|Cell biology of spinocerebellar ataxia.|
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|PMID: 22508507 Owner: NLM Status: MEDLINE|
|Ataxia is a neurological disorder characterized by loss of control of body movements. Spinocerebellar ataxia (SCA), previously known as autosomal dominant cerebellar ataxia, is a biologically robust group of close to 30 progressive neurodegenerative diseases. Six SCAs, including the more prevalent SCA1, SCA2, SCA3, and SCA6 along with SCA7 and SCA17 are caused by expansion of a CAG repeat that encodes a polyglutamine tract in the affected protein. How the mutated proteins in these polyglutamine SCAs cause disease is highly debated. Recent work suggests that the mutated protein contributes to pathogenesis within the context of its "normal" cellular function. Thus, understanding the cellular function of these proteins could aid in the development of therapeutics.|
|Harry T Orr|
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|Type: Journal Article; Research Support, N.I.H., Extramural; Review|
|Title: The Journal of cell biology Volume: 197 ISSN: 1540-8140 ISO Abbreviation: J. Cell Biol. Publication Date: 2012 Apr|
|Created Date: 2012-04-17 Completed Date: 2012-06-07 Revised Date: 2013-06-26|
Medline Journal Info:
|Nlm Unique ID: 0375356 Medline TA: J Cell Biol Country: United States|
|Languages: eng Pagination: 167-77 Citation Subset: IM|
|Department of Laboratory Medicine and Pathology, University of Minnesota Medical School, Minneapolis, MN 55455, USA. firstname.lastname@example.org|
|APA/MLA Format Download EndNote Download BibTex|
Amino Acid Sequence
Nerve Tissue Proteins / genetics*, metabolism
Nuclear Proteins / genetics*, metabolism
Peptides / chemistry*
RNA-Binding Proteins / metabolism
Spinocerebellar Ataxias / genetics*
Trinucleotide Repeat Expansion*
|NS22920-23/NS/NINDS NIH HHS; NS45667-09/NS/NINDS NIH HHS|
|0/Nerve Tissue Proteins; 0/Nuclear Proteins; 0/Peptides; 0/RBM17 protein, human; 0/RNA-Binding Proteins; 0/ataxin-1; 26700-71-0/polyglutamine|
Journal ID (nlm-ta): J Cell Biol
Journal ID (iso-abbrev): J. Cell Biol
Journal ID (hwp): jcb
Publisher: The Rockefeller University Press
© 2012 Orr
Received Day: 18 Month: 5 Year: 2011
Accepted Day: 20 Month: 3 Year: 2012
Print publication date: Day: 16 Month: 4 Year: 2012
Volume: 197 Issue: 2
First Page: 167 Last Page: 177
PubMed Id: 22508507
Publisher Id: 201105092
|Cell biology of spinocerebellar ataxia Alternate Title:Cell biology of spinocerebellar ataxia|
|Harry T. Orr|
|Department of Laboratory Medicine and Pathology, University of Minnesota Medical School, Minneapolis, MN 55455
|Correspondence: Correspondence to Harry T. Orr: email@example.com
Individuals suffering from ataxia are at first clumsy and unable to walk steadily, and have slurred speech. Patients can eventually lose the ability to swallow and breathe in a coordinated fashion, which can be fatal. Ataxia results from variable degeneration of neurons in the cerebellum, brain stem, spinocerebellar tracts, and their afferent/efferent connections. Such neurodegenerations can be due to a variety of clinical conditions, including multiple sclerosis, a brain tumor, alcoholism, or an inherited genetic defect. There are over 50 different forms of inherited ataxias that strike during childhood or adulthood (Taroni and DiDonato, 2004; Manto, 2005). Among the inherited forms of ataxia are several recessive forms of ataxia that include Friedreich ataxia—the most common inherited form of ataxia that affects mitochondrial function, AVED ataxia due to vitamin E deficiency, and ataxia telangiectasia affecting regulation of the cell cycle. Spinocerebellar ataxias, or SCAs, are inherited in an autosomal-dominant pattern. There are ∼30 different types of SCA identified to date but causative mutations have been identified for only half of them. Among these are the ataxias caused by mutations in protein kinase C (SCA14) and fibroblast growth factor 14. Most of the SCAs are caused by an abnormal expansion of a CAG repeat sequence that encodes for an expanded tract of polyglutamine (polyQ) residues within the mutated protein. It is the polyQ SCAs that are the subject of this review.
The cellular and molecular mechanisms responsible for pathogenesis of the polyQ neurodegenerative diseases are a matter of spirited discussions. For the most part these discussions center on two major points. The first focuses on to what extent the polyglutamine tract alone drives pathogenesis. It is clear that expanded polyQ peptides are toxic, with early studies indicating that disease might stem from the proteolytic production of such peptides (Marsh et al., 2000). Yet, only for Huntington’s disease is there evidence that proteolytic cleavage and the generation of a toxic polyQ peptide might be required for pathogenesis (Davies et al., 1997; DiFiglia et al., 1997; Graham et al., 2006). The second point is whether the tendency of mutant polyQ proteins to aggregate is responsible for the disease-associated neurodegeneration. PolyQ expansion renders the protein more prone to aggregation and formation of inclusion bodies that are a pathological hallmark of these disorders including the polyQ SCAs (Orr and Zoghbi, 2007). Yet, the extent to which these inclusions cause disease continues to be a complex issue. There are several studies demonstrating that in mouse models disease severity can be disassociated from presence of inclusions (Klement et al., 1998; Saudou et al., 1998; Cummings et al., 1999), Moreover, there are data indicating that inclusions may be protective, perhaps by sequestration of the mutant protein (Cummings et al., 1999; Arrasate et al., 2004; Bowman et al., 2007).
More recent studies in both patients and model systems support the concept that the native/normal functions of the polyQ proteins are required for development of disease. Most notably, in the polyQ disease spinobulbar muscular atrophy (SBMA), where disease is caused by a polyQ expansion in the androgen receptor (La Spada et al., 1991), both androgen binding and nuclear translocation of mutant androgen receptor are required for development of the SBMA-associated motor neuron disease (Katsuno et al., 2002; Takeyama et al., 2002; Nedelsky et al., 2010). Moreover, disruption of androgen receptor interaction with its normal transcriptional coregulators suppresses disease in a Drosophila model of SBMA (Nedelsky et al., 2010). In the case of the polyQ SCA SCA1, interactions with its native partners are required for disease in a mouse model of SCA1 (Lim et al., 2008). Furthermore, a SCA-like neurological phenotype can be induced in mice that overexpress wild-type ataxin-1 with a single amino acid substitution outside of the polyQ tract that enhances its interaction with a native partner (Duvick et al., 2010).
Glutamine-rich regions are found in the activation domains characteristic of a large family of highly conserved transcription activators exemplified by specificity factor 1 (Sp1). Within the multiprotein TFIID transcription complex, the glutamine rich regions of these activators function as protein–protein interaction domains (Saluja et al., 1998) Thus, not surprisingly, an alteration in neuronal transcription is a prominent model for polyQ pathogenesis. Very recently, a study in Caenorhabditis elegans revealed another function associated with a glutamine-rich protein, control of nonapoptotic cell death. Blum et al. (2012) found that the C. elegans polyQ protein pqn-41 is critical for the onset of linker-cell death during normal reproductive system development. Death of linker cells shares several morphological features seen in neurons undergoing polyQ-induced degeneration, e.g., formation of intracellular aggregates of the polyQ protein. It remains to be determined the extent to which neurodegeneration in diseases such as the polyQ SCAs is related to the nonapoptotic linker cell death regulated by pgn-41.
An emerging concept is that understanding the polyQ SCA diseases will require an appreciation of the role these proteins have in basic cellular processes (Orr, 2001). Thus, this review focuses on those polyQ SCAs (SCA1, SCA2, SCA3, SCA6, SCA7, and SCA17) where the cellular processes involving the affected protein are being uncovered. These functions span cellular processes from those at the cell membrane and in the cytoplasm to functions in the nucleus. Understanding the cell biology of these disorders is providing crucial insight into the pathogenesis of these SCAs. It is also of note that the cerebellum is one of the better understood neuronal networks in the brain. Thus, the SCAs offer a paradigm for moving from human genetics to cell biology to pathophysiology, a point exemplified by recent pathophysiological studies on mouse models showing that ataxia is associated with alterations in Purkinje cell innervation in SCA1 (Barnes et al., 2011; Hourez et al., 2011), and with a decrease in Purkinje cell intrinsic firing rate in SCA3 (Shakkottai et al., 2011).
SCA1 is typically a late-onset fatal progressive neurodegenerative disease caused by the expansion of a polyQ tract within the ataxin-1 (ATXN1) protein (Orr et al., 1993). In the brain, cerebellar Purkinje neurons are a prominent pathological target of mutant ATXN1. ATXN1 is located in the cytoplasm and nucleus (Servadio et al., 1995), with the wild-type ATXN1 able to shuttle back and forth between these two subcellular compartments (Fig. 1). The dynamics of ataxin-1 within the nucleus is altered by expansion of the polyQ tract (Krol et al., 2008). Although mutant ATXN1 with an expanded polyQ tract is able to enter the nucleus, its ability to be transported back into the cytoplasm is dramatically reduced (Irwin et al., 2005). Also, the length of the polyQ tract negatively affects SUMOylation of ATXN1, which occurs when ATXN1 is able to be transported to the nucleus (Riley et al., 2005).
Other cellular molecules with which ATXN1 normally interacts include RNA (Yue et al., 2001), and several regulators of transcription, SMRT (Tsai et al., 2004), Capicua (Lam et al., 2006), Gfi-1 (Tsuda et al., 2005), and the Rora–Tip60 complex (Serra et al., 2006). In the case of Capicua and the Rora–Tip60 complex, mutant ATXN1 seems to enhance their degradation. For Capicua, loss of ATXN1 decreases its steady-state level (Lam et al., 2006). ATXN1 also interacts with two RNA-splicing factors, RBM17 (Lim et al., 2008) and U2AF65 (de Chiara et al., 2009).
Two evolutionarily conserved regions within ATXN1 drive these interactions; the 120-amino acid AXH domain (de Chiara et al., 2003; Chen et al., 2004), which interacts with Capicua (Lam et al., 2006), Rora–Tip60 (Gehrking et al., 2011), Gfi-1 (Tsuda et al., 2005) and ATXN1L (Bowman et al., 2007), and a 12-amino acid segment, residues 768–780 toward the C terminus of ATXN1. This C-terminal segment contains three overlapping functional motifs and an endogenous site of phosphorylation at Ser776 (S776; Emamian et al., 2003; Huttlin et al., 2010). The functional motifs in the C-terminal region include a nuclear localization sequence (NLS), amino acids 771–774 (Klement et al., 1998), a 14-3-3 binding motif, amino acids 774–778 (Chen et al., 2003), and a UHM ligand motif (ULM), amino acids 771–776 (de Chiara et al., 2009)
It is increasingly apparent that the amino acid stretch, encompassing residues 771–778 in the C-terminal portion of ATXN1, plays a key role in its function and the dysfunction associated with SCA1. First, inactivation of the NLS in ATXN1 and preventing mutant ATXN1 from entering the nucleus of neurons blocks the ability of ATXN1 with an expanded polyQ tract to cause neurodegeneration in vivo (Klement et al., 1998). Second, Ser776, immediately adjacent to the NLS, is an endogenous site of phosphorylation (Emamian et al., 2003; Huttlin et al., 2010). Phosphorylation of S776 stabilizes ATXN1 because the phospho-resistant Ala776 (A776) ATXN1 is far less stable than either S776 or phospho-mimicking Asp776 (D776) ATXN1 (Jorgensen et al., 2009; Lai et al., 2011). Studies indicate that S776 and perhaps its phosphorylation has a crucial role in regulating interactions of wild-type and mutant ATXN1 with at least three cellular proteins, the phospho-serine/phospho-threonine binding protein 14-3-3 (Chen et al., 2003), a regulator of many signal transduction pathways (Morrison, 2009), and splicing factors RBM17 (Lim et al., 2008) and U2AF65 (de Chiara et al., 2009).
The interaction of ATXN1 with RBM17 increases with increasing length of the polyQ tract whereas the interaction of RBM17 with ATXN1-A776 is decreased dramatically regardless of polyQ tract length (Lim et al., 2008). Interestingly, replacing S776 with an aspartic acid reside results in a form of ATXN1-30Q, ATXN1[30Q]-D776, that has an enhanced interaction with RBM17 similar to that seen with ATXN1[82Q]-S776. Moreover, expression of ATXN1[30Q]-D776 in Purkinje neurons of transgenic mice results in a disease similar to that seen with ATXN1[82Q]-S776 (Duvick et al., 2010). Importantly, ATXN1[82Q]-A776, which interacts weakly with RBM17 in tissue culture cells, is not pathogenic when expressed in Purkinje cells (Emamian et al., 2003). These results indicate a direct link between pathogenicity of mutant ATXN1 and its interaction with RBM17 and suggest that the phosphorylation state of serine 776 is critical for the strength of this interaction.
Together, the data support a model for an ATXN1 cellular pathway that involves its phosphorylation at S776 in the cytoplasm, with perhaps dopamine D2 receptor signaling having a role in regulating ATXN1-S776 phosphorylation by PKA (Jorgensen et al., 2009; Hearst et al., 2010). Binding of 14-3-3 to ATXN1 protects pS776 from being dephosphorylated and subsequently degraded. Because the 14-3-3 binding site is immediately adjacent to the NLS in ATXN1, 14-3-3 binding masks the NLS and blocks entry of ATXN1 into the nucleus (Lai et al., 2011). Thus, 14-3-3 would be released from ATXN1, presumably by some regulated process, for ATXN1 to be transported into the nucleus. Once in the nucleus critical interactions are with splicing factors RBM17 and U2AF65 because the relative activity of these pathways is regulated by the length of the polyQ tract in ATXN1 and phosphorylation status of S776 (Fig. 1). Because the extent to which ATXN1 interacts with RBM17 varies with length of the polyQ tract within wild-type alleles (Lim et al., 2008), one can speculate that ATXN1 normally functions to regulate the balance between the RBM17 and U2AF65 pathways. As the polyQ expands into the pathogenic range, the RBM17 pathway becomes abnormally favored (Fig. 1).
A second pathway in which ATXN1 participates is an association with the transcription repressor Capicua (Cic). The biological effect on Cic of ATXN1 polyQ expansion is complex. First, overexpression of Cic was protective (Lam et al., 2006) in a fly model of SCA1, whereas partial loss of Cic prolonged life span in mice (Fryer et al., 2011). It seems that for some Cic gene targets expanded ATXN1 causes a loss of function, whereas at other targets polyQ-expanded ATXN1 enhances Cic binding inducing a state of hyper-repression. In the mouse, it is postulated that the hyper-repressive effect of expanded polyQ ATXN1 is toxic (Fryer et al., 2011). Intriguingly, mild exercise perhaps involving the Cic pathway in the brainstem improves survival in a mouse model of SCA1 in absence of improving the cerebellar motor dysfunction (Fryer et al., 2011). Although more vigorous motor activity that engages the cerebellum might restore motor function, one also needs to consider that distinct ATXN1 complexes, i.e., cellular pathways, contribute to disease in different regions of the CNS. Such a hypothesis is supported by the ability of a partial loss of 14-3-3 to improve cerebellar phenotypes and not brainstem phenotypes (Jafar-Nejad et al., 2011).
Like other SCAs, SCA2 patients present with limb and gait ataxia (Gwinn-Hardy et al., 2000; Shan et al., 2001). The polyQ protein affected in SCA2, ATXN2, as well as closely related homologues are implicated in range of biological functions, including cell specification, actin filament formation, receptor-mediated signaling, and secretion (Satterfield et al., 2002; Huynh et al., 2003; Wiedemeyer et al., 2003).
Evidence indicates that ATXN2 is involved in this diverse group of functions by virtue of it having a role in cytoplasmic RNA-related functions, in particular the regulation of translation (Fig. 2). First of all, the primary sequence of ATXN2 contains Lsm (like-Sm) motifs known to function in RNA splicing and mRNA decay in the cytoplasm (Neuwald and Koonin, 1998). In addition, the ATXN2 sequence contains a polyA-binding protein (PABP) interacting motif PAM2 (Kozlov et al., 2001). Consequently, ATXN2 interacts with PABP (Ciosk et al., 2004; Ralser et al., 2005). ATXN2 also interacts with a putative RNA protein called ataxin-2–binding protein (Shibata et al., 2000). Studies indicate that important subcellular sites for the regulation of translation by ATXN2 are stress granules and P-bodies, the main cellular compartments for regulating mRNA degradation, and translation (Eulalio et al., 2007; Buchan and Parker, 2009). In addition to the PABP, another stress granule and P-body component with which ATXN2 interacts is the DEAD/H-box RNA helicase DDX6 (Nonhoff et al., 2007). This study also found that ATXN2 has a role in assembly of stress granules and P-bodies. Recently, McCann et al. (2011) found that Drosophila Atx2 is required for repression of several miRNA target mRNAs, suggesting that ATXN2 also functions in miRNA pathways.
Additional data linking ATXN2 to regulation of translation comes from studies on the homologues of ATXN2 in model organisms. For example, in yeast there is a genetic interaction between Pab1, a gene that promotes translation, and the yeast ATXN2 homologue Pbp1. Deletion of Pbp1 suppresses lethality due to loss of Pab1 (Mangus et al., 1998). Furthermore, overexpression of Pbp1 in yeast results in the same phenotype as seen inhibiting translation with cycloheximide (Dunn and Jensen, 2003). In C. elegans partial loss of function of the ATXN2 homologue ATX-2 alters the abundance of certain proteins without altering the level of their mRNAs, indicating that ATX-2 functions in the regulation of translation in C. elegans. More direct evidence that ATXN2 functions in translation comes from the Drosophila homologue of ATXN2, ATX2. By sucrose gradient centrifugation, ATX2 assembles with polyribosomes in a manner dependent on the Lsm and PAM2 motifs (Satterfield and Pallanck, 2006). This study also found that ATXN2 in transfected human HEK293 cells co-sediments with polyribosomes.
Thus, there are considerable data indicating that ATXN2 interacts with various components of the cellular machinery involved in the regulation of mRNA translation (Fig. 2). ATXN2’s association with components of translational active polysomes as well as translational silent RNA granules suggests a role in the regulated trafficking of mRNA between these structures that allows a cell to tailor translation to meet the needs of changes in its environment. Intriguingly, in a Drosophila model of synaptic plasticity, long-term olfactory habituation (LTH), Atx2 functions along with the miRNA pathway components Me31B and Ago1 to generate the synaptic plasticity associated with LTH that is linked to translational repression (McCann et al., 2011). Unfortunately, there is little data indicating whether and at what points in the cellular translational pathway SCA2-associated polyQ expansion alters ATXN2 function.
There is a suggestion that the polyQ tract length in ATXN2 affects risk for another neurodegenerative disorder, amyotrophic lateral sclerosis (ALS), providing additional evidence linking ATXN2 to RNA metabolism. Mutations in the gene encoding 43-kD TAR DNA-binding protein (TDP-43) are associated with some sporadic and familial forms of ALS (Lagier-Tourenne and Cleveland, 2009; Pesiridis et al., 2009). Normally predominantly in the nucleus, in pathological material TDP-43 localizes to cytoplasmic inclusions, leading to the hypothesis that an altered subcellular localization of TDP-43 is pathogenic. TDP-43 is a heterogeneous nuclear riboprotein, hnRNP, which associates with single-stranded nucleic acids and is implicated in several aspects of RNA metabolism, including transcription, alternative splicing, and RNA stability. Three recent studies report that TDP-43 binds to multiple RNA targets in the brain with a preference for UG-rich intronic regions (Polymenidou et al., 2011; Sephton et al., 2011; Tollervey et al., 2011). In an unbiased screen for modifiers of TDP-43 toxicity in yeast, the yeast ATXN2 homologue Pbp1 enhanced TDP-43 toxicity (Elden et al., 2010). Atx2 was also found to modify TDP-43 toxicity in Drosophila. In yeast and mammalian cells, TDP-43 and ATXN2 interact in a fashion dependent on RNA (Elden et al., 2010). Further linking ATXN2 with TDP-43 is their observation that ATXN2 is mislocalized in ALS motor neurons. Taking the functional relationship between ATXN2 and TDP-43 one step further, Elden et al. (2010) show that intermediate expansions (27–33 glutamines) are significantly higher in ALS patents than in neurologically normal controls. The association between longer wild-type SCA2 repeat alleles with an increased risk for ALS was recently supported by a study by Van Damme et al. (2011). This association is interesting in two respects. First, it indicates that ATXN2 is a relatively common susceptibility gene for ALS. In addition, this relationship between risk for ALS and intermediate alleles of ATXN2 suggests that variation in the polyQ tract, within the wild-type range, affects its function—perhaps through some aspect of RNA metabolism impacted by both ATXN2 and TDP-43.
SCA3 is considered to be the most common SCA worldwide including the United States. Also known as Machado-Joseph disease, SCA3 is caused by the expansion of a polyQ stretch in ataxin-3 (ATXN3; Kawaguchi et al., 1994). ATXN3 is associated with two cellular processes: transcription repression (Li et al., 2002; Evert et al., 2006) and protein homeostasis (Reina et al., 2010). It remains unclear whether these two processes are linked and the extent to which one or both drive SCA3 pathogenesis.
Supporting the nucleus as the site of pathogenesis in SCA3 are studies using cell (Tait et al., 1998; Chai et al., 1999; Perez et al., 1999; Fujigasaki et al., 2000) and mouse models (Bichelmeier et al., 2007), which show that ATXN3 is more toxic in the nucleus than in the cytoplasm. In addition, ATXN3 interacts with several transcription regulators including TAFII130 (Shimohata et al., 2000; Takahashi et al., 2001), CBP (McCampbell et al., 2000; Chai et al., 2002), RAD23 (Wang et al., 2000), and NCoR, HDAC3, and HDAC6 (Burnett and Pittman, 2005; Evert et al., 2006). More recently, heat shock and oxidative stress were found to increase the nuclear localization of wild-type and mutant ATXN3 (Reina et al., 2010). This observation raises an interesting question regarding the nuclear function of ATXN3; perhaps it functions to regulate expression of genes that encode components of the cellular stress response.
Besides modulating the cellular stress response by regulating gene expression, ATXN3 likely regulates the ubiquitin–proteasome system directly. Considerable data show that ATXN3 can function as a deubiqutinating enzyme (DUB; Burnett et al., 2003; Scheel et al., 2003; Winborn et al., 2008). ATXN3 contains at its N terminus a Josephin domain (JD) that has ubiquitin protease activity (Burnett et al., 2003; Scheel et al., 2003) and up to three ubiquitin-interacting motifs (UIMs) that bind ubiquitin (Burnett et al., 2003; Chai et al., 2004). The number of UIMs varies due to alternative splicing, with the three UIM isoforms predominating in the brain (Harris et al., 2010). Both the JD and UIMs of ATXN3 are critical for its ability in Drosophila to protect neurons from the toxicity of other mutant polyQ proteins (Warrick et al., 2005). ATXN3 selectively edits Lys63 linkages in mixed ubiquitin chains (Winborn et al., 2008). In contrast to the role of Lys48-linked chains in targeting proteins to the proteasome for degradation, Lys63-linked chains are thought to convey regulatory information to the proteins. Lastly, the three-dimensional structure of the JD from ATXN3 demonstrates a tight connection between polyubiquitin binding and the DUB activity of ATXN3 (Mao et al., 2005; Nicastro et al., 2005).
In a recent study, Scaglione et al. (2011) showed that ATXN3 along with the initiator E2 Ube2w regulates the ability of the E3 ligase C terminus of Hsc70-interacting protein (CHIP) to ubiquitinate its substrates. Monoubiquitination of CHIP by Ube2w promotes the interaction of CHIP with ATXN3, which in turn through its DUB activity restricts the length of ubiquitin chains attached to CHIP substrates. In addition, once substrate ubiquitination is completed ATXN3 deubquitinates CHIP, thereby stopping the reaction. In terms of the role this pathway might play in SCA3/MJD pathogenesis, Scaglione et al. (2011) found that polyQ expansion in ATXN3 increases its affinity for CHIP that could underlie the decreased activity of this neuroprotective E3 seen in a mouse model of SCA3.
Thus, a substantive body of data supports a role for ATXN3 in regulating the ubiquitin–proteasome system, most likely in editing polyubiquitin chains. It is worth noting that the ubiquitin–proteasome system, besides dealing with misfolded proteins, has a role in transcription by regulating the assembly and disassembly of transcription complexes that accompany each cycle of promoter activation/inactivation (Muratani and Tansey, 2003). As described above, nuclear localization of wild-type and mutant ATXN3 is increased by cellular stress. Thus, it is tempting to speculate that the nuclear and cytoplasmic functions of ATXN3 are subcellular variations on the same theme. Perhaps the ability of ATXN3 to remove monoubiquitin side chains from yet to be identified nuclear proteins—as it does with CHIP (Scaglione et al., 2011)—is key to proper ubiquitin-dependent regulation of gene expression in the nucleus. In this model, it is proposed that like its ability to regulate the Ube2w/CHIP ubiquitination cycle, ATXN3 associates with E2 ligases to regulate gene expression through its DUB activity to promote a ubiquitination/deubiquitination cycle on yet to be identified transcription factors. Analogous to the Ube2W/CHIP/ATXN3 ubiquitination cycle presented by Scaglione et al. (2011), ATXN3 might also regulate the ubiquitination of transcription factors critical for setting up a proper assembly/disassembly cycle of transcription complexes (Fig. 3). In this model, there are transcription factors that upon ubiquitination by an E2 ligase would promote the recruitment of ATXN3 to the transcriptional complex on DNA, thus stabilizing the complex and stimulating transcription. ATXN3 regulates the length of the ubiquitin side chain on the transcription factor, keeping it within a critical length. When transcription is to cease, a signal would induce ATXN3 to deubiquitinate the transcription factor as it does with CHIP (Scaglione et al., 2011), thereby destabilizing the complex.
Recent studies on the DUB activity of the ATXN3 orthologue in C. elegans, atx-3, speak to the biological relevance of its role in regulating the ubiquitin–proteasome system. ATXN3 interacts with the mammalian p97 protein, a chaperone-like AAA ATPase, to regulate the degradation of misfolded ER proteins (Wang et al., 2006). In C. elegans the p97 homologue is CDC-48. Worms deficient for both cdc-82 and atx-3 have increased protein stability and increased longevity (Kuhlbrodt et al., 2011). Thus, it seems that ATX-3 is a critical regulator of lifespan in worms. One can anticipate that as the chain-editing roles of ATXN3 are better defined in mammalian systems, its role in other physiologically relevant pathways will be forthcoming.
At first, pathogenesis of SCA6 seemed to be a relatively straightforward channelopathy. This disease is due to an expansion of a polyQ tract in the C terminus of the α1A transmembrane subunit of the P/Q-type voltage-gated calcium channel CACNA1A (Riess et al., 1997; Zhuchenko et al., 1997). This channel is known to be abundant in Purkinje cells of the cerebellum (Kulik et al., 2004) and is the mutational target in several other inherited neurological disorders (Pietrobon, 2002). Initial studies indicated that SCA6 was a disorder due to P/Q channel dysfunction (Matsuyama et al., 1999; Restituito et al., 2000; Toru et al., 2000).
However, two additional findings complicate the picture. First, electrophysiological analysis of Sca684Q knock-in mice failed to find a change in the intrinsic properties of Purkinje cells (Watase et al., 2008). Kordasiewicz et al. (2006), noting earlier evidence that the polyQ-containing cytoplasmic C terminus is cleaved to form a stable peptide (Sakurai et al., 1996; Kubodera et al., 2003), examined the α1A C terminus in more detail. Intriguingly, Kordasiewicz et al. (2006) found that the α1A C-terminal peptide localizes to Purkinje cell nuclei in wild-type mice and humans. Moreover, the C-terminal peptide with an expanded polyQ tract is toxic to tissue culture cells with toxicity being dependent on its nuclear localization. These results support a pathogenic model for SCA6 where cleavage of the polyQ-containing C terminus of the α1A transmembrane subunit and its subsequent translocation to the nucleus contributes to disease. More generally, these data suggest that like certain other membrane proteins involved in signaling, e.g., βAPP, p75, Notch, and the α1C subunit of L-type calcium channels (De Jongh et al., 1994; Bland et al., 2003; Jung et al., 2003), in response to a stimulus at the membrane, the C terminus of the α1A calcium channel subunit is cleaved and translocates to the nucleus to regulate transcription.
Nevertheless, in the absence of direct evidence that fragment production is critical for disease, one should be cautious in discarding SCA6 as a calcium channelopathy given the vast amount of data implicating altered calcium signaling in the SCAs. Evidence for alterations in calcium signaling and/or handling is reported for SCA1 (Lin et al., 2000; Vig et al., 2001; Serra et al., 2004), SCA2 (Liu et al., 2009), and SCA3 (Chen et al., 2008). In addition, recent data show that SCA15, a non-polyQ SCA, is due to a mutation in the InsP3 receptor 1 gene encoding a receptor that functions in the release of Ca2+ from intracellular stores (van de Leemput et al., 2007).
Besides progressive cerebellar degeneration, patients with SCA7 uniquely display retinal degeneration. ATXN7 functions as a component of the SAGA (Spt–Ada–Gcn5 acetyltransferase) complex (Helmlinger et al., 2006). SAGA regulates transcription via its two histone-modifying activities, the Gcn5 histone acetyltransferase and the Usp22 deubiquitinase. Although ATXN7 has no enzymatic activity it is reported to anchor the Usp22 component to the SAGA complex (Köhler et al., 2008; Zhao et al., 2008). It is the Gcn5 histone acetyltransferase (HAT) activity of SAGA that seems to be affected by the presence of ATXN7 with an expanded polyQ tract. Whether mutant ATXN7 decreases HAT activity (McMahon et al., 2005; Palhan et al., 2005) or increases HAT activity (Helmlinger et al., 2006) remains unclear. The reported increase in HAT activity with mutant ATXN7 is based on an in vivo analysis in the retina, whereas the studies showing a loss of activity either used human ATXN7 in yeast or transfected 293T cells. Perhaps differences between model systems and/or tissue underlie the discrepancies regarding the effect that mutant ATXN7 has on Gcn5 HAT activity. It is worth noting that a mutant ATXN5-induced gain in Gcn5 HAT activity is in line with the autosomal-dominant inheritance pattern of SCA7.
SCA17 exemplifies a paradox facing essentially all inherited neurodegenerative diseases: how can mutations in a widely expressed gene cause selective damage to the nervous system? In SCA17, polyQ expansion that occurs in the TATA-binding protein (TBP), an essential component in the initiation of transcription of all three RNA polymerases, causes a neurodegenerative disease that in addition to ataxia can include dementia and epilepsy (Koide et al., 1999; Rolfs et al., 2003). Importantly, individuals homozygous for mutant SCA17 alleles survive to adulthood, indicating that normal TBP function during development is not impaired by polyQ expansion (Zühlke et al., 2003; Toyoshima et al., 2004). In a series of studies using a transgenic mouse model of SCA17, Xioa-Jiang Li and colleagues found evidence indicating that polyQ expansion in TBP alters its ability to bind DNA and transcription regulators, perhaps leading to down-regulation of a select set of genes, e.g., HSPB1 and TrkA (Friedman et al., 2007, 2008; Shah et al., 2009). Thus, for SCA7 and SCA17, the implication is that polyQ expansion specifically impacts the ability of these regulators of transcription to control expression of a subset of genes—ones critical for neuronal function—while not impacting their ability to regulate most other genes.
To what extent might the cellular processes for the polyQ-mediated SCAs reflect molecular pathways shared among the inherited cerebellar ataxias in general? A framework for addressing this question comes from an ataxia protein–protein interaction network, “ataxia” interactome, developed by Lim et al. (2006). The interactome was generated by yeast two-hybrid screens using 23 ataxia-causing proteins, cDNAs of proteins for 11 recessive and 12 dominant ataxias including the polyQ SCAs, and 31 ataxia-associated proteins, cDNAs for proteins that either were known to interact with an ataxia-causing protein or paralogues of such proteins. The study showed that many of the ataxia-causing proteins share interacting partners, supporting the idea that the disease phenotypes shared among the ataxias are due to common molecular pathways. Biological processes significantly enriched in the ataxia network included transcription regulation, import of proteins to nucleus, RNA splicing, and ubiquitination. Correspondingly, cellular components containing proteins enriched in the ataxia interactome include the nucleoplasm, nuclear membrane, and spliceosome complex. Among the enhanced molecular functions are transcription factor activity and kinase inhibitors. The high degree of overlap in the cellular/molecular themes in ataxia interactome with those discussed in the previous paragraph indicate that as the pathogenesis of these disorders is further understood, understanding of the SCAs more broadly will be forthcoming.
Clearly for the polyQ SCAs there remains much to learn before a targeted approach to treatment, one based on correcting an altered function that drives pathology, is in sight. Yet, there are a couple of encouraging points worth noting. First, there is evidence that at least for SCA1 and two other polyQ disorders, Huntington’s disease and spinalbulbar muscular atrophy, pathology can be reversed even after disease is underway (Yamamoto et al., 2000; Chevalier-Larsen et al., 2004; Zu et al., 2004). In the case of SCA1, the data indicate that the ability to recover normal function decreases with age and progression of disease. This provides support for the widely held notion that the sooner one intervenes therapeutically, the better the chance of having a positive impact. The second key point is that for these SCAs, as well as other polyQ disorders, pathogenesis requires the presence of the mutant protein. Thus, decreasing the amount of mutant protein becomes a viable approach to therapy even in the absence of an understanding of the downstream effects that lead to disease.
One approach shown to be effective in reducing expression of mutant ATXN1 in vivo is the delivery to the cerebellum of AAV vectors expressing an shRNA directed against ATXN1 (Xia et al., 2004). Mutant ATXN1 expression was reduced such that motor function was significantly improved and Purkinje cell morphology was normalized in transduced cells. Although this SCA1 study used an shRNA that would target both wild-type and mutant ATXN1, allele-specific strategies where the mutant allele would be preferentially targeted are under development for several of the polyQ disorders including SCA3 (Alves et al., 2008). In this regard, selective targeting of the polyQ-expressing slice isoform of Cav2.1 should be applicable to SCA6 (Tsou et al., 2011).
That these diseases require expression of the mutant protein for disease to manifest itself has an additional implication in terms of a potential approach to therapy. The term proteostasis has been applied to the protein homeostatic network of cellular pathways that regulate the overall quality control of proteins that normally make up the proteome of each cell (Balch et al., 2008). There are numerous examples that the ability of this system to adapt to normal metabolic demands becomes compromised with aging and with the presence of misfolded mutant proteins such as those associated with many of the inherited neurodegenerative diseases (Voisine et al., 2010). For example, using a C. elegans model of Machado-Joseph disease (SCA3), the age-associated mutant ATXN3-induced phenotypes were suppressed by down-regulation of the Igf1-like pathway and activation of heat shock factor 1 (Teixeira-Castro et al., 2011). Such results provide support to the use of regulators of protein homeostasis as therapeutic agents in diseases like the polyglutamine ataxias.
The polyQ SCAs, as well as other inherited neurodegenerative diseases, are rich ground for investigation, one where cell biologists can make seminal contributions. The genes for these disorders are identified, yet how the proteins function normally and how this function is altered in disease remains to be established. Understanding the cell biology that underlies each affected protein and how it is altered in each disorder will be crucial for the development of therapeutic strategies. Furthermore, just as the study of genetic mutants in model organisms has made novel and fundamental contributions to basic cell biological processes, so can the study of inherited human neurodegenerative diseases such as the SCAs.
|Abbreviations used in this paper:|
|ALS||amyotrophic lateral sclerosis|
|CHIP||C terminus of Hsc70-interacting protein|
|NLS||nuclear localization sequence|
The author greatly appreciates the artistic talent of Jillian Frisch.
The research presented from the author was supported by National Institutes of Health/National Institute of Neurological Disorders and Stroke grants NS22920-23 and NS45667-09.
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[Figure ID: fig1]
An ATXN1 cellular pathway. ATXN1 is phosphorylated at S776 in the cytoplasm upon which it forms a complex with 14-3-3. Association with 14-3-3 blocks dephosphorylation of pS776 and transport of ATXN1 to the nucleus. Thus, nuclear transport of ATXN1 requires dissociation from 14-3-3, the regulation of which has yet to be determined. In the nucleus, ATXN1 is involved in alternative splicing by virtue of its interaction with RBM17 when phosphorylated on S776, or with U2AF65 after dephosphorylation of pS776. ↑[Q]n indicates that an increased interaction of expanded polyQ ATXN1 with RBM17 is hypothesized to be critical for driving disease in cerebellar Purkinje cells.
[Figure ID: fig2]
Proposed functions of ATXN2 in the regulation of mRNA translation. The SCA2-encoded protein, ATXN2, is thought to have a role in mRNA metabolism as a component of translating polysomes, cytoplasmic stress granules, P-bodies, and the miRNA pathway. One intriguing possibility would be for ATXN2 to function in the trafficking of RNA/RNPs between actively translating polysomes and inactive stress granules and P-bodies.
[Figure ID: fig3]
A model for ATXN3 in the editing of Ub chains on nuclear targets. The model combines the recent work of Scaglione et al. (2011) with earlier studies showing that ATXN3, a deubiquitinating enzyme, has a role in regulating gene expression. Like the proposed role of ATXN3 in the Ube2W/CHIP ubiquitination cycle of misfolded proteins, it is postulated that ATXN3 also regulates a ubiquitination cycle involved in assembly/disassembly of transcription complexes in the nucleus. ↑[Q]n indicates an increased interaction of expanded polyQ ATXN3 with a yet to be identified nuclear protein involved in regulation of transcription.
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