Skip to main content
International Journal of Cell Biology logoLink to International Journal of Cell Biology
. 2012 May 17;2012:908724. doi: 10.1155/2012/908724

Altered Gene Expression, Mitochondrial Damage and Oxidative Stress: Converging Routes in Motor Neuron Degeneration

Luisa Rossi 1, Cristiana Valle 2,3, Maria Teresa Carrì 1,3,*
PMCID: PMC3362844  PMID: 22675362

Abstract

Motor neuron diseases (MNDs) are a rather heterogeneous group of diseases, with either sporadic or genetic origin or both, all characterized by the progressive degeneration of motor neurons. At the cellular level, MNDs share features such as protein misfolding and aggregation, mitochondrial damage and energy deficit, and excitotoxicity and calcium mishandling. This is particularly well demonstrated in ALS, where both sporadic and familial forms share the same symptoms and pathological phenotype, with a prominent role for mitochondrial damage and resulting oxidative stress. Based on recent data, however, altered control of gene expression seems to be a most relevant, and previously overlooked, player in MNDs. Here we discuss which may be the links that make pathways apparently as different as altered gene expression, mitochondrial damage, and oxidative stress converge to generate a similar motoneuron-toxic phenotype.

1. Introduction

Motor neuron diseases (MNDs) are a rather heterogeneous group of diseases, with either sporadic or genetic origin or both, all characterized by the progressive degeneration of motor neurons. All MNDs are primarily axonopathies of the motor neurons in which neuromuscular synapses are early targets of damage and death of motor neurons probably occurs following loss of the neuromuscular junctions [1]. MNDs may manifest as weakness, atrophy of muscles, difficulty in breathing, speaking, and swallowing, with symptoms and severity varying as a consequence of the different involvement of upper or lower motor neurons or both.

The most common and studied form in adults is Amyotrophic Lateral Sclerosis (ALS), followed by Progressive Bulbar Palsy (PBP), the rarer forms being Progressive Muscular Atrophy (PMA) and Primary Lateral Sclerosis (PLS). These conditions seem to form a continuum of diseases since only part of patients have a “pure” phenotype, while others with PBP or PLS eventually develop the widespread symptoms common to ALS [2]. In all these MNDs, onset of symptoms occurs mainly in people aged 40–70. Life expectancy is between 2 to about 5 years after onset in ALS and 6 months to 3 years in PBP, while pure PLS patients may have a normal or near-to-normal life duration. MNDs also include Spinal and Bulbar Muscular Atrophy (SBMA), in which age of onset and severity of manifestations vary from adolescence to old age, but longevity is usually not compromised. Infantile MNDs include Spinal Muscular Atrophy (SMA) with an infantile or juvenile onset and Lethal Congenital Contracture Syndrome (LCCS), causing prenatal death and thus being the most severe form of motor neuron disease.

2. Aetiology of MNDs

LCCS1 is an autosomal recessive condition found in communities of the northeastern part of Finland with a prevalence of 1 in 25,250 births [3]. LCCS manifests in utero with a marked atrophy of spinal cord motor neurons and fetal immobility due to lack of anterior horn motor neurons, severe atrophy of the ventral spinal cord, and hypoplastic skeletal muscles. It is characterized by total immobility of the fetus, detectable at the 13th week of pregnancy and invariably leading to prenatal death before the 32nd gestational week. The defective gene for LCCS1 is a 16-exon gene coding for GLE1, an mRNA export mediator that is known to interact with the nuclear pore complex and is expressed in the neural tube of 11-day-old mice embryos, specifically in the ventral cell population from which the motor neurons differentiate, and later in other tissues including somites, from which skeletal muscle and bone tissue differentiate [3]. The most frequent mutation in LCCS1 (FinMajor) does not dramatically alter the stability or localization of the protein GLE1 but is predicted to introduce three aminoacid residues in a region that may be critical in the interaction between GLE1 and a motor neuron-specific protein [3].

SMA is the most frequent genetic cause of infant mortality and exists in various forms invariably caused by a genetic defect. Patients with the most common form (proximal SMA) are either deleted for the nine-exon gene SMN1, encoding the ubiquitously expressed protein SMN (Survival Motor Neuron) or carry small mutations in the same gene. However, SMA patients always carry at least one copy of the gene SMN2, which encodes the same protein as SMN1 and is only partially functional because of a critical, translationally silent single nucleotide C/T transition inside exon 7 that profoundly affects correct splicing. The clinical severity of SMA ranges from respiratory distress at birth associated with limited life expectancy (SMA1) to onset at older than 10 years and a normal life expectancy (SMA4) and is inversely related to the level of SMN2 compensating for SMN1 deletion [4].

SBMA (also called Kennedy's disease) is an X-linked recessive motor neuron disease in which only lower spinal cord and brain stem motor neurons are affected [5]. SBMA is caused by a polyglutamine expansion in the androgen receptor (AR) [6]; CAG repeat numbers range from 38 to 62 in SBMA patients, whereas healthy individuals have 10 to 36 CAG repeats. Symptoms appear in childhood or early adolescence [7]; SBMA is a rare disease, with the exception of some population in the Vasa region of Western Finland where it was estimated that the prevalence is 13 in 85,000 male inhabitants [8].

While SMA, SBMA, and LCCS1 are invariably familial diseases, adult-onset MNDs are both sporadic and familial. PBP, PMA, and PLS are usually sporadic. ALS occurs sporadically in the majority of cases [9]. Proposed risk factors for ALS include ingestion of high concentrations of β-methyl-amino-L-alanine [10], use of cholesterol-lowering drugs [11], intensive physical exercise [12] including football playing [13, 14] and service in the USA Army [15], possibly linked to intermittent occupational hypoxia [16] or to head injury [1719]. Environmental factors also include cigarette smoking [18, 20], exposure to heavy metals [21], and pesticides or herbicides [2224]. Approximately 10% of ALS cases is inherited, with multiple autosomal dominant and recessive forms that have been ascribed to mutations in a number of different genes, each of them accounting for a different percentage of cases (Table 1). Interestingly, ALS-associated mutated proteins are implicated in a wide range of cellular processes, from antioxidant response to axonal and vesicular transport, angiogenesis, endoplasmic reticulum (ER) stress and unfolded protein response (UPR), and, most noticeably, to RNA metabolism.

Table 1.

Genes involved in MNDs.

Gene Protein MND Main known function
SOD1 Cu, Zn superoxide dismutase ALS1 Antioxidant enzyme
ALS2 Alsin ALS2 guanine nucleotide exchange factor for GTPases
SETX Senataxin ALS4 DNA/RNA metabolism and repair
SPG11 Spataxin ALS5 Neuron differentiation and axonal transport
FUS/TLS Fused in sarcoma ALS6 RNA binding protein
VAPB VAMP-associated protein B ALS8 Trafficking between the endoplasmic reticulum and Golgi apparatus
TDP-43 TAR-DNA-binding protein-43 ALS9 DNA- and RNA-binding protein
ANG Angiogenin ALS10 Angiogenesis in response to hypoxia; possibly RNA metabolism
FIG4 PI(3,5)P(2)5-phosphatase ALS11 Metabolism of phosphatidyl inositol bisphosphate and vesicle dynamic
OPTN Optineurin ALS12 Vesicular trafficking
nAChR Neuronal nicotinic acetylcholine receptor ALS Glutamatergic pathway
CHMP2B Charged multivesicular protein 2B ALS Chromatin-modifying protein/charged multivesicular body protein family
VCP Valosin-containing protein ALS Membrane trafficking, organelle biogenesis, maturation of ubiquitin-containing autophagosomes
DAO D-aminoacid oxidase ALS Oxidative deamination of D-aminoacid
UBQLN2 Ubiquilin2 ALS Ubiquitin-proteasome response
Sig-1R Sigma-1 receptor ALS ER chaperone, modulates calcium signaling through the IP3 receptor
C9ORF72 Unknown ALS Unknown
AR Androgen receptor SBMA Androgen receptor
SMN Survival Motor Neuron SMA RNA processing
GLE1 Nucleoporin GLE1 LCCS1 Export of mRNAs containing poly(A)

3. Multifactoriality of MNDs: The Role of Altered Gene Expression

At the cellular level, MNDs share features such as protein misfolding and aggregation, mitochondrial damage and energy deficit, excitotoxicity, and calcium mishandling [1], a condition often indicated as multifactoriality. This is particularly well demonstrated in ALS, where both sporadic and familial forms share the same symptoms and pathological phenotype, that are recapitulated in available animal and cell models, with a prominent role for mitochondrial damage and resulting oxidative stress (for an extended Review, see [25]). Oxidative stress is reported also in SMA [26] and reactive oxygen species (ROS) inhibit assembly and activity of SMN complex in a dose-dependent manner [27]. Mitochondrial damage seems to be invariably present in neurodegenerative conditions [28] including SMA [2932] and SBMA [33], in which mitochondrial dysfunction may be due to the interaction between AR and cytochrome c oxidase subunit Vb (COXVb) [34].

Based on recent data, however, altered control of gene expression seems to be a most relevant, and previously overlooked, player in MNDs.

Several studies addressing epigenetic modifications, transcriptomics, and proteomics of models and tissues from patients indicate that the overall pattern of gene expression is modified in MNDs. Because of the known non-cell autonomous mechanism of death of motor neurons, studies in ALS have been performed in tissues [35, 36] and in neuronal and in nonneuronal cultured cells (astrocytes, muscle) and revealed that most of the deregulated genes are involved in defense responses, cytoskeletal dynamics, protein degradation system, and mitochondrial dysfunction in neurons [37], while the insulin-like growth factor-1 receptor and the RNA-binding protein ROD1 are the most downregulated genes in glia [38]. The pattern is altered also in muscle, in which many of deregulated genes are the same found in surgically denervated muscles, while others appear to be ALS-specific and include proteins clearly involved in the redox response (e.g., metallothionein-2 and thioredoxin-1) [39, 40]. In a recent proteomic study on embryonic stem cell from a severe SMA mouse model differentiated into motor neurons in vitro, Wu et al. reported that 6 proteins are downregulated and 14 upregulated in this model. Most of these proteins belong to the same categories altered in ALS models, that is, are involved in energy metabolism, cell stress response, protein degradation, and cytoskeleton stability [41].

As in other neurodegenerative conditions, alterations of transcription in MNDs may follow altered epigenetic control due to an unbalance between histone acetyl transferases (HATs) and histone deacetylases (HDACs, including sirtuins, SIRTs) activities [42]. These enzymes catalyze forward and reverse reactions of lysine residue acetylation; thus, HATs modify core histone tails thereby enhancing DNA accessibility to transcription factors (TFs), while HDACs activity in general results in transcriptional repression and gene silencing. Interestingly, various TFs, like RelA, E2F, p53, and GATA1, which form part of the transcription initiation complex, are themselves substrates susceptible to the action of HATs and HDACs.

Evidence for the involvement of this kind of regulation in MNDs is accumulating, although still far from definitive, and unspecific HDAC inhibitors such as sodium phenylbutyrate, trichostatin A, and valproic acid have been tested as neuroprotective drugs for the treatment of ALS with some positive result [4347]. It is interesting to note that valproic acid is also endowed with antioxidative and antiapoptotic properties. However, most likely only selected HDACs participate to onset or propagation of motor neuron damage and thus must be targeted for an effective therapy. This concept is strengthened by the observation that complexes formed by ALS-linked proteins TDP-43 and FUS/TLS control the expression level of HDAC6 [48].

The SMN gene has a reproducible pattern of histone acetylation that is largely conserved among different tissues and species [49] and several HDAC pan-inhibitors such as suberoylanilide hydroxamic acid (SAHA) [50], trichostatin A [51], and the benzamide M344 [52] increase SMN2 transcript and protein levels. Valproic acid is currently tested in phase I and II clinical trials for the treatment of SMA (http://clinicaltrials.gov /). However, valproic acid has also serious adverse effects in cell and mice models for SMA [53, 54] pointing again to the need of inhibition of selected HDACs in MNDs, especially in the light of a recent report that the SMN2 gene is differentially regulated by individual HDAC proteins and silencing of HDAC5 and 6 enhances inclusion of an alternatively spliced exon in SMN2 [55]. Finally, oral administration of the HDAC inhibitor sodium butyrate has been tested also in a transgenic mouse model of SBMA with some positive outcome but only within a narrow range of drug dosage [56].

Epigenetic control of transcription may also occur via methylation by DNA methyltransferases (DNMTs) or histone methyltransferases (HMTs), both using S-adenosylmethionine (SAM o AdoMet) as the methyl donor. DNA methylation in eukaryotes occurs by the covalent modification of cytosine residues (on the fifth carbon) in CpG dinucleotides, leading to gene silencing. Methylation of histones (as well as transcription factors) occurs on lysine or arginine. Methylated lysine residues can carry up to three methyl moieties on their amine group, whereas arginine can be mono- or dimethylated on the guanidinyl group. Lysine methylation of histones is associated with activation or repression of transcription, depending on the degree of methylation and on the residue location [57].

Methylation may be extremely relevant in MNDs if one considers, for instance, that recognition of some Sm proteins by the SMN complex (that mediates the assembly of the Sm proteins onto snRNAs involved in pre-mRNA splicing and histone mRNA processing) is dependent on symmetrical dimethyl arginine modifications of their RG-rich tails [58, 59]. This methylation is achieved by PRMT (protein arginine methyltransferase)5 or by PRMT7, two enzymes that function nonredundantly [60] and utilize SAM as methyl donor. Furthermore, the SMN2 gene is subject to gene silencing by DNA methylation and some HDAC inhibitors including vorinostat and romidepsin are able to bypass SMN2 gene silencing by DNA methylation, while others such as valproic acid and phenylbutyrate are not [61].

Other observations support the concept that MNDs may be considered as “RNA dysmetabolisms” [62]. As reported in Table 1, several of the genetic factors involved in MNDs encode proteins with a role in RNA metabolism, and some overlap may exist among different diseases. For instance, copy number abnormalities of the SMN genes have been reported in sporadic ALS, although decrease of SMN protein in the anterior horn cells of ALS patients may be only a secondary phenomenon [63, 64]. RNA metabolism, however, consists of several intertwined steps, such as pre-mRNA splicing, mRNA transport, translational regulation, or mRNA decay, and the precise RNA pathway that is affected in a single MND remains unknown because virtually every one of the involved RNA-binding proteins has been implicated in more than one of these steps. Thus, it is not clear why motor neurons are so vulnerable to mutations in RNA-binding proteins.

Very recently, familial ALS has been associated with an expansion of a noncoding GGGGCC hexanucleotide repeat in the gene C9ORF72 [65, 66] that codes for an unknown protein. The transcribed GGGGCC repeat forms intracellular accumulations of RNA fragments in cells in the frontal cortex and the spinal cord from patients carrying the expansion [65]. These RNA foci are composed of the expanded nucleotide repeats that may disturb transcription by sequestering RNA-binding proteins involved in transcription regulation as observed for other expanded RNA repeats diseases [67] such as myotonic dystrophy [68]. Interestingly, the GGGGCC sequence also represents a potential binding site of several RNA-binding proteins including hnRNP A2/B1, a TDP-43 interactor [69, 70].

4. Altered Gene Expression, Mitochondrial Damage, and Oxidative Stress in MNDs: Which Are the Links?

Which are the links among altered gene expression, mitochondrial damage, and oxidative stress in MNDs is not clear yet. While oxidative stress and mitochondrial dysfunction are obviously connected into a vicious cycle in which excess in ROS production may influence the functionality of the organelles, that in turn would produce excess ROS, the connection with altered gene expression in MNDs is still somewhat foggy.

A few considerations may help to shed some light on possible, not mutually exclusive, mechanisms.

In analogy to what has been proposed in development [71] and in cancer [72], an interplay among oxidative stress, thiol redox signaling, and epigenetic modulation by methylation may be critical in motor neurons. The antioxidant capacity of cells is influenced by the production of glutathione (GSH), and increased GSH production influences DNA and histone methylation by limiting the availability of SAM, the cofactor utilized during epigenetic control of gene expression by DNA and histone methyltransferases [71]. The above mentioned forms of methylation, which are relevant in MNDs, are not directly linked, since they involve different enzymes and different targets. However, they all require the same methyl donor, which could be limiting in MNDs.

HDACs themselves seem to be linked to and modulated by oxidative stress. Pan-HDAC inhibition promotes neuronal protection against oxidative stress in a model of glutathione depletion [73], thus suggesting that HDACs are downstream mediator in the mechanisms of toxicity by ROS, while carbonylation of reactive cysteines of some, but not all, class I HDACs causes reduction of histone deacetylase activity and change in histones acetylation and transcription of genes repressed by these HDACs [74]. Thus, oxidative stress may be a modulator of gene expression through the modulation of DNA accessibility.

In turn, the activity of HDACs modulates alternative splicing of human genes when the nascent RNA is still associated with chromatin (in particular the splicing of hundreds of genes is altered upon HDAC inhibition) [75] but also the activity of various TFs. Noticeably, oxidative stress is also a modulator of several TFs and thus ROS and HDACs may concur in the generation of a pathological phenotype through the same mechanism. For instance, as reviewed by Rahman et al. [76], oxidative stress inhibits HDAC activity and activates HAT activity; this leads to NF-κB activation, which, in turn activates proinflammatory mediators. The antioxidant and/or anti-inflammatory effects of thiol molecules (GSH, N-acetyl-L-cysteine and Nacystelyn) and dietary polyphenols (e.g., curcumin and resveratrol) have a role in either the control of NF-κB activation or the modulation of HDAC. Thus, oxidative stress may regulate both TFs and chromatin remodeling which in turn impacts on proinflammatory responses.

Furthermore, SIRTs (class III HDACs) control the expression or the activity of a number of proteins involved in redox regulation (Table 2). Among these proteins, some are mitochondrial and many have been involved in one or more MNDs by transcriptomic/proteomic studies [7779].

Table 2.

Effects of class II HDACs (Sirtuins) on redox-related proteins.

Sirtuin Target Effect Reference
SIRT1 (nucleus and mitochondria) FOXO3a ↑ Transcriptional activity [82]
PGC-1α ↑ Transcriptional coactivation [83, 84]
HIF1α ↓ Transcriptional activity [85]
HIF2α ↑ Transcriptional activity [86]
eNOS ↑ Enzyme activity [87]
p53 Mediates transcriptional activity, depending on SIRT1 expression level [88, 89]
SIRT2 (cytoplasm) FOXO3a ↑ Transcriptional activity [90]
SIRT3 (mitochondria) HIF1α ↓ Transcriptional activity [91]
SOD2 ↑ Enzyme activity [92, 93]
OTC ↑ Enzyme activity [94]
NDUFA9 ↑ Enzyme activity [95]
GDH ↑ Enzyme activity [96]
IDH2 ↑ Enzyme activity [97]
SIRT4 (mitochondria) GDH ↓ Enzyme activity [98]
SIRT5 (mitochondria) CPS1 ↑ Enzyme activity [99]
SIRT6 (mitochondria) HIF1α ↓ Transcriptional activity [100]
SIRT7 (nucleoli) p53 Mediates transcriptional activity, depending on SIRT7 expression level [101]

CPS1: carbamoyl phosphate synthetase 1; eNOS: endothelial nitric oxide synthase; FOXO3a: Forkhead box O3 a; GDH: glutamate dehydrogenase; HIF1α: hypoxia-inducible factor 1, alpha subunit; HIF2α: hypoxia-inducible factor 2, alpha subunit; IDH2: isocitrate dehydrogenase 2; NDUFA9: NADH dehydrogenase [ubiquinone] 1 alpha subcomplex subunit 9; OTC: ornithine transcarbamylase; PGC-1α: Peroxisome proliferator-activated receptor gamma coactivator 1-alpha; SOD2: superoxide dismutase 2.

Last, but not the least, we have reported that mitochondrial damage itself is a cause of modification in the abundance of selected splicing variants [80] and that defective RNA metabolism seems to play a role also in SOD1-linked ALS and to descend directly from mitochondrial stress [81].

5. A Unifying Mechanism for MNDs?

From what summarized above, it is tempting to speculate that indeed all MNDs are mainly forms of RNA dysmetabolisms. Motor neurons seem to be exceedingly susceptible to defects in RNA transcription or processing; one appealing explanation is that they require that RNA is not only correctly transcribed and spliced, but also correctly transported along axons to neuromuscular junctions (NMJ). While there is no clear demonstration of the presence of mRNAs at the NMJs yet, this process (at least in ALS) might resent from the known alterations in axonal transport that precedes onset of symptoms [102].

However, one form or the other of alteration of RNA expression may have different weight in different MNDs and, most importantly, RNA dysmetabolisms may be a primary event (for instance in SMA or in TDP43- and FUS/TLS-linked ALS) or dysregulation of components of the genetic machinery (the HATs/HDACs system, transcription factors, the splicing complex) may be secondary to oxidative stress or energy failure. In turn, which step is the primary site of damage may dictate the severity of disease (age of onset, progression), and which cell type beside motor neurons is primarily affected may dictate the form of MND. This field surely deserves further investigation aimed to the individuation of novel therapeutic approaches for MNDs.

Acknowledgments

L. Rossi research is supported by Grants from MIUR (PRIN 2008J2LRWZ); M. T. Carrì research is supported by Grants from MIUR (PRIN 20083R593R), IMI-San Paolo and ERA-Net Neuron.

Abbreviations

ALS:

Amyotrophic lateral sclerosis

ALS2:

Alsin

ANG:

Angiogenin

AR:

Androgen receptor

CHMP2B:

Charged multivesicular protein 2B

COXVb:

Cytochrome c oxidase subunit Vb

DAO:

D-amino acid oxidase

DNMT:

DNA methyltransferase

ER:

Endoplasmic reticulum

FIG4:

PI(3,5)P(2)5-phosphatase

FUS/TLS:

Fused in sarcoma/translocated in liposarcoma

GLE1:

Nucleoporin GLE1

GSH:

Glutathione

HAT:

Histone acetyl transferase

HDAC:

Histone deacetylase

HMT:

Histone methyltransferase

LCCS:

Lethal congenital contracture syndrome

MND:

Motor neuron disease

nAChR:

Neuronal nicotinic acetylcholine receptor

OPTN:

Optineurin;

PBP:

Progressive bulbar palsy

PLS:

Primary lateral sclerosis

PMA:

Progressive muscular atrophy

PRMT5:

Protein arginine methyltransferase 5

PRMT7:

Protein arginine methyltransferase 7

ROS:

Reactive oxygen species

SAHA:

Suberoylanilide hydroxamic acid

SAM:

S-adenosylmethionine

SBMA:

Spinal and bulbar muscular atrophy

SETX:

Senataxin

Sig-1R Sigma:

1 receptor

SIRT:

Sirtuin

SMA:

Spinal muscular atrophy

SMN:

Survival motor neuron

SOD1:

Cu, Zn superoxide dismutase

SPG11:

Spataxin

TDP-43:

TAR DNA-binding protein 43

TF:

Transcription factor

UBQLN2:

Ubiquilin 2

UPR:

Unfolded protein response

VAPB:

VAMP-associated protein

VCP:

Valosin-containing protein.

References

  • 1.Saxena S, Caroni P. Selective neuronal vulnerability in neurodegenerative diseases: from stressor thresholds to degeneration. Neuron. 2011;71(1):35–48. doi: 10.1016/j.neuron.2011.06.031. [DOI] [PubMed] [Google Scholar]
  • 2.Strong MJ, Gordon PH. Primary lateral sclerosis, hereditary spastic paraplegia and amyotrophic lateral sclerosis: discrete entities or spectrum? Amyotrophic Lateral Sclerosis and Other Motor Neuron Disorders. 2005;6(1):8–16. doi: 10.1080/14660820410021267. [DOI] [PubMed] [Google Scholar]
  • 3.Nousiainen HO, Kestilä M, Pakkasjärvi N, et al. Mutations in mRNA export mediator GLE1 result in a fetal motoneuron disease. Nature Genetics. 2008;40(2):155–157. doi: 10.1038/ng.2007.65. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 4.Lunn MR, Wang CH. Spinal muscular atrophy. The Lancet. 2008;371(9630):2120–2133. doi: 10.1016/S0140-6736(08)60921-6. [DOI] [PubMed] [Google Scholar]
  • 5.Sobue G, Hashizume Y, Mukai E, Hirayama M, Mitsuma T, Takahashi A. X-linked recessive bulbospinal neuronopathy. A clinicopathological study. Brain. 1989;112, part 1:209–232. doi: 10.1093/brain/112.1.209. [DOI] [PubMed] [Google Scholar]
  • 6.La Spada AR, Wilson EM, Lubahn DB, Harding AE, Fischbeck KH. Androgen receptor gene mutations in X-linked spinal and bulbar muscular atrophy. Nature. 1991;352(6330):77–79. doi: 10.1038/352077a0. [DOI] [PubMed] [Google Scholar]
  • 7.Sperfeld AD, Karitzky J, Brummer D, et al. X-linked bulbospinal neuronopathy: Kennedy disease. Archives of Neurology. 2002;59(12):1921–1926. doi: 10.1001/archneur.59.12.1921. [DOI] [PubMed] [Google Scholar]
  • 8.Udd B, Juvonen V, Hakamies L, et al. High prevalence of Kennedy’s disease Western Finland—is the syndrome underdiagnosed? Acta Neurologica Scandinavica. 1998;98(2):128–133. doi: 10.1111/j.1600-0404.1998.tb01732.x. [DOI] [PubMed] [Google Scholar]
  • 9.Valdmanis PN, Daoud H, Dion PA, Rouleau GA. Recent advances in the genetics of amyotrophic lateral sclerosis. Current Neurology and Neuroscience Reports. 2009;9(3):198–205. doi: 10.1007/s11910-009-0030-9. [DOI] [PubMed] [Google Scholar]
  • 10.Cox PA, Sacks OW. Cycad neurotoxins, consumption of flying foxes, and ALS-PDC disease in Guam. Neurology. 2002;58(6):956–959. doi: 10.1212/wnl.58.6.956. [DOI] [PubMed] [Google Scholar]
  • 11.Golomb BA, Kwon EK, Koperski S, Evans MA. Amyotrophic lateral sclerosis-like conditions in possible association with cholesterol-lowering drugs: an analysis of patient reports to the University of California, San Diego (UCSD) statin effects study. Drug Safety. 2009;32(8):649–661. doi: 10.2165/00002018-200932080-00004. [DOI] [PubMed] [Google Scholar]
  • 12.Harwood CA, McDermott CJ, Shaw PJ. Physical activity as an exogenous risk factor in motor neuron disease (MND): a review of the evidence. Amyotrophic Lateral Sclerosis. 2009;10(4):191–204. doi: 10.1080/17482960802549739. [DOI] [PubMed] [Google Scholar]
  • 13.Chiò A, Benzi G, Dossena M, Mutani R, Mora G. Severely increased risk of amyotrophic lateral sclerosis among Italian professional football players. Brain. 2005;128, part 3:472–476. doi: 10.1093/brain/awh373. [DOI] [PubMed] [Google Scholar]
  • 14.Wicks P, Ganesalingham J, Collin C, Prevett M, Leigh NP, Al-Chalabi A. Three soccer playing friends with simultaneous amyotrophic lateral sclerosis. Amyotrophic Lateral Sclerosis. 2007;8(3):177–179. doi: 10.1080/17482960701195220. [DOI] [PubMed] [Google Scholar]
  • 15.Kasarskis EJ, Lindquist JH, Coffman CJ, et al. Clinical aspects of ALS in Gulf War Veterans. Amyotrophic Lateral Sclerosis. 2009;10(1):35–41. doi: 10.1080/17482960802351029. [DOI] [PubMed] [Google Scholar]
  • 16.Vanacore N, Cocco P, Fadda D, Dosemeci M. Job strain, hypoxia and risk of amyotrophic lateral sclerosis: results from a death certificate study. Amyotrophic Lateral Sclerosis. 2010;11(5):430–434. doi: 10.3109/17482961003605796. [DOI] [PubMed] [Google Scholar]
  • 17.Chen H, Richard M, Sandler DP, Umbach DM, Kamel F. Head injury and amyotrophic lateral sclerosis. American Journal of Epidemiology. 2007;166(7):810–816. doi: 10.1093/aje/kwm153. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 18.Schmidt S, Kwee LC, Allen KD, Oddone EZ. Association of ALS with head injury, cigarette smoking and APOE genotypes. Journal of the Neurological Sciences. 2010;291(1-2):22–29. doi: 10.1016/j.jns.2010.01.011. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 19.McKee AC, et al. TDP-43 proteinopathy and motor neuron disease in chronic traumatic encephalopathy. Journal of Neuropathology and Experimental Neurology. 2010;69(9):918–929. doi: 10.1097/NEN.0b013e3181ee7d85. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 20.Gallo V, Bueno-De-Mesquita HB, Vermeulen R, et al. Smoking and risk for amyotrophic lateral sclerosis: analysis of the EPIC cohort. Annals of Neurology. 2009;65(4):378–385. doi: 10.1002/ana.21653. [DOI] [PubMed] [Google Scholar]
  • 21.Kamel F, Umbach DM, Hu H, et al. Lead exposure as a risk factor for amyotrophic lateral sclerosis. Neurodegenerative Diseases. 2005;2(3-4):195–201. doi: 10.1159/000089625. [DOI] [PubMed] [Google Scholar]
  • 22.Brooks BR. Risk factors in the early diagnosis of ALS: North American epidemiological studies. Amyotrophic Lateral Sclerosis and Other Motor Neuron Disorders. 2000;1(supplement 1):S19–S26. doi: 10.1080/14660820052415871. [DOI] [PubMed] [Google Scholar]
  • 23.Burns CJ, Beard KK, Cartmill JB. Mortality in chemical workers potentially exposed to 2,4-dichlorophenoxyacetic acid (2,4-D) 1945-94: an update. Occupational and Environmental Medicine. 2001;58(1):24–30. doi: 10.1136/oem.58.1.24. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 24.Sutedja NA, Veldink JH, Fischer K, et al. Exposure to chemicals and metals and risk of amyotrophic lateral sclerosis: a systematic review. Amyotrophic Lateral Sclerosis. 2009;10(5-6):302–309. doi: 10.3109/17482960802455416. [DOI] [PubMed] [Google Scholar]
  • 25.Cozzolino M, Carri MT. Mitochondrial dysfunction in ALS. Progress in Neurobiology. 2012;97(2):54–66. doi: 10.1016/j.pneurobio.2011.06.003. [DOI] [PubMed] [Google Scholar]
  • 26.Hayashi M, Araki S, Arai N, et al. Oxidative stress and disturbed glutamate transport in spinal muscular atrophy. Brain and Development. 2002;24(8):770–775. doi: 10.1016/s0387-7604(02)00103-1. [DOI] [PubMed] [Google Scholar]
  • 27.Wan L, Ottinger E, Cho S, Dreyfuss G. Inactivation of the SMN complex by oxidative stress. Molecular Cell. 2008;31(2):244–254. doi: 10.1016/j.molcel.2008.06.004. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 28.Schon EA, Przedborski S. Mitochondria: the next (Neurode) generation. Neuron. 2011;70(6):1033–1053. doi: 10.1016/j.neuron.2011.06.003. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 29.Berger A, Mayr JA, Meierhofer D, et al. Severe depletion of mitochondrial DNA in spinal muscular atrophy. Acta Neuropathologica. 2003;105(3):245–251. doi: 10.1007/s00401-002-0638-1. [DOI] [PubMed] [Google Scholar]
  • 30.Jongpiputvanich S, Sueblinvong T, Norapucsunton T. Mitochondrial respiratory chain dysfunction in various neuromuscular diseases. Journal of Clinical Neuroscience. 2005;12(4):426–428. doi: 10.1016/j.jocn.2004.06.014. [DOI] [PubMed] [Google Scholar]
  • 31.Acsadi G, Lee I, Li X, et al. Mitochondrial dysfunction in a neural cell model of spinal muscular atrophy. Journal of Neuroscience Research. 2009;87(12):2748–2756. doi: 10.1002/jnr.22106. [DOI] [PubMed] [Google Scholar]
  • 32.Voigt T, Meyer K, Baum O, Schümperli D. Ultrastructural changes in diaphragm neuromuscular junctions in a severe mouse model for Spinal Muscular Atrophy and their prevention by bifunctional U7 snRNA correcting SMN2 splicing. Neuromuscular Disorders. 2010;20(11):744–752. doi: 10.1016/j.nmd.2010.06.010. [DOI] [PubMed] [Google Scholar]
  • 33.Ranganathan S, Harmison GG, Meyertholen K, Pennuto M, Burnett BG, Fischbeck KH. Mitochondrial abnormalities in spinal and bulbar muscular atrophy. Human Molecular Genetics. 2009;18(1):27–42. doi: 10.1093/hmg/ddn310. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 34.Beauchemin AMJ, Gottlieb B, Beitel LK, Elhaji YA, Pinsky L, Trifiro MA. Cytochrome c oxidase subunit Vb interacts with human androgen receptor: a potential mechanism for neurotoxicity in spinobulbar muscular atrophy. Brain Research Bulletin. 2001;56(3-4):285–297. doi: 10.1016/s0361-9230(01)00583-4. [DOI] [PubMed] [Google Scholar]
  • 35.Malaspina A, Kaushik N, de Belleroche J. Differential expression of 14 genes in amyotrophic lateral sclerosis spinal cord detected using gridded cDNA arrays. Journal of Neurochemistry. 2001;77(1):132–145. doi: 10.1046/j.1471-4159.2001.t01-1-00231.x. [DOI] [PubMed] [Google Scholar]
  • 36.Lederer CW, Torrisi A, Pantelidou M, Santama N, Cavallaro S. Pathways and genes differentially expressed in the motor cortex of patients with sporadic amyotrophic lateral sclerosis. BMC Genomics. 2007;8, article 26 doi: 10.1186/1471-2164-8-26. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 37.Tanaka F, et al. Neuropathology and omics in motor neuron diseases. doi: 10.1111/j.1440-1789.2011.01281.x. Neuropathology. In press. [DOI] [PubMed] [Google Scholar]
  • 38.Vargas MR, Pehar M, Díaz-Amarilla PJ, Beckman JS, Barbeito L. Transcriptional profile of primary astrocytes expressing ALS-linked mutant SOD1. Journal of Neuroscience Research. 2008;86(16):3515–3525. doi: 10.1002/jnr.21797. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 39.Gonzalez de Aguilar JL, Niederhauser-Wiederkehr C, Halter B, et al. Gene profiling of skeletal muscle in an amyotrophic lateral sclerosis mouse model. Physiological Genomics. 2008;32(2):207–218. doi: 10.1152/physiolgenomics.00017.2007. [DOI] [PubMed] [Google Scholar]
  • 40.Pradat PF, et al. Muscle gene expression is a marker of amyotrophic lateral sclerosis severity. Neuro-Degenerative Diseases. 2012;9(1):38–52. doi: 10.1159/000329723. [DOI] [PubMed] [Google Scholar]
  • 41.Wu CY, Whye D, Glazewski L, et al. Proteomic assessment of a cell model of spinal muscular atrophy. BMC Neuroscience. 2011;12, article 25 doi: 10.1186/1471-2202-12-25. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 42.Saha RN, Pahan K. HATs and HDACs in neurodegeneration: A tale of disconcerted acetylation homeostasis. Cell Death and Differentiation. 2006;13(4):539–550. doi: 10.1038/sj.cdd.4401769. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 43.Petri S, Kiaei M, Kipiani K, et al. Additive neuroprotective effects of a histone deacetylase inhibitor and a catalytic antioxidant in a transgenic mouse model of amyotrophic lateral sclerosis. Neurobiology of Disease. 2006;22(1):40–49. doi: 10.1016/j.nbd.2005.09.013. [DOI] [PubMed] [Google Scholar]
  • 44.Cudkowicz ME, Andres PL, Macdonald SA, et al. Phase 2 study of sodium phenylbutyrate in ALS. Amyotrophic Lateral Sclerosis. 2009;10(2):99–106. doi: 10.1080/17482960802320487. [DOI] [PubMed] [Google Scholar]
  • 45.Sugai F, Yamamoto Y, Miyaguchi K, et al. Benefit of valproic acid in suppressing disease progression of ALS model mice. European Journal of Neuroscience. 2004;20(11):3179–3183. doi: 10.1111/j.1460-9568.2004.03765.x. [DOI] [PubMed] [Google Scholar]
  • 46.Feng HL, Leng Y, Ma CH, Zhang J, Ren M, Chuang DM. Combined lithium and valproate treatment delays disease onset, reduces neurological deficits and prolongs survival in an amyotrophic lateral sclerosis mouse model. Neuroscience. 2008;155(3):567–572. doi: 10.1016/j.neuroscience.2008.06.040. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 47.Yoo YE, Ko CP. Treatment with trichostatin A initiated after disease onset delays disease progression and increases survival in a mouse model of amyotrophic lateral sclerosis. Experimental Neurology. 2011;231(1):147–159. doi: 10.1016/j.expneurol.2011.06.003. [DOI] [PubMed] [Google Scholar]
  • 48.Kim SH, Shanware NP, Bowler MJ, Tibbetts RS. Amyotrophic lateral sclerosis-associated proteins TDP-43 and FUS/TLS function in a common biochemical complex to co-regulate HDAC6 mRNA. The Journal of Biological Chemistry. 2010;285(44):34097–34105. doi: 10.1074/jbc.M110.154831. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 49.Kernochan LE, Russo ML, Woodling NS, et al. The role of histone acetylation in SMN gene expression. Human Molecular Genetics. 2005;14(9):1171–1182. doi: 10.1093/hmg/ddi130. [DOI] [PubMed] [Google Scholar]
  • 50.Hahnen E, Eyüpoglu IY, Brichta L, et al. In vitro and ex vivo evaluation of second-generation histone deacetylase inhibitors for the treatment of spinal muscular atrophy. Journal of Neurochemistry. 2006;98(1):193–202. doi: 10.1111/j.1471-4159.2006.03868.x. [DOI] [PubMed] [Google Scholar]
  • 51.Avila AM, Burnett BG, Taye AA, et al. Trichostatin A increases SMN expression and survival in a mouse model of spinal muscular atrophy. Journal of Clinical Investigation. 2007;117(3):659–671. doi: 10.1172/JCI29562. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 52.Riessland M, Brichta L, Hahnen E, Wirth B. The benzamide M344, a novel histone deacetylase inhibitor, significantly increases SMN2 RNA/protein levels in spinal muscular atrophy cells. Human Genetics. 2006;120(1):101–110. doi: 10.1007/s00439-006-0186-1. [DOI] [PubMed] [Google Scholar]
  • 53.Rak K, Lechner BD, Schneider C, Drexl H, Sendtner M, Jablonka S. Valproic acid blocks excitability in SMA type I mouse motor neurons. Neurobiology of Disease. 2009;36(3):477–487. doi: 10.1016/j.nbd.2009.08.014. [DOI] [PubMed] [Google Scholar]
  • 54.Fuller HR, Man NT, Lam LT, Shamanin VA, Androphy EJ, Morris GE. Valproate and bone loss: iTRAQ proteomics show that valproate reduces collagens and osteonectin in SMA cells. Journal of Proteome Research. 2010;9(8):4228–4233. doi: 10.1021/pr1005263. [DOI] [PubMed] [Google Scholar]
  • 55.Evans MC, Cherry JJ, Androphy EJ, et al. Differential regulation of the SMN2 gene by individual HDAC proteins. Biochemical and Biophysical Research Communications. 2011;414(1):25–30. doi: 10.1016/j.bbrc.2011.09.011. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 56.Minamiyama M, Katsuno M, Adachi H, et al. Sodium butyrate ameliorates phenotypic expression in a transgenic mouse model of spinal and bulbar muscular atrophy. Human Molecular Genetics. 2004;13(11):1183–1192. doi: 10.1093/hmg/ddh131. [DOI] [PubMed] [Google Scholar]
  • 57.Berger SL. The complex language of chromatin regulation during transcription. Nature. 2007;447(7143):407–412. doi: 10.1038/nature05915. [DOI] [PubMed] [Google Scholar]
  • 58.Tapia O, Bengoechea R, Berciano MT, Lafarga M. Nucleolar targeting of coilin is regulated by its hypomethylation state. Chromosoma. 2010;119(5):527–540. doi: 10.1007/s00412-010-0276-7. [DOI] [PubMed] [Google Scholar]
  • 59.Tripsianes K. Structural basis for dimethylarginine recognition by the Tudor domains of human SMN and SPF30 proteins. Nature Structural & Molecular Biology. 2011;18(12):1414–1420. doi: 10.1038/nsmb.2185. [DOI] [PubMed] [Google Scholar]
  • 60.Gonsalvez GB, Tian L, Ospina JK, Boisvert FM, Lamond AI, Matera AG. Two distinct arginine methyltransferases are required for biogenesis of Sm-class ribonucleoproteins. Journal of Cell Biology. 2007;178(5):733–740. doi: 10.1083/jcb.200702147. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 61.Hauke J, Riessland M, Lunke S, et al. Survival motor neuron gene 2 silencing by DNA methylation correlates with spinal muscular atrophy disease severity and can be bypassed by histone deacetylase inhibition. Human Molecular Genetics. 2009;18(2):304–317. doi: 10.1093/hmg/ddn357. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 62.Bäumer D, Ansorge O, Almeida M, Talbot K. The role of RNA processing in the pathogenesis of motor neuron degeneration. Expert Reviews in Molecular Medicine. 2010;12:p. e21. doi: 10.1017/S1462399410001523. [DOI] [PubMed] [Google Scholar]
  • 63.Corcia P, Camu W, Praline J, Gordon PH, Vourch P, Andres C. The importance of the SMN genes in the genetics of sporadic ALS. Amyotrophic Lateral Sclerosis. 2009;10(5-6):436–440. doi: 10.3109/17482960902759162. [DOI] [PubMed] [Google Scholar]
  • 64.Piao Y, Hashimoto T, Takahama S, et al. Survival motor neuron (SMN) protein in the spinal anterior horn cells of patients with sporadic amyotrophic lateral sclerosis. Brain Research. 2011;1372:152–159. doi: 10.1016/j.brainres.2010.11.070. [DOI] [PubMed] [Google Scholar]
  • 65.Dejesus-Hernandez M, et al. Expanded GGGGCC hexanucleotide repeat in noncoding region of C9ORF72 causes chromosome 9p-linked FTD and ALS. Neuron. 2011;72(2):245–256. doi: 10.1016/j.neuron.2011.09.011. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 66.Renton AE, et al. A hexanucleotide repeat expansion in C9ORF72 is the cause of chromosome 9p21-linked ALS-FTD. Neuron. 2011;72(2):257–268. doi: 10.1016/j.neuron.2011.09.010. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 67.Wojciechowska M, Krzyzosiak WJ. Cellular toxicity of expanded RNA repeats: focus on RNA foci. Human Molecular Genetics. 2011;20(19):3811–3821. doi: 10.1093/hmg/ddr299. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 68.Sicot G, Gourdon G, Gomes-Pereira M. Myotonic dystrophy, when simple repeats reveal complex pathogenic entities: new findings and future challenges. Human Molecular Genetics. 2011;20(2):R116–R123. doi: 10.1093/hmg/ddr343. [DOI] [PubMed] [Google Scholar]
  • 69.Buratti E, Brindisi A, Giombi M, Tisminetzky S, Ayala YM, Baralle FE. TDP-43 binds heterogeneous nuclear ribonucleoprotein A/B through its C-terminal tail: an important region for the inhibition of cystic fibrosis transmembrane conductance regulator exon 9 splicing. The Journal of Biological Chemistry. 2005;280(45):37572–37584. doi: 10.1074/jbc.M505557200. [DOI] [PubMed] [Google Scholar]
  • 70.Sofola OA, Jin P, Qin Y, et al. RNA-binding proteins hnRNP A2/B1 and CUGBP1 suppress fragile X CGG premutation repeat-induced neurodegeneration in a drosophila model of FXTAS. Neuron. 2007;55(4):565–571. doi: 10.1016/j.neuron.2007.07.021. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 71.Hitchler MJ, Domann FE. An epigenetic perspective on the free radical theory of development. Free Radical Biology and Medicine. 2007;43(7):1023–1036. doi: 10.1016/j.freeradbiomed.2007.06.027. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 72.Hitchler MJ, Domann FE. Metabolic defects provide a spark for the epigenetic switch in cancer. Free Radical Biology and Medicine. 2009;47(2):115–127. doi: 10.1016/j.freeradbiomed.2009.04.010. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 73.Langley B, D’Annibale MA, Suh K, et al. Pulse inhibition of histone deacetylases induces complete resistance to oxidative death in cortical neurons without toxicity and reveals a role for cytoplasmic p21waf1/cip1 in cell cycle-independent neuroprotection. Journal of Neuroscience. 2008;28(1):163–176. doi: 10.1523/JNEUROSCI.3200-07.2008. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 74.Doyle K, Fitzpatrick FA. Redox signaling, alkylation (carbonylation) of conserved cysteines inactivates class I histone deacetylases 1, 2, and 3 and antagonizes their transcriptional repressor function. The Journal of Biological Chemistry. 2010;285(23):17417–17424. doi: 10.1074/jbc.M109.089250. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 75.Hnilicová J, Hozeifi S, Dušková E, Icha J, Tománková T, Staněk D. Histone deacetylase activity modulates alternative splicing. PLoS ONE. 2011;6(2) doi: 10.1371/journal.pone.0016727. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 76.Rahman I, Marwick J, Kirkham P. Redox modulation of chromatin remodeling: Impact on histone acetylation and deacetylation, NF-κB and pro-inflammatory gene expression. Biochemical Pharmacology. 2004;68(6):1255–1267. doi: 10.1016/j.bcp.2004.05.042. [DOI] [PubMed] [Google Scholar]
  • 77.Li Q, Velde CV, Israelson A, et al. ALS-linked mutant superoxide dismutase 1 (SOD1) alters mitochondrial protein composition and decreases protein import. Proceedings of the National Academy of Sciences of the United States of America. 2010;107(49):21146–21151. doi: 10.1073/pnas.1014862107. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 78.Bergemalm D, Forsberg K, Andreas Jonsson P, et al. Changes in the spinal cord proteome of an amyotrophic lateral sclerosis murine model determined by differential in-gel electrophoresis. Molecular and Cellular Proteomics. 2009;8(6):1306–1317. doi: 10.1074/mcp.M900046-MCP200. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 79.Massignan T, Casoni F, Basso M, et al. Proteomic analysis of spinal cord of presymptomatic amyotrophic lateral sclerosis G93A SOD1 mouse. Biochemical and Biophysical Research Communications. 2007;353(3):719–725. doi: 10.1016/j.bbrc.2006.12.075. [DOI] [PubMed] [Google Scholar]
  • 80.Maracchioni A, Totaro A, Angelini DF, et al. Mitochondrial damage modulates alternative splicing in neuronal cells: Implications for neurodegeneration. Journal of Neurochemistry. 2007;100(1):142–153. doi: 10.1111/j.1471-4159.2006.04204.x. [DOI] [PubMed] [Google Scholar]
  • 81.Lenzken SC, Romeo V, Zolezzi F, et al. Mutant SOD1 and mitochondrial damage alter expression and splicing of genes controlling neuritogenesis in models of neurodegeneration. Human Mutation. 2011;32(2):168–182. doi: 10.1002/humu.21394. [DOI] [PubMed] [Google Scholar]
  • 82.Brunet A, Sweeney LB, Sturgill JF, et al. Stress-dependent regulation of FOXO transcription factors by the SIRT1 deacetylase. Science. 2004;303(5666):2011–2015. doi: 10.1126/science.1094637. [DOI] [PubMed] [Google Scholar]
  • 83.Lu Z, Xu X, Hu X, et al. PGC-1α regulates expression of myocardial mitochondrial antioxidants and myocardial oxidative stress after chronic systolic overload. Antioxidants and Redox Signaling. 2010;13(7):1011–1022. doi: 10.1089/ars.2009.2940. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 84.Aquilano K, Vigilanza P, Baldelli S, Pagliei B, Rotilio G, Ciriolo MR. Peroxisome proliferator-activated receptor γ co-activator 1 α (PGC-1α) and sirtuin 1 (SIRT1) reside in mitochondria: possible direct function in mitochondrial biogenesis. The Journal of Biological Chemistry. 2010;285(28):21590–21599. doi: 10.1074/jbc.M109.070169. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 85.Lim JH, Lee YM, Chun YS, Chen J, Kim JE, Park JW. Sirtuin 1 modulates cellular responses to hypoxia by deacetylating hypoxia-inducible factor 1alpha. Molecular cell. 2010;38(6):864–878. doi: 10.1016/j.molcel.2010.05.023. [DOI] [PubMed] [Google Scholar]
  • 86.Dioum EM, Chen R, Alexander MS, et al. Regulation of hypoxia-inducible factor 2α signaling by the stress-responsive deacetylase sirtuin 1. Science. 2009;324(5932):1289–1293. doi: 10.1126/science.1169956. [DOI] [PubMed] [Google Scholar]
  • 87.Mattagajasingh I, Kim CS, Naqvi A, et al. SIRT1 promotes endothelium-dependent vascular relaxation by activating endothelial nitric oxide synthase. Proceedings of the National Academy of Sciences of the United States of America. 2007;104(37):14855–14860. doi: 10.1073/pnas.0704329104. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 88.Yang Y, Fu W, Chen J, et al. SIRT1 sumoylation regulates its deacetylase activity and cellular response to genotoxic stress. Nature Cell Biology. 2007;9(11):1253–1262. doi: 10.1038/ncb1645. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 89.Han MK, Song EK, Guo Y, Ou X, Mantel C, Broxmeyer HE. SIRT1 regulates apoptosis and Nanog expression in mouse embryonic stem cells by controlling p53 subcellular localization. Cell Stem Cell. 2008;2(3):241–251. doi: 10.1016/j.stem.2008.01.002. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 90.Wang F, Nguyen M, Qin FXF, Tong Q. SIRT2 deacetylates FOXO3a in response to oxidative stress and caloric restriction. Aging Cell. 2007;6(4):505–514. doi: 10.1111/j.1474-9726.2007.00304.x. [DOI] [PubMed] [Google Scholar]
  • 91.Bell EL, Emerling BM, Ricoult SJH, Guarente L. SirT3 suppresses hypoxia inducible factor 1α and tumor growth by inhibiting mitochondrial ROS production. Oncogene. 2011;30(26):2986–2996. doi: 10.1038/onc.2011.37. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 92.Tao R, Coleman MC, Pennington JD, et al. Sirt3-mediated deacetylation of evolutionarily conserved lysine 122 regulates MnSOD activity in response to stress. Molecular Cell. 2010;40(6):893–904. doi: 10.1016/j.molcel.2010.12.013. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 93.Chen Y, Zhang J, Lin Y, et al. Tumour suppressor SIRT3 deacetylates and activates manganese superoxide dismutase to scavenge ROS. EMBO Reports. 2011;12(6):534–541. doi: 10.1038/embor.2011.65. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 94.Hallows WC, Yu W, Smith BC, et al. Sirt3 promotes the urea cycle and fatty acid oxidation during dietary restriction. Molecular Cell. 2011;41(2):139–149. doi: 10.1016/j.molcel.2011.01.002. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 95.Ahn BH, Kim HS, Song S, et al. A role for the mitochondrial deacetylase Sirt3 in regulating energy homeostasis. Proceedings of the National Academy of Sciences of the United States of America. 2008;105(38):14447–14452. doi: 10.1073/pnas.0803790105. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 96.Lombard DB, Alt FW, Cheng HL, et al. Mammalian Sir2 homolog SIRT3 regulates global mitochondrial lysine acetylation. Molecular and Cellular Biology. 2007;27(24):8807–8814. doi: 10.1128/MCB.01636-07. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 97.Someya S, Yu W, Hallows WC, et al. Sirt3 mediates reduction of oxidative damage and prevention of age-related hearing loss under caloric restriction. Cell. 2010;143(5):802–812. doi: 10.1016/j.cell.2010.10.002. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 98.Haigis MC, Mostoslavsky R, Haigis KM, et al. SIRT4 inhibits glutamate dehydrogenase and opposes the effects of calorie restriction in pancreatic β cells. Cell. 2006;126(5):941–954. doi: 10.1016/j.cell.2006.06.057. [DOI] [PubMed] [Google Scholar]
  • 99.Nakagawa T, Lomb DJ, Haigis MC, Guarente L. SIRT5 deacetylates carbamoyl phosphate synthetase 1 and regulates the urea cycle. Cell. 2009;137(3):560–570. doi: 10.1016/j.cell.2009.02.026. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 100.Zhong L, D’Urso A, Toiber D, et al. The histone deacetylase Sirt6 regulates glucose homeostasis via Hif1α . Cell. 2010;140(2):280–293. doi: 10.1016/j.cell.2009.12.041. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 101.Vakhrusheva O, Smolka C, Gajawada P, et al. Sirt7 increases stress resistance of cardiomyocytes and prevents apoptosis and inflammatory cardiomyopathy in mice. Circulation Research. 2008;102(6):703–710. doi: 10.1161/CIRCRESAHA.107.164558. [DOI] [PubMed] [Google Scholar]
  • 102.Bilsland LG, Sahai E, Kelly G, Golding M, Greensmith L, Schiavo G. Deficits in axonal transport precede ALS symptoms in vivo. Proceedings of the National Academy of Sciences of the United States of America. 2010;107(47):20523–20528. doi: 10.1073/pnas.1006869107. [DOI] [PMC free article] [PubMed] [Google Scholar]

Articles from International Journal of Cell Biology are provided here courtesy of Wiley

RESOURCES