Adefective response to DNA damage is observed in several human autosomal recessive ataxias with oculomotor apraxia, including ataxia-telangiectasia. We report that senataxin, defective in ataxia oculomotor apraxia (AOA) type 2, is a nuclear protein involved in the DNA damage response. AOA2 cells are sensitive to H2O2, camptothecin, and mitomycin C, but not to ionizing radiation, and sensitivity was rescued with full-length SETX cDNA. AOA2 cells exhibited constitutive oxidative DNA damage and enhanced chromosomal instability in response to H2O2. Rejoining of H2O2-induced DNA double-strand breaks (DSBs) was significantly reduced in AOA2 cells compared to controls, and there was no evidence for a defect in DNA single-strand break repair. This defect in DSB repair was corrected by full-length SETX cDNA. These results provide evidence that an additional member of the autosomal recessive AOA is also characterized by a defective response to DNA damage, which may contribute to the neurodegeneration seen in this syndrome.
Ataxia-telangiectasia (A-T) represents a paradigm for several autosomal recessive ataxias characterized by defects in the recognition and/or repair of DNA damage (Lavin and Shiloh, 1997). The protein defective in A-T, A-T mutated (ATM), recognizes and is activated by DNA double-strand breaks (DSBs) to signal this damage to the cell cycle checkpoints and the DNA repair machinery (Kurz and Lees-Miller, 2004). Loss of ATM function results in hypersensitivity to ionizing radiation (IR), cell cycle checkpoint defects, genome instability, increased cancer incidence, and neurodegeneration (Hernandez et al., 1993). A-T–like disorder (A-TLD), as a result of hypomorphic mutations in the MRE11 gene, most closely resembles A-T in its clinical phenotype (Taylor et al., 2004). Mre11 functions in a complex with Rad50 and Nbs1 (defective in Nijmegen breakage syndrome) to localize to sites of DNA DSB. This complex acts upstream of ATM in sensing DSB and ensures efficient activation of ATM (Uziel et al., 2003; Cerosaletti and Concannon, 2004; Lee and Paull, 2005). Once activated, ATM phosphorylates a series of substrates, including Nbs1, which acts as an adaptor molecule for control of the intra-S and G2/M cell cycle checkpoints (Uziel et al., 2003). A third syndrome, ataxia oculomotor apraxia (AOA) type 1, also overlaps in its clinical phenotype with A-T (Aicardi et al., 1988; Le Ber et al., 2003). Mutations in the APTX gene are responsible for this neurological disorder (Date et al., 2001; Moreira et al., 2001). Recent evidence shows that the protein mutated in this syndrome, aprataxin, plays a role in the repair of DNA single-strand breaks (SSBs; Clements et al., 2004; Gueven et al., 2004; Mosesso et al., 2005), possibly by resolving abortive DNA ligation intermediates (Ahel et al., 2006).
A distinct form of AOA linked to chromosome 9q34, AOA2 also has an overlapping clinical phenotype with the three disorders described in the previous paragraph (Nemeth et al., 2000; Duquette et al., 2005; Le Ber et al., 2005). This syndrome is characterized by cerebellar atrophy, oculomotor apraxia, peripheral neuropathy, and elevated serum α-fetoprotein in some cases (Le Ber et al., 2005; Criscuolo et al., 2006). The gene defective in AOA2, SETX, was recently identified (Moreira et al., 2004). Mutations in SETX are also associated with an autosomal dominant, juvenile onset form of amyotrophic lateral sclerosis (Chen et al., 2004). Senataxin, the predicted protein encoded by SETX is 2,677 amino acids in length and contains a seven-motif domain at its C terminus, typical of the superfamily I of DNA/RNA helicases (Moreira et al., 2004). Senataxin has extensive homology to the Schizosaccharomyces pombe Sen1p proteins that possess helicase activity and are required for the processing of diverse RNA species that include transfer RNA, ribosomal RNA, small nuclear RNA, and small nucleolar RNA (Ursic et al., 1997). Sen1p proteins are also related to other DNA/RNA helicases, Upf1, involved in nonsense-mediated decay (Weng et al., 1996) and IGHMBP2, defective in a form of spinal muscular atrophy (Grohmann et al., 2001). Use of global and candidate-specific two-hybrid screens identified Rpo21p, a subunit of RNA polymerase II and Rnt1p, an endoribonuclease required for RNA maturation, as a Sen1p-interacting protein (Ursic et al., 2004), providing further support for a role in RNA processing. Recently, Steinmetz et al. (2006) showed that a single amino acid mutation that compromises Sen1 function in Saccharomyces cerevisiae altered the genome-wide distribution of RNA polymerase II, providing evidence for a role in transcription regulation. Interestingly, Sen1p was also shown to interact with Rad2p, a DNase required for nucleotide excision repair after DNA damage (Ursic et al., 2004). These observations on yeast orthologues, together with an overlapping phenotype with other autosomal recessive ataxias with oculomotor apraxia, which are characterized by defective DNA repair, led us to investigate whether senataxin might also play a role in the DNA damage response. We show here that senataxin is primarily a nuclear protein and that AOA2 cells have increased sensitivity to H2O2, camptothecin (CPT), and mitomycin C (MMC), but a normal response to IR, compared with controls. To determine whether senataxin was responsible for this cellular phenotype, we cloned full-length SETX cDNA and demonstrated complementation of agent sensitivity in stably transfected AOA2 cell lines. The increased sensitivity to H2O2 was associated with a defect in DNA DSB repair, but there was no defect in repair of SSBs or in DSBs produced by IR exposure. These results add further substance to the hypothesis that a defective DNA damage response contributes to the neurodegenerative phenotype in a subgroup of the autosomal recessive ataxias.
Detection and subcellular localization of senataxin
Cell lines were established from two patients with AOA2, fibroblasts (SETX-1RM) and a lymphoblastoid cell line (SETX-2RM). Identification of the mutations in SETX was performed by PCR followed by DNA sequencing. The results in Fig. S1 A show that for SETX-1RM, a homozygous deletion of 1 kb occurred at the cDNA level as a result of a large deletion in genomic DNA, which resulted in the deletion of exons 14–21 of SETX. Mutation in SETX was also homozygous for SETX-2RM, involving exon 23 skipping because of a missense mutation at the splice site (IVS 23 + 5 G > A; Fig. S1 B).
To detect the presence of senataxin protein and investigate its subcellular localization, we produced two polyclonal antibodies against the C-terminal (Ab-1/Ab-3) and another against the N-terminal (Ab-2) regions of the protein (Fig. S2 A). Specificity of the antibodies was determined by dot blot analysis (Fig. S2, B–E). The two C-terminal antibodies reacted only with a GST fusion protein corresponding to this C-terminal region of the molecule (senataxin GST-1), whereas the N-terminal antibody specifically recognized this region of the molecule (senataxin GST-2). Preimmune serum failed to detect senataxin GST. The results in Fig. 1 A show that Ab-l detected the presence of a single prominent band at ∼300 kD for two control cell lines (C2ABR and C3ABR), two AOA1 cell lines (L990 and L938), an unclassified AOA cell line (ATL2ABR) but was absent in an AOA2 cell line (SETX-2RM), as predicted from the exon-skipping mutation. The same pattern was observed with all three antibodies (unpublished data). Immunoprecipitation with Ab-1 followed by immunoblotting with the same antibody also detected a single band of the same size, which was again absent in the AOA2 cells (Fig. 1 B). Nonspecific antisera failed to immunoprecipitate senataxin. It was not possible to detect senataxin in primary fibroblasts with up to twofold increased protein loading by immunoblotting on total cell extracts (unpublished data). However, immunoprecipitation with Ab-1 followed by immunoblotting with two senataxin antibodies (Ab-1 and Ab-2) revealed the presence of senataxin in normal foreskin fibroblasts (NFFs; Fig. 1 C). This might be explained by a lesser amount present in the fibroblasts or a reduced relative amount of nuclear protein in fibroblasts compared with lymphoblasts. A slightly lower molecular size band for senataxin was detectable in an AOA2 fibroblast (SETX-1RM), consistent with the deletion of exons 14–21, which would maintain the reading frame but would lead to the loss of 322 amino acids (Fig. 1 C). Fractionation of cell extracts followed by immunoblotting with senataxin antibodies revealed that this protein was primarily a nuclear protein (Fig. 1 D). Senataxin was present in the cytoplasm but markedly reduced compared with that in the nucleus. It is notable that the amount of senataxin varied with cell type being highest in lymphoblastoid cells. Comparison of AOA2 (SETX-1RM) fibroblasts with NFFs (controls) using immunofluorescence demonstrated reduced nuclear staining in the AOA2 cells (Fig. 1 E). To confirm that the nuclear staining was specific, we performed competition experiments with antigen (senataxin GST-1) corresponding to a C-terminal peptide (Fig. 1 F). The results in Fig. 2 A confirm that senataxin, detected by both N- and C-terminal antibodies, is predominantly a nuclear protein and appears to be excluded from the nucleolus, as shown by a staining pattern similar to that of RNA polymerase II, a nucleoplasmic protein. Further support for this is provided by the failure of senataxin to colocalize with nucleolin in the nucleolus of NFFs or HeLa cells (Fig. 2 B). This was also the case for SETX-1RM fibroblasts, which contain a truncated form of senataxin. Finally, evidence that senataxin is predominantly a nucleoplasmic protein was provided by subcellular fractionation and immunoblotting (Fig. 2 C). Under these conditions, a prominent senataxin band was detected in the nucleoplasm but not in the nucleolus or cytoplasm. Immunoblotting for RNA polymerase II and nucleolin was performed to demonstrate the integrity of the cellular fractions (Fig. 2 C).
Sensitivity of AOA2 cells to DNA damaging agents and complementation of the defect
Because it has been demonstrated that cell lines from patients with other autosomal recessive ataxias, which overlap in their clinical phenotype with AOA2, are sensitive to DNA damaging agents, we determined whether this might also be the case for AOA2. The results in Fig. 3 A reveal that AOA2 lymphoblastoid cells (SETX-2RM) show a normal pattern of sensitivity to IR but have increased sensitivity to H2O2, CPT, and MMC, compared with controls. AOA1 cells are also sensitive to H2O2, as we have previously shown (Gueven et al., 2004). A-T cells showed normal sensitivity to these DNA damaging agents but hypersensitivity to IR. Increased sensitivity was also observed with H2O2, MMC, and CPT in AOA2 fibroblasts (Fig. 3 B). Although these agents give rise to either cross-links or SSBs and DSBs in DNA, there is also evidence that their toxicity is associated with redox-related pathways (Pagano et al., 2005). AOA1 fibroblasts were also sensitive to H2O2 (Fig. 3 B). As an additional measure of sensitivity, we compared the levels of H2O2-induced chromosome aberrations. The results in Fig. 3 C reveal approximately two induced chromosome aberrations per metaphase in H2O2-treated control cells, whereas a further twofold increase was observed in AOA2. To demonstrate that the increased sensitivity to H2O2 was due to loss of senataxin, we cloned full-length SETX cDNA into the Epstein-Barr virus–based expression vector pMEP4, containing a FLAG tag sequence, and established stable cell lines as previously described (Zhang et al., 1997). DNA sequencing detected five polymorphic changes in SETX and three nonconserved amino acid changes compared with the sequence in the database (available from GenBank/EMBL/DDBJ under accession no. AB014525). This construct, pSETX1, contains a metallothionein promoter, which allows inducible expression of senataxin by CdCl2. Induction of senataxin was detected by immunoprecipitation with anti-senataxin and anti-FLAG antibodies followed by immunoblotting with the respective antibodies (Fig. 4 A, right). Immunoblotting on total cell extracts confirmed that AOA2 (SETX-2RM) parental cells lack senataxin as compared with control cells (Fig. 4 A, left). Exposure of SETX-transfected AOA2 cells to H2O2 after induction of senataxin corrected the H2O2 hypersensitivity in these cells (Fig. 4 B). On the other hand, AOA2 cells transfected with empty vector remained hypersensitive to H2O2. SETX cDNA also corrected the H2O2-induced chromosome aberrations in AOA2 cells (Fig. 4 C), whereas vector alone did not change the number of aberrations.
Constitutive oxidative DNA damage in AOA2 cells
Because AOA2 cells were sensitive to H2O2, CPT, and MMC, all of which are capable of generating oxidative stress (Pagano et al., 2005), we investigated whether there might be an inherent defect in coping with oxidative damage in these cells. The presence of 8-oxo-deoxyguanosine (8-oxo-dG) was determined as a marker of reactive oxygen species–mediated DNA damage (Cooke et al., 2000). The results in Fig. 5 A reveal a high basal level of 8-oxo-dG in AOA2 fibroblasts (SETX-1RM), but not in controls (NFFs). Quantitation of 8-oxo-dG fluorescence intensity reveals an approximately twofold increase in AOA2 cells compared with controls (Fig. 5 B). Exposure of cells to H2O2 caused an increase in 8-oxo-dG in both controls and AOA2, but the extent of staining remained higher in the AOA2 cells (Fig. 5, A and B). To determine whether this represented more general oxidative damage in AOA2 cells or a defect at the level of DNA, we also assayed for protein nitrotyrosination and lipid peroxidation. The results showed background levels for both 3-nitrotyrosine and 4HNE-Michael adducts in AOA2 cells similar to those observed in normal fibroblasts, suggesting that these cells were not undergoing generalized oxidative stress (Fig. 5, C and D).
Repair of oxidative damage to DNA
Given that AOA2 cells were sensitive to agents that cause oxidative stress, and because these cells had evidence of constitutive oxidative DNA damage, we investigated their DNA repair capacity. For DNA SSB repair, we used alkaline elution analysis. Using this assay, we failed to observe any difference between control and AOA2 cells over a time course of 1-h repair (Fig. 6 A). These results were confirmed by determining intracellular NAD(P)H levels, which represents a reliable method to monitor imbalance in break repair in cells (Nakamura et al., 2003). Again, in this case, there was no evidence for a defect in the extent or duration of DNA single-strand breakage (Fig. 6 B).
H2O2 is also capable of inducing DSBs in DNA (Dahm-Daphi et al., 2000). To detect DSBs arising in DNA as a result of oxidative damage and eliminate those that occur as a consequence of DNA replication fork movement across a site of damage, cells were grown to confluency. DNA DSBs were detected by measuring H2AX phosphorylation visualized as foci at sites of DNA damage, a quantitative assessment for the appearance and repair of DNA DSBs (Rothkamm and Lobrich, 2003). Approximately equal numbers of γH2AX foci were detected in control and AOA2 cells between 10 and 50 min after treatment with H2O2 (Fig. S3), and in both cases, these foci coincided with MDC1 foci, further supporting that they were sites of DNA DSB (Fig. 7 A). However, the extent of disappearance of these foci appeared to be slower in AOA2 cells at 8 h after treatment than in controls (Fig. 7 A). Quantitation of these results showed that there was a significant difference between AOA2 and controls at 4, 6, and 8 h after treatment. By 8 h after treatment, 10% of the foci remained in control nuclei compared with 39% in AOA2 cells, indicating a defect in repair of DSBs (Fig. 8 A). To determine whether this was a general defect in repair of DSBs, cells were exposed to IR, and the rate of disappearance of γH2AX foci was measured (Fig. 7 B). No difference in the rate of DSB repair after IR was observed (Fig. 8 B). The reduced capacity of AOA2 cells to repair the DSB induced by H2O2 does not appear to be explained by a trivial reason, such as widespread oxidative damage to proteins after incubation with H2O2 in the form of nitrotyrosinated proteins, as there was no evidence of gross damage (Fig. 5 C). To investigate further whether senataxin played a direct role in the DNA damage response, we performed transient transfections of AOA2 cells with SETX-GFP cDNA and assayed for correction of the DNA DSB defect after H2O2 treatment. Use of the SETX-GFP construct allowed us to differentiate between transfected and untransfected cells, providing an internal control for scoring of γH2AX foci. The results in Fig. S4 A reveal that the number of γH2AX foci are comparable in unlabeled and GFP-labeled cells. However, by 8 h after treatment, the number of γH2AX foci in GFP-labeled cells is significantly lower than that of γH2AX foci in nontransfected cells (Fig. S4 B). Similar experiments in transfected control fibroblasts revealed that the number of γH2AX foci was the same in unlabeled and GFP-labeled cells at 30 min after treatment with H2O2, and both cell types efficiently repaired the DNA DSBs by 8 h (Fig. S4, C and D). Foci were counted in at least 50 GFP-transfected and unlabeled cells and quantitated to reveal that SETX-cDNA corrected the DSB defect in AOA2 cells. These data appear in Fig. 8 A, indicating that full-length cDNA corrects the DNA DSB defect in AOA2 cells.
Antibodies directed against both extremities of senataxin detected a protein of ∼300 kD, the predicted size from the reported open reading frame (Moreira et al., 2004). This protein was not detected in AOA2 lymphoblastoid cells with a mutation in SETX predicted to give rise to a prematurely truncated protein, but was detected as a lower molecular size form in fibroblasts (SETX-1RM) where an in-frame deletion was observed. We also provided firm evidence that senataxin is a nuclear protein with only minimal amounts in the cytoplasm. This protein is diffusely distributed throughout the nucleus with no evidence of localization to any subnuclear compartments. This is in contrast to a recent report demonstrating that senataxin was diffusely present in the cytoplasm and in the nucleolus in cultured cells (Chen et al., 2006). These data suggested that senataxin was expressed strongly in the cytoplasm in primate deep cerebellar nucleus but dull and diffuse in the nucleus. Using three different antibodies directed against both termini of senataxin, we showed diffuse nuclear labeling by immunofluoresence, which is supported by immunoblotting, revealing predominantly nuclear localization of the protein. We did not detect any senataxin in the nucleolus using either immunofluoresence or subcellular fractionation. It is of interest that Chen et al. (2006), using an N-terminal FLAG-tagged SETX construct, demonstrated only strong immunoreactivity throughout the nucleoplasm with an anti-FLAG antibody, in contrast to the results obtained with their anti-senataxin antibody. The authors interpreted this to mean that FLAG-senataxin is mislocalized. On the contrary, our data suggest that this is the correct localization.
Similar to that observed in A-T, A-TLD, and AOA1 cells, AOA2 cells are also characterized by sensitivity to DNA damaging agents. A-T cells are hypersensitive to IR and radiomimetic agents that give rise to DSBs in DNA (Taylor et al., 1975; Chen et al., 1978). A-TLD cells are also sensitive to these agents but not to the same extent as A-T (Stewart et al., 1999). The pattern of sensitivity described for AOA1 cells overlaps with that reported here for AOA2 (Gueven et al., 2004; Mosesso et al., 2005). Both cell types show increased sensitivity to H2O2, CPT, and MMC, but are not sensitive to IR. All three agents to which AOA2 cells are sensitive can give rise to DNA SSBs, but we found no evidence for a defect in SSB repair in AOA2. On the other hand, there is some evidence that AOA1 cells have a defect in SSB repair (Mosesso et al., 2005; Gueven et al., 2007), which is compatible with a role for aprataxin in resolving abortive DNA ligation intermediates (Ahel et al., 2006). Thus, the basis for the sensitivity to these agents appears to differ in AOA1 and AOA2 cells. The toxicity of these agents (MMC, CPT, and H2O2) is also associated with redox-related pathways (Pagano et al., 2005). A common observation in neurodegenerative disorders associated with DNA repair/signaling defects is an increase of spontaneous oxidative damages (Hayashi et al., 2001; Barzilai et al., 2002). Investigation of oxidative stress markers in AOA2 cells revealed higher basal levels of oxidative DNA damage (8-oxo-dG) compared with controls, suggesting a reduced capacity to repair this type of DNA lesion (Hoffmann et al., 2004). This is further supported by a failure to observe more general oxidative damage in these cells.
At a higher concentration, H2O2-induced DSBs are also detected in DNA, as determined by the formation of γH2AX foci (Chen et al., 2005). They described the appearance of γH2AX foci in H2O2-treated cells after 2 h, which gradually decreased over 24 h. Coincidence was demonstrated between γH2AX and 53BP1 foci, providing additional evidence that these were DNA DSBs. In this study, we revealed a coincidence between γH2AX and MDC1 foci, a γH2AX-interacting protein that bridges the binding of the DNA damage response machinery to sites of DNA breaks (Stucki and Jackson, 2006). In the present study, these foci occurred to the same extent in both control and AOA2 cells in response to H2O2 treatment. However, the rate of loss of γH2AX foci was significantly reduced in AOA2 cells compared with controls from 4–8 h after treatment. The presence of high constitutive levels of 8-oxo-dG in AOA2 cells did not affect the number of breaks introduced into DNA by H2O2, but it is possible that these lesions might interfere with the rate of repair of the DSBs. An alternative but less likely explanation for the persistence of γH2AX foci in AOA2 cells is that these foci are indicative of aberrant chromatin structure by inappropriate rejoining of DNA breaks. Suzuki et al. (2006) provided this as an explanation to account for the persistence of γH2AX foci at a time when all the breaks were repaired on mitotic chromosomes. The defect in repair to DSBs was not a general one because AOA2 cells were as efficient as controls in repairing breaks induced by IR. These results suggest that the nature of the breaks is different after H2O2 and IR exposure. DNA damage caused by oxidation is complex and is deposited along the DNA molecule as single alterations or in clusters termed multiple DNA damage sites (Letavayova et al., 2006). This damage is primarily oxidized base damage and, when present at close proximity on opposite strands, can give rise to abortive base excision repair that leads to the formation of DNA DSBs (Wallace, 2002). What distinguishes a DSB resulting from IR or H2O2 treatment? There is no easy answer to this, but it is evident that a DNA DSB arising from IR is efficient in attracting the Mre11 complex, activating ATM and the components of DNA repair (Bakkenist and Kastan, 2003; Kozlov et al., 2006). On the other hand, H2O2 is less efficient in activating ATM (Ismail et al., 2005; unpublished data). Furthermore, PDGFβ receptor transactivation acts as an upstream mediator of ATM kinase stimulation in response to H2O2 and, under these conditions, p53 is phosphorylated only on Ser15 (Chen et al., 2003). These data suggest that the mechanism of activation of ATM by IR and H2O2 are different and provide support for a difference in the nature of the DNA DSB generated in each case. Further support for a difference in the nature of the damage inflicted by H2O2 and IR is demonstrated by a lack of correlation in sensitivity to these agents in different cell lines (Cantoni et al., 1989; Bouzyk et al., 2000; Gueven et al., 2004) and difference in mutagenesis capacity (Gustafson et al., 2000) and in their effects on cell cycle progression (Wharton, 1995). Thus, it is not inconceivable that senataxin plays a specific role only in the processing of breaks generated by oxidative DNA damage.
It appears from the shape of the DNA repair curve that the initial rate of removal of breaks is comparable in control and AOA2 and that the defect is in a slower component of repair. This could be explained by a defect in repairing a subgroup of DNA breaks arising as a consequence of oxidative damage. 8 h after treatment with H2O2, 10% of breaks remained unrepaired in control cells, whereas almost four times as many (39%) were still detected in AOA2 cells. The subgroup of breaks may relate to double-strand ends with damaged termini. Although it is likely that ·OH generated from H2O2 is responsible for much of the damage, there is also evidence for metal-mediated DNA damage, which is not protected against with hydroxyl radical scavengers (Li et al., 1999). Although Artemis-dependent processing of a subgroup of DNA breaks in response to radiation damage has been reported (Riballo et al., 2004), it is unlikely that the involvement of senataxin is in the ATM–Artemis pathway because DSBs induced by IR are normally repaired in AOA2.
The predicted protein sequence of senataxin contains a seven-helicase motif near its C terminus related to that present in the helicase superfamilies I and II (Gorbalenya et al., 1989), which play essential roles in maintaining genome integrity through their involvement in DNA replication, transcription, recombination, and repair (Hickson, 2003). Two members of the RecQ helicase family, WRN and RECQL4, mutated in Werner syndrome and Rothmund-Thompson syndrome, respectively, also protect against oxidative DNA damage (Szekely et al., 2005; Werner et al., 2006). The increased sensitivity to agents that cause oxidative stress and the reduced DSB repair in response to H2O2 exposure in AOA2 cells might also be explained by a defect in a helicase. However, although senataxin is an orthologue of yeast DNA/RNA helicases, no such activity has yet been demonstrated for this protein. A recent report by Steinmetz et al. (2006) showed that the yeast Sen1 helicase controlled the genome-wide distribution of RNA polymerase II, and a mutation that affected the function of this helicase led to profound changes in polymerase II distribution over noncoding and protein-coding genes, suggesting that Sen1 has an important role in control of gene expression. Given the similarity between the yeast and human Sen1 proteins, they suggested that mutations in senataxin may also lead to misregulation of transcription and in turn account for the progressive neurological defect in this syndrome. If it were to emerge that senataxin plays a similar role to yeast Sen1 in mammalian cells, it is not immediately evident how the transcriptional misregulation might account for some of the cellular characteristics that are described here for AOA2. Mouse cells lacking the WRN helicase exhibit altered expression of genes responding to oxidative stress (Deschenes et al., 2005). Furthermore, combining the defect with abrogation of the DNA repair gene poly (ADP-ribose) polymerase-1 (PARP-1) increased the extent of misregulation of gene expression. Aberrant transcription, chronic cellular stress, and apoptosis have also been suggested to contribute to the phenotype in Alzheimer's disease (Toiber and Soreq, 2005). The appearance of oxidative stress in AOA2 as described here could thus be explained by misregulation of transcription. Failure to respond normally to DNA damage and repair DSBs arising as a result of oxidative DNA damage might also be explained by the down-regulation of specific genes that are important for this process. Alternatively, as senataxin is a large protein characterized by only one putative helicase domain, it is possible that it has other activities or controls other proteins through interaction. Being able to reconcile the AOA2 cellular characteristics described here with a possible defect in regulation of gene expression requires a greater understanding of the functioning of this protein.
Materials And Methods
Cell lines, survival, and induced chromosome aberrations
Lymphoblastoid cell lines (LCLs) from control (C3ABR and C2ABR), AOA1 (L938 and L939), Friedrich's ataxia (FRDA1), and AOA2 (SETX-2RM) patients were cultured in RPMI 1640 medium (Invitrogen) containing 10% FCS (JRH Biosciences), 2 mM l-glutamine (Life Technologies), 100 U/ml penicillin (Invitrogen), and 100 U/ml streptomycin (Invitrogen), and maintained in a humidified incubator at 37°C/5% CO2. Fibroblasts from an AOA2 patient (SETX-1RM), NFFs (a gift from P. Parsons, Queensland Institute of Medical Research, Queensland, Australia), and HeLa were cultured in DME medium (Invitrogen) containing 10% FCS. LCLs were used at a density of 1 × 106 cells/ml, and adherent cells were used at 75% confluency except in the case of γH2AX foci experiments, where confluent cells were used. MMC, CPT, and H2O2 were purchased from Sigma-Aldrich. Irradiations were performed at room temperature using a 137Cs source (Gammacell 40 Exactor [MDS Nordion]; dose rate 1.1 Gy/min). Lymphoblastoid cell viability (triplicate wells for each drug concentration) was measured by adding 0.1 ml of 0.4% trypan blue to 0.5 ml of cell suspension. The number of viable cells was counted, and viabilities were expressed as the number of cells in drug-treated wells relative to cells in untreated wells (percentage of viable cells), as previously described (Chen et al., 1978). The cells were incubated with the genotoxic agents for 1 h (MMC), 3 h (CPT), and 30 min (H2O2) before washing twice with PBS and suspension in culture medium. The number of viable cells was counted daily up to 4 d after treatment, and viability was calculated as described. The conditions were the same for fibroblasts, but survival was determined by colony formation. Cells were left for 2–3 wk to form colonies before staining with methylene blue and counting. Chromosomal aberrations were determined by treating cells with 2 mM H2O2 for 30 min in media under aerobic conditions. Colcemid (final concentration 0.1 μg/ml) was added immediately after treatment, 2 h before harvesting. The cells were treated for 15 min in 0.0075 M KCl and fixed in methanol ± glacial acetic acid (3:1), and the fixed cells were spread onto glass slides, air-dried, and stained with Giemsa. 50 metaphases were analyzed for each sample.
Cloning and expression of senataxin antigens
To produce senataxin antibodies, two regions of SETX were PCR amplified and cloned into bacterial expression vectors. In brief, a region of 450 bp of human SETX cDNA was PCR amplified from the 3′ end of senataxin using Ab-1F/Ab-1R primer pair. This SETX fragment was subsequently cloned into NheI and NotI sites of pTYB1 plasmid (New England Biolabs, Inc.), containing a C-terminal chitin binding domain. A second region of 1.1 kb of SETX was PCR amplified from the 5′ end of senataxin using Ab-2F/Ab-2R primer pair. The 5′ SETX fragment was cloned into EcoRI and NotI sites of pGEX-5X-1 plasmid (GE Healthcare), containing an N-terminal GST tag. Both of these constructs were transformed into Escherichia coli BL21 (DE3) pLysE cells, and overexpression was induced using 0.3 mM IPTG.
Production and purification of anti-senataxin antibodies
To produce senataxin antibodies, two regions of SETX corresponding to the N and C termini of the protein were PCR amplified, cloned into bacterial expression vectors, and transformed into E. coli (BL21 [DE3] pLysE). N- and C-terminal fusion proteins were affinity purified using chitin beads and glutathione–Sepharose resin, respectively, using the manufacturer's protocol. Sheep or rabbits were inoculated with senataxin antigens, and polyclonal antibodies were generated against the C (Ab-1/Ab-3) and N termini (Ab-2) of human senataxin using methods described previously (Bar-Peled and Raikhel, 1996). Senataxin antibodies were affinity purified using a series of GST-only and GST-N-ter/GST-C-ter columns.
Cloning of full-length SETX cDNA
Full-length SETX was PCR amplified and cloned into KpnI–NotI digested pMEP4 (see the supplemental text). For complementation studies, expression of senataxin was induced or mock-induced from pMEP4-transfected cells with 5 μM CdCl2. SETX was also cloned into pEGFP-C2 by applying full-length SETX cDNA from pSPORT1_Sfi (RZPD Deutsches Ressourcenzentrum). SETX-GFP was used in transient transfection experiments.
PCR primers were designed to amplify two SETX fragments overlapping a unique SphI restriction site located at position 4432. Primer pairs HEF1/HER2 amplified a 5′ region from 1 to 4,375 bp and HEF3/HER3 amplified a 3′ region from 4,131 to 8,038 bp. PCR amplification was performed with 100 ng C3ABR cDNA, 1 μg of each primer, 100 μM dNTP, 1 × buffer 3, and 5 U Taq (Expand high fidelity Taq; Roche). Thermal cycling was performed in a PE-9700 PCR machine with the following settings: 95°C for 2 min, 30 cycles of 95°C for 30 s, 65°C for 30 s, and 6 min at 72°C. After amplification, DNA were purified on agarose gels. PCR fragments were subsequently A-tailed and cloned into pGEM-T-Vector (Promega). The 4-kb 3′ senataxin fragment was excised with SphI and SphI (pGEM-T vector site) and cloned into the 5′ SphI–SphI (pGEM-T vector site) restriction sites. After screening for correct orientation, the resulting full-length SETX cDNA clone was called pSETX. For expression of senataxin, the full-length senataxin cDNA was amplified from pSETX with Pfu Turbot Taq (Stratagene) using HEF5/HER5 primer pair, and the resulting product was cloned into KpnI–NotI digested pMEP4. The resulting pMEP4-SETX construct is referred to as pSETX1.
Detection of 8-oxo-dG by immunofluorescence
Cells on coverslips were fixed with 100% prechilled methanol for 5 min and immersed in 100% prechilled acetone for 5 min. Coverslips were subsequently air-dried, treated with 0.05 N HCl for 5 min on ice, and washed three times with PBS. RNA was digested by incubating the coverslips in 100 μg/ml RNase in 150 mM NaCl with 15 mM sodium citrate for 1 h at 37°C. After RNA digestion, coverslips were sequentially washed in PBS, 35, 50, and 75% ethanol for 2 min each. DNA was denatured by incubating the coverslips with 0.15 N NaOH in 70% ethanol for 4 min. A series of washes was performed starting with 70% ethanol containing 4% vol/vol formaldehyde and then 50% ethanol, 35% ethanol, and finally PBS for 2 min each. Proteins were digested with 5 μg/ml proteinase K in TE, pH 7.5, for 10 min at 37°C. After several PBS washes, coverslips were incubated with anti-8-oxo-dG antibody (1:250; 4355-MC-100 [Trevigen]) in PBT20 (1× PBS/1% BSA/0.1% Tween 20) for 1 h at room temperature. After several washes with 0.1× PBS, 8-oxo-dG was detected using an Alexa Fluor 488 secondary antibody (1:500 in PBT20; Invitrogen). Nuclei were counterstained with DAPI, and slides were mounted for immunofluorescence.
Cellular fractionation, immunoprecipitation, and immunoblotting
Cells were separated into cytoplasmic, nucleoplasmic, and nucleolar fractions as previously described (Scherl et al., 2002). For immunoprecipitations, cells were washed in PBS and resuspended in lysis buffer (50 mM Tris-HCl, pH 7.5, 50 mM β-glycerophosphate, 150 mM NaCl, 10% glycerol, and 1% Tween 20, supplemented with protease and phosphatase inhibitors) for 1 h at 4°C. Insoluble components were removed by centrifugation at 16,000 g for 20 min at 4°C. For immunoprecipitations, 1 mg of total cell extract was precleared with 30 μl of protein G–Sepharose beads (GE Healthcare) for 3 h at 4°C. Senataxin was immunoprecipitated with 7.5 μg senataxin Ab-1 antibody overnight at 4°C. The following day, 40 μl of protein G–Sepharose beads was added for 1 h and incubated at 4°C. Immunoprecipitates were washed three times with lysis buffer and resuspended in 20 μl of sample loading buffer before separation of the proteins by SDS-PAGE. The proteins were then transferred onto a nitrocellulose membrane (Pall Life Sciences), and immunoblots were performed with the relevant antibodies.
NFFs, AOA2 (SETX-1RM) fibroblasts, and HeLa were grown on glass coverslips for 48 h, washed with PBS, fixed in 2% paraformaldehyde/PBS for 10 min, and processed for immunofluorescence as previously described (Becherel et al., 2006) using the relevant antibodies, senataxin Ab-3 (1:400) and Ab-2 (1:200), RNA polymerase II (1:400; ab5408 [Abcam]), nucleolin (1:500; M019-3 [MBL International Corporation]), 3-nitrotyrosine (1:100; 9691 [Cell Signaling Technology]), 4-HNE-Michael adducts (1:100; 393207 [Calbiochem]). 8-oxo-dG was detected according to the manufacturer's protocol. Fluorochromes conjugated to the relevant secondary antibodies were Alexa Fluor 488 and 594 (Invitrogen). Images were captured using a digital camera (AxioCam MRm; Carl Zeiss MicroImaging, Inc.) attached to a fluorescent microscope (Axioskop2 mot plus; Carl Zeiss MicroImaging, Inc.) using Plan Apochromat 1.4 oil differential interference contrast (63× magnification). Imaging medium was PBS, and acquisition was performed at ambient temperature (25°C). AxioVision LE 4.3 software (Carl Zeiss MicroImaging, Inc.) was used to capture the individual images, which were assembled using Photoshop 7.0 (Adobe). Fluorescence intensity was quantitated on the RAW images using the public domain software ImageJ version 1.34s (NIH) before their assembly in Photoshop 7.0. After assembly, contrast was enhanced on all images simultaneously in Photoshop 7.0 using the brightness and contrast tool. No further image processing (e.g., surface or volume rendering, γ adjustment) was performed.
Analysis of DNA SSB repair
To induce SSB, cells were exposed to 20 μM H2O2 in RPMI 1640 medium without supplements for 15 min at 37°C. To remove H2O2, 880 U/ml catalase was added. Cells were collected by centrifugation (1,500 U/min for 5 min) and washed with PBSCMF (140 mM NaCl, 3 mM KCl, 8 mM Na2HPO4, and 1 mM KH2PO4). The numbers of SSBs were determined by an alkaline elution assay as previously described (Epe and Hegler, 1994). The numbers of SSBs in untreated control cells were subtracted in all cases. NAD(P)H depletion after H2O2 and MMS treatments was performed as previously described (Nakamura et al., 2003).
Repair kinetics of γH2AX foci
Cells were seeded onto coverslips, and experiments were performed on confluent fibroblasts. Cells were either irradiated or treated with H2O2 by adding 2 mM H2O2 into the growth medium for 10 or 30 min. Cells were washed with PBS and returned to fresh media. At the time points indicated, the cells were processed for immunofluorescence as described. Images were captured and assembled as described.
Online supplemental material
Fig. S1 shows characterization of mutations in two AOA2 cell lines. Fig. S2 shows characterization of senataxin antibodies. Fig. S3 shows induction of γH2AX foci in control (NFF) and AOA2 (SETX-1RM) cells after exposure to 2 mM H2O2. Fig. S4 shows complementation of the DNA DSB repair defect in AOA2 cells. The supplemental text gives primers used in this study.
We thank Aine Farrell for excellent cell culture assistance and Peter Parsons for the NFF strain.
This work is supported by the Australian National Health and Medical Research Council.
The authors declare that they have no conflict of interest.
A. Suraweera and O.J. Becherel contributed equally to this paper.
Abbreviations used in this paper: AOA, ataxia oculomotor apraxia; A-T; ataxia-telangiectasia; A-TLD, A-T–like disorder; ATM, A-T mutated; CPT, camptothecin; DSB, double-strand break; IR, ionizing radiation; MMC, mitomycin C; NFF, normal foreskin fibroblast; SSB, single-strand break.