha-synuclein oligomer formation and rescue alpha-synuclein-induced toxicity. J. Pharm. Exp. Ther. 332, 849–857 (2010).
Titze-de-Almeida, R. et al. Suppressing nNOS enzyme by small-interfering RNAs protects SH-SY5Y cells and nigral dopaminergic neurons from 6-OHDA injury. Neurotox. Res. 36, 117–131 (2019).
Lowenstein, C. J. & Padalko, E. iNOS (NOS2) at a glance. J. Cell Sci. 117, 2865–2867 (2004).
Hunot, S. et al. Nitric oxide synthase and neuronal vulnerability in Parkinson’s disease. Neuroscience 72, 355–363 (1996).
Broom, L. et al. Neuroprotection by the selective iNOS inhibitor GW274150 in a model of Parkinson disease. Free Radic. Biol. Med. 50, 633–640 (2011).
Zhu, J. et al. Apelin-36 mediates neuroprotective effects by regulating oxidative stress, autophagy and apoptosis in MPTP-induced Parkinson’s disease model mice. Brain Res. 1726, 146493 (2020).
Tapias, V. et al. Synthetic alpha-synuclein fibrils cause mitochondrial impairment and selective dopamine neurodegeneration in part via iNOS-mediated nitric oxide production. Cell Mol. Life Sci. 74, 2851–2874 (2017).
Dehmer, T., Lindenau, J., Haid, S., Dichgans, J. & Schulz, J. B. Deficiency of inducible nitric oxide synthase protects against MPTP toxicity in vivo. J. Neurochem. 74, 2213–2216 (2000).
Jansson, E. A. et al. A mammalian functional nitrate reductase that regulates nitrite and nitric oxide homeostasis. Nat. Chem. Biol. 4, 411–417 (2008).
Kozlov, A. V., Staniek, K. & Nohl, H. Nitrite reductase activity is a novel function of mammalian mitochondria. FEBS Lett. 454, 127–130 (1999).
Presley, T. D. et al. Acute effect of a high nitrate diet on brain perfusion in older adults. Nitric Oxide 24, 34–42 (2011).
Millar, J. The nitric oxide/ascorbate cycle: how neurones may control their own oxygen supply. Med. Hypotheses 45, 21–26 (1995).
Pereira, C., Ferreira, N. R., Rocha, B. S., Barbosa, R. M. & Laranjinha, J. The redox interplay between nitrite and nitric oxide: From the gut to the brain. Redox Biol. 1, 276–284 (2013).
Nohl, H. et al. Mitochondria recycle nitrite back to the bioregulator nitric monoxide. Acta Biochim. Pol. 47, 913–921 (2000).
Perez-Pardo, P. et al. The gut-brain axis in Parkinson’s disease: possibilities for food-based therapies. Eur. J. Pharm. 817, 86–95 (2017).
Dodiya, H. B. et al. Chronic stress-induced gut dysfunction exacerbates Parkinson’s disease phenotype and pathology in a rotenone-induced mouse model of Parkinson’s disease. Neurobiol. Dis. 135, 104352 (2020).
Kim, J. S. et al. alpha-Synuclein in the colon and premotor markers of Parkinson disease in neurologically normal subjects. Neurol. Sci. 38, 171–179 (2017).
Uemura, N. et al. Inoculation of alpha-synuclein preformed fibrils into the mouse gastrointestinal tract induces Lewy body-like aggregates in the brainstem via the vagus nerve. Mol. Neurodegener. 13, 21 (2018).
Kim, S. et al. Transneuronal propagation of pathologic alpha-synuclein from the gut to the brain models Parkinson’s disease. Neuron 103, 627–641 e627 (2019).
Sampson, T. R. et al. Gut microbiota regulate motor deficits and neuroinflammation in a model of Parkinson’s disease. Cell 167, 1469–1480.e1412 (2016).
Blandini, F. et al. Functional and neurochemical changes of the gastrointestinal tract in a rodent model of Parkinson’s disease. Neurosci. Lett. 467, 203–207 (2009).
Wang, L. et al. Mice overexpressing wild-type human alpha-synuclein display alterations in colonic myenteric ganglia and defecation. Neurogastroenterol. Motil. 24, e425–e436 (2012).
Sun, M. F. et al. Neuroprotective effects of fecal microbiota transplantation on MPTP-induced Parkinson’s disease mice: Gut microbiota, glial reaction and TLR4/TNF-alpha signaling pathway. Brain Behav. Immun. 70, 48–60 (2018).
Moreno-Lopez, B. & Gonzalez-Forero, D. Nitric oxide and synaptic dynamics in the adult brain: physiopathological aspects. Rev. Neurosci. 17, 309–357 (2006).
Bradley, S. A. & Steinert, J. R. Nitric oxide-mediated posttranslational modifications: impacts at the synapse. Oxid. Med. Cell Longev. 2016, 5681036 (2016).
Nakamura, T. et al. Noncanonical transnitrosylation network contributes to synapse loss in Alzheimer’s disease. Science 371, https://doi.org/10.1126/science.aaw0843 (2021).
Amal, H. et al. Shank3 mutation in a mouse model of autism leads to changes in the S-nitroso-proteome and affects key proteins involved in vesicle release and synaptic function. Mol. Psychiatry 25, 1835–1848 (2020).
Choi, Y. B. et al. Molecular basis of NMDA receptor-coupled ion channel modulation by S-nitrosylation. Nat. Neurosci. 3, 15–21 (2000).
Selvakumar, B., Huganir, R. L. & Snyder, S. H. S-nitrosylation of stargazin regulates surface expression of AMPA-glutamate neurotransmitter receptors. Proc. Natl Acad. Sci. U.S.A. 106, 16440–16445 (2009).
Umanah, G. K. E. et al. AMPA receptor surface expression is regulated by S-nitrosylation of thorase and transnitrosylation of NSF. Cell Rep. 33, 108329 (2020).
Petzold, G. C. et al. Nitric oxide modulates calcium entry through P/Q-type calcium channels and N-methyl-d-aspartate receptors in rat cortical neurons. Brain Res. 1063, 9–14 (2005).
Tegenge, M. A., Stern, M. & Bicker, G. Nitric oxide and cyclic nucleotide signal transduction modulates synaptic vesicle turnover in human model neurons. J. Neurochem. 111, 1434–1446 (2009).
Lu, Y. F., Kandel, E. R. & Hawkins, R. D. Nitric oxide signaling contributes to late-phase LTP and CREB phosphorylation in the hippocampus. J. Neurosci. 19, 10250–10261 (1999).
Arancio, O. et al. Nitric oxide acts directly in the presynaptic neuron to produce long-term potentiation in cultured hippocampal neurons. Cell 87, 1025–1035 (1996).
Kobayashi, Y. et al. Bisphenol A and rotenone induce S-nitrosylation of protein disulfide isomerase (PDI) and inhibit neurite outgrowth of primary cultured cells of the rat hippocampus and PC12 cells. J. Toxicol. Sci. 45, 783–794 (2020).
Stroissnigg, H. et al. S-nitrosylation of microtubule-associated protein 1B mediates nitric-oxide-induced axon retraction. Nat. Cell Biol. 9, 1035–1045 (2007).
Dawson, V. L., Dawson, T. M., London, E. D., Bredt, D. S. & Snyder, S. H. Nitric oxide mediated glutatmate neurotoxicity in primary cortical cultures. Proc. Natl Acad. Sci. U.S.A. 88, 6368–6371 (1991).
Shi, Z. Q. et al. S-nitrosylated SHP-2 contributes to NMDA receptor-mediated excitotoxicity in acute ischemic stroke. Proc. Natl Acad. Sci. U.S.A. 110, 3137–3142 (2013).
Ba, M., Ding, W., Guan, L., Lv, Y. & Kong, M. S-nitrosylation of Src by NR2B-nNOS signal causes Src activation and NR2B tyrosine phosphorylation in levodopa-induced dyskinetic rat model. Hum. Exp. Toxicol. 38, 303–310 (2019).
Giesen, J. et al. AMPA Induces NO-dependent cGMP signals in hippocampal and cortical neurons via L-type voltage-gated calcium channels. Cereb. Cortex 30, 2128–2143 (2020).
Ryan, S. D. et al. Isogenic human iPSC Parkinson’s model shows nitrosative stress-induced dysfunction in MEF2-PGC1alpha transcription. Cell 155, 1351–1364 (2013).
Chung, C. Y. et al. Identification and rescue of α-synuclein toxicity in parkinson patient-derived neurons. Science 342, 983–987 (2013).
Stykel, M. G. et al. Nitration of microtubules blocks axonal mitochondrial transport in a human pluripotent stem cell model of Parkinson’s disease. FASEB J. 32, 5350–5364 (2018).
Redondo, J., Hares, K., Wilkins, A., Scolding, N. & Kemp, K. Reductions in kinesin expression are associated with nitric oxide-induced axonal damage. J. Neurosci. Res. 93, 882–892 (2015).
Wang, Y. et al. Protein cysteine S-nitrosylation inhibits vesicular uptake of neurotransmitters. Neuroscience 311, 374–381 (2015).
Brown, G. C. & Cooper, C. E. Nanomolar concentrations of nitric oxide reversibly inhibit synaptosomal respiration by competing with oxygen at cytochrome oxidase. FEBS Lett. 356, 295–298 (1994).
Cassina, A. & Radi, R. Differential inhibitory action of nitric oxide and peroxynitrite on mitochondrial electron transport. Arch. Biochem. Biophys. 328, 309–316 (1996).
Brown, G. C. Regulation of mitochondrial respiration by nitric oxide inhibition of cytochrome c oxidase. Biochem. Biophys. Acta 1504, 46–57 (2001).
Chang, A. H. et al. Respiratory substrates regulate S-nitrosylation of mitochondrial proteins through a thiol-dependent pathway. Chem. Res. Toxicol. 27, 794–804 (2014).
Tonazzi, A., Giangregorio, N., Console, L., De Palma, A. & Indiveri, C. Nitric oxide inhibits the mitochondrial carnitine/acylcarnitine carrier through reversible S-nitrosylation of cysteine 136. Biochim. Biophys. Acta Bioenerg. 1858, 475–482 (2017).
Faienza, F., Rizza, S., Giglio, P. & Filomeni, G. TRAP1: a metabolic hub linking aging pathophysiology to mitochondrial S-nitrosylation. Front. Physiol. 11, 340 (2020).
Halestrap, A. P. What is the mitochondrial permeability transition pore. J. Mol. Cell Cardiol. 46, 821–831 (2009).
Cheng, Q., Sedlic, F., Pravdic, D., Bosnjak, Z. J. & Kwok, W. M. Biphasic effect of nitric oxide on the cardiac voltage-dependent anion channel. FEBS Lett. 585, 328–334 (2011).
Aquilano, K., Baldelli, S. & Ciriolo, M. R. Nuclear recruitment of neuronal nitric-oxide synthase by alpha-syntrophin is crucial for the induction of mitochondrial biogenesis. J. Biol. Chem. 289, 365–378 (2014).
Shibuya, A. et al. Nitration of PPARy inhibits ligand-dependent translocation into the nucleus in a macrophage-like cell line, RAW 264. FEBS Lett. 525, 43–47 (2002).
Nakamura, T. & Lipton, S. A. S-nitrosylation of critical protein thiols mediates protein misfolding and mitochondrial dysfunction in neurodegenerative disease. Antioxid. Redox Signal. 14, 1479–1492 (2011).
Ge, P., Dawson, V. L. & Dawson, T. M. PINK1 and Parkin mitochondrial quality control: a source of regional vulnerability in Parkinson’s disease. Mol. Neurodegener. 15, 20 (2020).
Yao, D. et al. Nitrosative stress linked to sporadic Parkinson’s disease: S-nitrosylation of parkin regulates its E3 ubiquitin ligase activity. Proc. Natl Acad. Sci. U.S.A. 101, 10810–10814 (2004).
Chung, K. K. et al. S-Nitrosylation of Parkin regulates ubiquitination and compromises Parkin’s protective function. Science 304, 1328–1331 (2004).
Ozawa, K. et al. DJ-1 is indispensable for the S-nitrosylation of Parkin, which maintains function of mitochondria. Sci. Rep. 10, 4377 (2020).
Oh, C. K. et al. S-Nitrosylation of PINK1 attenuates PINK1/Parkin-dependent mitophagy in hiPSC-based Parkinson’s disease models. Cell Rep. 21, 2171–2182 (2017).
Qu, Y. et al. Prohibitin S-nitrosylation is required for the neuroprotective effect of nitric oxide in neuronal cultures. J. Neurosci. 40, 3142–3151 (2020).
Dutta, D. et al. Low levels of prohibitin in substantia nigra makes dopaminergic neurons vulnerable in Parkinson’s disease. Mol. Neurobiol. 55, 804–821 (2018).
Fang, J., Nakamura, T., Cho, D. H., Gu, Z. & Lipton, S. A. S-nitrosylation of peroxiredoxin 2 promotes oxidative stress-induced neuronal cell death in Parkinson’s disease. Proc. Natl Acad. Sci. U.S.A. 104, 18742–18747 (2007).
Kuhn, D. M., Aretha, C. W. & Geddes, T. J. Peroxynitrite inactivation of tyrosine hydroxylase: mediation by sulfhydryl oxidation, not tyrosine nitration. J. Neurosci. 19, 10289–10294 (1999).
Pong, K., doctrow, S. R. & Baudry, M. Prevention of 1-methyl-4-phenylpyridinium- and 6-hydroxydopamine-induced nitration of tyrosine hydroxylase and neurotoxicity by EUK-134, a superoxide dismutase and catalase mimetic, in cultured dopaminergic neurons. Brain Res. 881, 182–189 (2000).
Nappi, A. J. & Vass, E. The effects of nitric oxide on the oxidations of l-dopa and dopamine mediated by tyrosinase and peroxidase. J. Biol. Chem. 276, 11214–11222 (2001).
Antunes, F., Nunes, C., Laranjinha, J. & Cadenas, E. Redox interactions of nitric oxide with dopamine and its derivatives. Toxicology 208, 207–212 (2005).
Nunes, C., Almeida, L. & Laranjinha, J. Synergistic inhibition of respiration in brain mitochondria by nitric oxide and dihydroxyphenylacetic acid (DOPAC). Implications for Parkinson’s disease. Neurochem. Int. 47, 173–182 (2005).
Nunes, C., Barbosa, R. M., Almeida, L. & Laranjinha, J. Nitric oxide and DOPAC-induced cell death: from GSH depletion to mitochondrial energy crisis. Mol. Cell Neurosci. 48, 94–103 (2011).
Hsu, M., Srinivas, B., Kumar, J., Subramanian, R. & Andersen, J. Glutathione depletion resulting in selective mitochondrial complex I inhibition in dopaminergic cells is via an NO-mediated pathway not involving peroxynitrite: implications for Parkinson’s disease. J. Neurochem. 92, 1091–1103 (2005).
Chinta, S. J. & Andersen, J. K. Reversible inhibition of mitochondrial complex I activity following chronic dopaminergic glutathione depletion in vitro: implications for Parkinson’s disease. Free Radic. Biol. Med. 41, 1442–1448 (2006).
Watanabe-Nakayama, T. et al. Self- and cross-seeding on alpha-Synuclein Fibril growth kinetics and structure observed by high-speed atomic force microscopy. ACS Nano 14, 9979–9989 (2020).
Leitao, A. D. G. et al. Selectivity of Lewy body protein interactions along the aggregation pathway of alpha-synuclein. Commun. Biol. 4, 1124 (2021).
Danzer, K. M., Krebs, S. K., Wolff, M., Birk, G. & Hengerer, B. Seeding induced by alpha-synuclein oligomers provides evidence for spreading of alpha-synuclein pathology. J. Neurochem. 111, 192–203 (2009).
Hansen, C. et al. a-Synuclein propagates from mouse brain to grafted dopaminergic neurons and seeds aggregation in cultured human cells. J. Clin. Investig. 121, 715–725 (2011).
Lee, H. J. et al. Assembly-dependent endocytosis and clearance of extracellular alpha-synuclein. Int. J. Biochem. Cell Biol. 40, 1835–1849 (2008).
Grudina, C. et al. Human NPCs can degrade alpha-syn fibrils and transfer them preferentially in a cell contact-dependent manner possibly through TNT-like structures. Neurobiol. Dis. 132, 104609 (2019).
Mao, X. et al. Pathological alpha-synuclein transmission initiated by binding lymphocyte-activation gene 3. Science 353, https://doi.org/10.1126/science.aah3374 (2016).
Andreasen, M., Lorenzen, N. & Otzen, D. Interactions between misfolded protein oligomers and membranes: a central topic in neurodegenerative diseases. Biochim. Biophys. Acta 1848, 1897–1907 (2015).
Ganjam, G. K. et al. Mitochondrial damage by alpha-synuclein causes cell death in human dopaminergic neurons. Cell Death Dis. 10, 865 (2019).
Cuervo, A. M., Stefanis, L., Fredenburg, R., Lansbury, P. T. & Sulzer, D. Impaired degradation of mutant a-synuclein by chaperone-mediated autophagy. Science 305, 1292–1295 (2004).
Winslow, A. R. et al. alpha-Synuclein impairs macroautophagy: implications for Parkinson’s disease. J. Cell Biol. 190, 1023–1037 (2010).
McKinnon, C. et al. Early-onset impairment of the ubiquitin-proteasome system in dopaminergic neurons caused by alpha-synuclein. Acta Neuropathol. Commun. 8, 17 (2020).
Choi, B. K. et al. Large alpha-synuclein oligomers inhibit neuronal SNARE-mediated vesicle docking. Proc. Natl Acad. Sci. U.S.A. 110, 4087–4092 (2013).
Braak, H. et al. Staging of brain pathology related to sporadic Parkinson’s disease. Neurobiol. Aging 24, 197–211 (2003).
Burai, R., Ait-Bouziad, N., Chiki, A. & Lashuel, H. A. Elucidating the role of site-specific nitration of alpha-synuclein in the pathogenesis of Parkinson’s disease via protein semisynthesis and mutagenesis. J. Am. Chem. Soc. 137, 5041–5052 (2015).
Hodara, R. et al. Functional consequences of alpha-synuclein tyrosine nitration: diminished binding to lipid vesicles and increased fibril formation. J. Biol. Chem. 279, 47746–47753 (2004).
Krishnan, S. et al. Oxidative dimer formation is the critical rate-limiting step for parkinson’s disease a-synuclein fibrillogenesis. Biochemistry 42, 829–837 (2003).
Danielson, S. R. et al. Preferentially increased nitration of alpha-synuclein at tyrosine-39 in a cellular oxidative model of Parkinson’s disease. Anal. Chem. 81, 7823–7828 (2009).
Sevcsik, E., Trexler, A. J., Dunn, J. M. & Rhoades, E. Allostery in a disordered protein: oxidative modifications to alpha-synuclein act distally to regulate membrane binding. J. Am. Chem. Soc. 133, 7152–7158 (2011).
Musgrove, R. E. et al. Oxidative stress in vagal neurons promotes parkinsonian pathology and intercellular alpha-synuclein transfer. J. Clin. Investig. 129, 3738–3753 (2019).
Paxinou, E. et al. Induction of alpha-synuclein aggregation by intracellular nitrative insult. J. Neurosci. 21, 8053–8061 (2001).
Uversky, V. N. et al. Effects of nitration on the structure and aggregation of alpha-synuclein. Brain Res. Mol. Brain Res. 134, 84–102 (2005).
Norris, E. H., Giasson, B. I., Ischiropoulos, H. & Lee, V. M. Effects of oxidative and nitrative challenges on alpha-synuclein fibrillogenesis involve distinct mechanisms of protein modifications. J. Biol. Chem. 278, 27230–27240 (2003).
Yamin, G., Uversky, V. N. & Fink, A. L. Nitration inhibits fibrillation of human α-synuclein in vitro by formation of soluble oligomers. FEBS Lett. 542, 147–152 (2003).
Vicente Miranda, H. et al. Posttranslational modifications of blood-derived alpha-synuclein as biochemical markers for Parkinson’s disease. Sci. Rep. 7, 13713 (2017).
Giasson, B. I. et al. Oxidative damage linked to neurodegeneration by selective a-synuclein nitration in synucleinopathy lesions. Science 290, 985–989 (2000).
Przedborski, S. et al. Oxidative post-translational modi®cations of a-synuclein in the 1-methyl-4-phenyl-1,2,3,6tetrahydropyridine (MPTP) mouse model of Parkinson’s disease. J. Neurochem. 76, 637–640 (2001).
Mishizen-Eberz, A. J. et al. Cleavage of a-Synuclein by calpain: potential role in degradation of fibrillized and nitrated species of a-Synuclein. Biochemistry 44, 7818–7829 (2005).
Yu, Z. et al. Nitrated alpha-synuclein induces the loss of dopaminergic neurons in the substantia nigra of rats. PLoS One 5, e9956 (2010).
Sunico, C. R. et al. Role of sulfiredoxin as a peroxiredoxin-2 denitrosylase in human iPSC-derived dopaminergic neurons. Proc. Natl Acad. Sci. U.S.A. 113, E7564–E7571 (2016).
Choi, M. S. et al. Transnitrosylation from DJ-1 to PTEN attenuates neuronal cell death in parkinson’s disease models. J. Neurosci. 34, 15123–15131 (2014).
Gao, H. M. et al. Neuroinflammation and oxidation/nitration of alpha-synuclein linked to dopaminergic neurodegeneration. J. Neurosci. 28, 7687–7698 (2008).
Tokarew, J. M. et al. Age-associated insolubility of parkin in human midbrain is linked to redox balance and sequestration of reactive dopamine metabolites. Acta Neuropathol. 141, 725–754 (2021).
Imai, Y., Soda, M. & Takahashi, R. Parkin suppresses unfolded protein stress-induced cell death through its E3 ubiquitin-protein ligase activity. J. Biol. Chem. 275, 35661–35664 (2000).
Shahmoradian, S. H. et al. Lewy pathology in Parkinson’s disease consists of crowded organelles and lipid membranes. Nat. Neurosci. 22, 1099–1109 (2019).
Gomes, M. Z., Raisman-Vozari, R. & Del Bel, E. A. A nitric oxide synthase inhibitor decreases 6-hydroxydopamine effects on tyrosine hydroxylase and neuronal nitric oxide synthase in the rat nigrostriatal pathway. Brain Res. 1203, 160–169 (2008).
Yuste, J. E. et al. 7-Nitroindazole down-regulates dopamine/DARPP-32 signaling in neostriatal neurons in a rat model of Parkinson’s disease. Neuropharmacology 63, 1258–1267 (2012).
Czaniecki, C. et al. Axonal pathology in hPSC-based models of Parkinson’s disease results from loss of Nrf2 transcriptional activity at the Map1b gene locus. Proc. Natl Acad. Sci. U.S.A. 116, 14280–14289 (2019).
Hoang, T. et al. Neuronal NOS and cyclooxygenase-2 contribute to DNA damage in a mouse model of Parkinson disease. Free Radic. Biol. Med. 47, 1049–1056 (2009).
Schildknecht, S. et al. The NOX1/4 inhibitor GKT136901 as selective and direct scavenger of peroxynitrite. Curr. Med. Chem. 21, 365–376 (2014).
Tomas-Camardiel, M. et al. Minocycline reduces the lipopolysaccharide-induced inflammatory reaction, peroxynitrite-mediated nitration of proteins, disruption of the blood-brain barrier, and damage in the nigral dopaminergic system. Neurobiol. Dis. 16, 190–201 (2004).
He, Y., Appel, S. & Le, W. Minocycline inhibits microglial activation and protects nigral cells after 6-hydroxydopamine injection into mouse striatum. Brain Res. 909, 187–193 (2001).
Du, Y. et al. Minocycline prevents nigrostriatal dopaminergic neurodegeneration in the MPTP model of Parkinson’s disease. Proc. Natl Acad. Sci. U.S.A. 98, 14669–14674 (2001).
Barua, S., Kim, J. Y., Yenari, M. A. & Lee, J. E. The role of NOX inhibitors in neurodegenerative diseases. IBRO Rep. 7, 59–69 (2019).
Carroll, C. B. & Wyse, R. K. H. Simvastatin as a potential disease-modifying therapy for patients with Parkinson’s disease: rationale for clinical trial. Curr. Prog. J. Parkinson's Dis. 7, 545–568 (2017).
Scuderi, S. A., Ardizzone, A., Paterniti, I., Esposito, E. & Campolo, M. Antioxidant and anti-inflammatory effect of Nrf2 inducer dimethyl fumarate in neurodegenerative diseases. Antioxidants 9, https://doi.org/10.3390/antiox9070630 (2020).
Tong, H. et al. Simvastatin inhibits activation of NADPH Oxidase/p38 MAPK pathway and enhances expression of antioxidant protein in Parkinson disease models. Front. Mol. Neurosci. 11, 165 (2018).
Ahuja, M. et al. Distinct Nrf2 signaling mechanisms of fumaric acid esters and their role in neuroprotection against 1-methyl-4-phenyl-1,2,3,6-tetrahydropyridine-induced experimental Parkinson’s-like disease. J. Neurosci. 36, 6332–6351 (2016).
Jing, X. et al. Dimethyl fumarate attenuates 6-OHDA-induced neurotoxicity in SH-SY5Y cells and in animal model of Parkinson’s disease by enhancing Nrf2 activity. Neuroscience 286, 131–140 (2015).
Campolo, M. et al. The neuroprotective effect of dimethyl fumarate in an MPTP-mouse model of Parkinson’s disease: involvement of reactive oxygen species/nuclear factor-kappaB/nuclear transcription factor related to NF-E2. Antioxid. Redox Signal. 27, 453–471 (2017).
Lastres-Becker, I. et al. Repurposing the NRF2 activator dimethyl fumarate as therapy against synucleinopathy in Parkinson’s disease. Antioxid. Redox Signal 25, 61–77 (2016).
Vallee, A., Vallee, J. N. & Lecarpentier, Y. Parkinson’s disease: potential actions of lithium by targeting the WNT/beta-catenin pathway, oxidative stress, inflammation and glutamatergic pathway. Cells 10, https://doi.org/10.3390/cells10020230 (2021).
Lee, Y. S., Feng, C. W., Peng, M. Y., Chan, T. F. & Chen, Y. C. Neuroprotective effects of estradiol plus lithium chloride via anti-apoptosis and neurogenesis pathway in in vitro and in vivo. Parkinson’s Dis. Models Parkinson's Dis. 2021, 3064892 (2021).
Zhao, Q. et al. Neuroprotective effects of lithium on a chronic MPTP mouse model of Parkinson’s disease via regulation of alphasynuclein methylation. Mol. Med. Rep. 19, 4989–4997 (2019).
Liu, L., Wang, J. & Wang, H. Hydrogen sulfide alleviates oxidative stress injury and reduces apoptosis induced by MPP(+) in Parkinson’s disease cell model. Mol. Cell Biochem. 472, 231–240 (2020).
Zhang, Z. et al. Hydrogen-saturated saline mediated neuroprotection through autophagy via PI3K/AKT/mTOR pathway in early and medium stages of rotenone-induced Parkinson’s disease rats. Brain Res. Bull. 172, 1–13 (2021).
Molina-Holgado, F., Gaeta, A., Francis, P. T., Williams, R. J. & Hider, R. C. Neuroprotective actions of deferiprone in cultured cortical neurones and SHSY-5Y cells. J. Neurochem. 105, 2466–2476 (2008).
Carboni, E. et al. Deferiprone rescues behavioral deficits induced by mild iron exposure in a mouse model of alpha-synuclein aggregation. Neuromol. Med. 19, 309–321 (2017).
Hou, X. et al. GYY4137, an H2S slow-releasing donor, prevents nitrative stress and alpha-synuclein nitration in an MPTP mouse model of Parkinson’s disease. Front. Pharm. 8, 741 (2017).
Yuan, Y. Q. et al. Impaired CBS-H2S signaling axis contributes to MPTP-induced neurodegeneration in a mouse model of Parkinson’s disease. Brain Behav. Immun. 67, 77–90 (2018).
Martin-Bastida, A. et al. Brain iron chelation by deferiprone in a phase 2 randomised double-blinded placebo controlled clinical trial in Parkinson’s disease. Sci. Rep. 7, 1398 (2017).
Yoritaka, A., Kobayashi, Y., Hayashi, T., Saiki, S. & Hattori, N. Randomized double-blind placebo-controlled trial of hydrogen inhalation for Parkinson’s disease: a pilot study. Neurol. Sci. 42, 4767–4770 (2021).
Yoritaka, A. et al. Randomized, double-blind, multicenter trial of hydrogen water for Parkinson’s disease. Mov. Disord. 33, 1505–1507 (2018).
Ghosh, S. et al. alpha-synuclein aggregates induce c-Abl activation and dopaminergic neuronal loss by a feed-forward redox stress mechanism. Prog. Neurobiol. 202, 102070 (2021).
Berman, A. E. et al. N-acetylcysteine prevents loss of dopaminergic neurons in the EAAC1-/- mouse. Ann. Neurol. 69, 509–520 (2011).
Munoz, A. M., Rey, P., Soto-Otero, R., Guerra, M. J. & Labandeira-Garcia, J. L. Systemic administration of N-acetylcysteine protects dopaminergic neurons against 6-hydroxydopamine-induced degeneration. J. Neurosci. Res. 76, 551–562 (2004).
Clark, J. et al. Oral N-acetyl-cysteine attenuates loss of dopaminergic terminals in alpha-synuclein overexpressing mice. PLoS One 5, e12333 (2010).
Monti, D. A. et al. N-acetyl cysteine may support dopamine neurons in Parkinson’s disease: preliminary clinical and cell line data. PLoS One 11, e0157602 (2016).
Monti, D. A. et al. N-acetyl cysteine is associated with dopaminergic improvement in Parkinson’s disease. Clin. Pharm. Ther. 106, 884–890 (2019).
Sircar, E., Rai, S. R., Wilson, M. A., Schlossmacher, M. G. & Sengupta, R. Neurodegeneration: impact of S-nitrosylated Parkin, DJ-1 and PINK1 on the pathogenesis of Parkinson’s disease. Arch. Biochem. Biophys. 704, 108869 (2021).
Hao, G., Derakhshan, B., Shi, L., Campagne, F. & Gross, S. S. SNOSID, a proteomic method for identification of cysteine S-nitrosylation sites in complex protein mixtures. Proc. Natl Acad. Sci. U.S.A. 103, 1012–1017 (2006).
Benhar, M., Thompson, J. W., Moseley, M. A. & Stamler, J. S. Identification of S-nitrosylated targets of thioredoxin using a quantitative proteomic approach. Biochemistry 49, 6963–6969 (2010).
Zareba-Koziol, M., Szwajda, A., Dadlez, M., Wyslouch-Cieszynska, A. & Lalowski, M. Global analysis of S-nitrosylation sites in the wild type (APP) transgenic mouse brain-clues for synaptic pathology. Mol. Cell Proteom. 13, 2288–2305 (2014).
Thom, S. R., Bhopale, V. M., Mancini, D. J. & Milovanova, T. N. Actin S-nitrosylation inhibits neutrophil beta2 integrin function. J. Biol. Chem. 283, 10822–10834 (2008).
Lefievre, L. et al. Human spermatozoa contain multiple targets for protein S-nitrosylation: an alternative mechanism of the modulation of sperm function by nitric oxide? Proteomics 7, 3066–3084 (2007).
Jaffrey, S. R., Erdjument-Bromage, H., Ferris, C. D., Tempst, P. & Snyder, S. H. Protein S-nitrosylation: a physiological signal for neuronal nitric oxide. Nat. Cell Biol. 3, 193–197 (2001).
Bizzozero, O. A. & Zheng, J. Identification of major S-nitrosylated proteins in murine experimental autoimmune encephalomyelitis. J. Neurosci. Res. 87, 2881–2889 (2009).
Zahid, S., Khan, R., Oellerich, M., Ahmed, N. & Asif, A. R. Differential S-nitrosylation of proteins in Alzheimer’s disease. Neuroscience 256, 126–136 (2014).
Swomley, A. M. & Butterfield, D. A. Oxidative stress in Alzheimer disease and mild cognitive impairment: evidence from human data provided by redox proteomics. Arch. Toxicol. 89, 1669–1680 (2015).
Mnatsakanyan, R. et al. Proteome-wide detection of S-nitrosylation targets and motifs using bioorthogonal cleavable-linker-based enrichment and switch technique. Nat. Commun. 10, 2195 (2019).
Kuncewicz, T., Sheta, E. A., Goldknopf, I. L. & Kone, B. C. Proteomic analysis of S-nitrosylated proteins in mesangial cells. Mol. Cell Proteom. 2, 156–163 (2003).
Sun, J., Morgan, M., Shen, R. F., Steenbergen, C. & Murphy, E. Preconditioning results in S-nitrosylation of proteins involved in regulation of mitochondrial energetics and calcium transport. Circ. Res. 101, 1155–1163 (2007).
Landino, L. M., Koumas, M. T., Mason, C. E. & Alston, J. A. Modification of tubulin cysteines by nitric oxide and nitroxyl donors alters tubulin polymerization activity. Chem. Res. Toxicol. 20, 1693–1700 (2007).
Kamnev, A., Muhar, M., Preinreich, M., Ammer, H. & Propst, F. Difficulties in generating specific antibodies for immunohistochemical detection of nitrosylated tubulins. PLoS One 8, e68168 (2013).
Wang, G., Moniri, N. H., Ozawa, K., Stamler, J. S. & Daaka, Y. Nitric oxide regulates endocytosis by S-nitrosylation of dynamin. Proc. Natl Acad. Sci. U.S.A. 103, 1295–1300 (2006).
Seneviratne, U. et al. S-nitrosation of proteins relevant to Alzheimer’s disease during early stages of neurodegeneration. Proc. Natl Acad. Sci. U.S.A. 113, 4152–4157 (2016).
Molina y Vedia, L. et al. Nitric oxide-induced S-nitrosylation of glyceraldehyde-3-phosphate dehydrogenase inhibits enzymatic activity and increases endogenous ADP-ribosylation. J. Biol. Chem. 267, 24929–24932 (1992).
Hara, M. R. et al. S-nitrosylated GAPDH initiates apoptotic cell death by nuclear translocation following Siah1 binding. Nat. Cell Biol. 7, 665–674 (2005).
Qiu, C. et al. First nitrosoproteomic profiling deciphers the cysteine S-nitrosylation involved in multiple metabolic pathways of tea leaves. Sci. Rep. 9, 17525 (2019).
Martinez-Ruiz, A. et al. S-nitrosylation of Hsp90 promotes the inhibition of its ATPase and endothelial nitric oxide synthase regulatory activities. Proc. Natl Acad. Sci. U.S.A. 102, 8525–8530 (2005).
Chouchani, E. T. et al. Identification of S-nitrosated mitochondrial proteins by S-nitrosothiol difference in gel electrophoresis (SNO-DIGE): implications for the regulation of mitochondrial function by reversible S-nitrosation. Biochem. J. 430, 49–59 (2010).
Yonashiro, R. et al. Mitochondrial ubiquitin ligase MITOL blocks S-nitrosylated MAP1B-light chain 1-mediated mitochondrial dysfunction and neuronal cell death. Proc. Natl Acad. Sci. U.S.A. 109, 2382–2387 (2012).
Bellucci, A. et al. Abnormal processing of tau in the brain of aged TgCRND8 mice. Neurobiol. Dis. 27, 328–338 (2007).
Spurny, R. et al. Oxidation and nitrosylation of cysteines proximal to the intermediate filament (IF)-binding site of plectin: effects on structure and vimentin binding and involvement in IF collapse. J. Biol. Chem. 282, 8175–8187 (2007).
Grau, M. et al. RBC-NOS-dependent S-nitrosylation of cytoskeletal proteins improves RBC deformability. PLoS One 8, e56759 (2013).
Wang, Z., Kim, J. I., Frilot, N. & Daaka, Y. Dynamin2 S-nitrosylation regulates adenovirus type 5 infection of epithelial cells. J. Gen. Virol. 93, 2109–2117 (2012).
Forrester, M. T. et al. Proteomic analysis of S-nitrosylation and denitrosylation by resin-assisted capture. Nat. Biotechnol. 27, 557–559 (2009).
Amal, H. et al. S-nitrosylation of E3 ubiquitin-protein ligase RNF213 alters non-canonical Wnt/Ca+2 signaling in the P301S mouse model of tauopathy. Transl. Psychiatry 9, 44 (2019).
Huang, B., Liao, C. L., Lin, Y. P., Chen, S. C. & Wang, D. L. S-nitrosoproteome in endothelial cells revealed by a modified biotin switch approach coupled with Western blot-based two-dimensional gel electrophoresis. J. Proteome Res. 8, 4835–4843 (2009).
Huang, B., Chen, S. C. & Wang, D. L. Shear flow increases S-nitrosylation of proteins in endothelial cells. Cardiovasc. Res. 83, 536–546 (2009).
Chen, S. C. et al. Acute hypoxia enhances proteins’ S-nitrosylation in endothelial cells. Biochem. Biophys. Res. Commun. 377, 1274–1278 (2008).
Acknowledgements
This work was supported in part by the Canadian Institutes of Health, Research (2014-685 to S.D.R.), the Natural Sciences and Engineering Research Council of Canada, (RG060805 and CRDPJ: 490841-15 to S.D.R.), and the Vanier Program (to M.G.S.). Figures were assembled using Biorender.
Author information
Authors and Affiliations
Contributions
This review was written and edited by both M.G.S. and S.D.R. Figures and tables were assembled and edited by both M.G.S. and S.D.R.
Corresponding author
Ethics declarations
Competing interests
The authors declare no competing interests.
Additional information
Publisher’s note Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.
Rights and permissions
Open Access This article is licensed under a Creative Commons Attribution 4.0 International License, which permits use, sharing, adaptation, distribution and reproduction in any medium or format, as long as you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made. The images or other third party material in this article are included in the article’s Creative Commons license, unless indicated otherwise in a credit line to the material. If material is not included in the article’s Creative Commons license and your intended use is not permitted by statutory regulation or exceeds the permitted use, you will need to obtain permission directly from the copyright holder. To view a copy of this license, visit http://creativecommons.org/licenses/by/4.0/.
About this article
Cite this article
Stykel, M.G., Ryan, S.D. Nitrosative stress in Parkinson’s disease. npj Parkinsons Dis. 8, 104 (2022). https://doi.org/10.1038/s41531-022-00370-3
Received:
Accepted:
Published:
DOI: https://doi.org/10.1038/s41531-022-00370-3
This article is cited by
-
Microtubule acetylation dyshomeostasis in Parkinson’s disease
Translational Neurodegeneration (2023)
