The SMC5/6 complex is the least understood of SMC complexes. In yeast, smc5/6 mutants phenocopy mutations in sgs1, the BLM ortholog that is deficient in Bloom's syndrome (BS). We here show that NSMCE2 (Mms21, in Saccharomyces cerevisiae), an essential SUMO ligase of the SMC5/6 complex, suppresses cancer and aging in mice. Surprisingly, a mutation that compromises NSMCE2‐dependent SUMOylation does not have a detectable impact on murine lifespan. In contrast, NSMCE2 deletion in adult mice leads to pathologies resembling those found in patients of BS. Moreover, and whereas NSMCE2 deletion does not have a detectable impact on DNA replication, NSMCE2‐deficient cells also present the cellular hallmarks of BS such as increased recombination rates and an accumulation of micronuclei. Despite the similarities, NSMCE2 and BLM foci do not colocalize and concomitant deletion of Blm and Nsmce2 in B lymphocytes further increases recombination rates and is synthetic lethal due to severe chromosome mis‐segregation. Our work reveals that SUMO‐ and BLM‐independent activities of NSMCE2 limit recombination and facilitate segregation; functions of the SMC5/6 complex that are necessary to prevent cancer and aging in mice.
The conserved Structural Maintenance of Chromosomes (SMC) complex SMC5/6 maintains genome stability and contains a subunit with SUMO E3 ligase activity, NSMCE2/MMS21. Characterization of mutant mice reveals that NSMCE2 limits cancer and aging, but that its SUMO ligase activity is largely dispensable in mice.
NSMCE2 deficiency promotes cancer and aging in mice.
NSMCE2‐deficient cells undergo normal DNA replication.
Lack of NSMCE2 leads to cellular and animal phenotypes reminiscent of Bloom's Syndrome.
Bloom's Syndrome helicase BLM and NSMCE2 independently suppress recombination and chromosome missegregation.
Mutant NSMCE2 lacking only SUMO ligase activity has no overt effects on murine development or lifespan.
The structural maintenance of chromosome (SMC) complexes play key roles in chromosome architecture and dynamics (Losada & Hirano, 2005; Nasmyth & Haering, 2005). SMC proteins contain globular N‐ and C‐terminal ATPase domains (Walker boxes), which are linked through two long α‐helixes folded against each other at a hinge domain. Bacteria present a single SMC protein, and six can be identified in eukaryotes. These six proteins are arranged in three independent heterodimeric complexes named SMC1/3 (cohesin), SMC2/4 (condensin), and SMC5/6. Whereas the functions of cohesin and condensin in chromosome structure are well established, what the SMC5/6 complex does is still a matter of debate (Murray & Carr, 2008; De Piccoli et al, 2009; Stephan et al, 2011b).
The SMC5/6 complex was initially identified in fission yeast as a heterodimer of Rad18 and Spr18 proteins that presented the architecture of SMC proteins (Lehmann et al, 1995; Fousteri & Lehmann, 2000). Human orthologs were subsequently identified and were shown to be particularly abundant during meiosis (Fousteri & Lehmann, 2000). The complex contains six additional polypeptides named non‐SMC elements (NSMCE) 1–6 (McDonald et al, 2003; Pebernard et al, 2004; Sergeant et al, 2005), although only four (NSMCE1‐4) have been identified in mammals (Taylor et al, 2008). Besides the ATPase activity of SMC5 and SMC6, 2 additional activities are found in the complex. NSMCE1 presents an E3 ubiquitin (UQ) ligase activity that is only detectable upon interaction with NSMCE3 (Pebernard et al, 2008a; Doyle et al, 2010). In addition, NSMCE2 has a C‐terminal Siz/PIAS‐RING (SP‐RING) domain with E3 SUMO ligase activity (Andrews et al, 2005; Potts & Yu, 2005; Zhao & Blobel, 2005). The last component found in mammals, NSMCE4, is the kleisin subunit that bridges SMC5 and SMC6 (Morikawa et al, 2004; Palecek et al, 2006). To date, and due to the viability of catalytically dead mutants, many of the studies on the SMC5/6 complex have focused on the SUMO ligase activity of NSMCE2.
The consensus is that the SMC5/6 complex is involved in genome maintenance, consistent with the original rad18 (Smc5) and mms21 (Nsmce2) mutants being isolated on the basis of sensitivity to genotoxic agents (Nasim & Smith, 1975; Prakash & Prakash, 1977). Mutations or RNAi studies for SMC5/6 have further confirmed sensitivity to genotoxic agents in plants, chicken, and human cells (reviewed in Stephan et al, 2011b). Still, the actual role of this complex in preventing DNA damage is not well defined. On one hand, the complex has been proposed to promote homologous recombination (HR). Accordingly, RNAi studies in human cells reported lower rates of sister chromatid exchanges (SCE) in NSMCE2‐depleted cells (Potts et al, 2006; Wu et al, 2012). The same group also reported reduced rates of telomere recombination (T‐SCE) upon SMC5/6 knockdown (Potts & Yu, 2007). On the other hand, these results are at odds with the fact that mutants of the SMC5/6 complex display increased recombination rates in every model organism tested. In fact, the mms21 mutant was first isolated in yeast for presenting a 23‐fold increase in mitotic recombination (Prakash & Prakash, 1977). Likewise, Nsmce2 or Smc5 knockouts in chicken (Stephan et al, 2011a; Kliszczak et al, 2012) and reduced levels of SMC6 in mice (Ju et al, 2013) all led to increased rates of SCE. To what extent these effects reflect species‐specific roles or technical differences remains to be solved.
Despite a role in HR, this cannot account for all SMC5/6 functions. All components of the SMC5/6 complex are essential in Saccharomyces cerevisiae (Zhao & Blobel, 2005), whereas HR is not. The essential role of SMC5/6 might relate to defects in chromosome segregation (Torres‐Rosell et al, 2005). These problems could derive from persistent DNA (Torres‐Rosell et al, 2005; Branzei et al, 2006; Bermudez‐Lopez et al, 2010) or protein (Outwin et al, 2009) links between sister chromatids during mitosis. Accordingly, yeast lacking SMC5/6 undergo catastrophic meiosis due to unresolved inter‐chromosome links (Farmer et al, 2011). Noteworthy, this role of SMC5/6 on the dissolution of joint DNA molecules (JM) is analogous to the one carried by Sgs1, the yeast ortholog of the BLM protein that is deficient in patients of the Bloom syndrome (OMIM 210900). BLM is one of the five helicases from the RecQ family, three of which (BLM, WRN, and RECQL4) are associated with cancer predisposition and premature aging in human hereditary disorders (Chu & Hickson, 2009). Similar to yeast smc5/6 mutants, BLM‐deficient human cells also present segregation problems due to anaphase bridges between unresolved chromatids (Chan et al, 2007, 2009; Naim & Rosselli, 2009). To what extent the similarities between the SMC5/6 complex and BLM are also present at the organism level remains unknown.
To explore the physiological roles of the SMC5/6 complex in mammals, we developed three independent murine alleles of NSMCE2, the essential SUMO ligase of the complex (constitutive knockout, conditional knockout, and SUMO‐dead knock‐in). Overall, our data support that the main role of the SMC5/6 complex is on facilitating segregation and suppressing recombination by an essential BLM‐ and SUMOylation‐independent pathway. Finally, this work reveals for the first time that the genome protection activity provided by the SMC5/6 complex is essential for the suppression of cancer and aging in mammals.
NSMCE2 localizes with BRCA1 at sites distinct from DNA breaks
In order to explore the potential functions of NSMCE2 in mammals, we developed antibodies against the murine and human proteins. In humans, NSMCE2 expression was highest in proliferating tissues (Appendix Fig S1A and B). Likewise, NSMCE2 expression was most abundant on Ki67‐positive regions of mouse embryos (Appendix Fig S1C). NSMCE2 levels were distinctively high in human and mouse testis (Fig 1A; Appendix Fig S1B). To investigate the potential role that NSMCE2 could be playing during spermatogenesis, we analyzed the distribution of NSMCE2 on spermatocyte spreads. Preparations were co‐stained with antibodies detecting SCP3, a lateral element of the synaptonemal complex, which provided information about the degree of synapsis between homologous chromosomes (Fig 1B). In contrast to the punctuated pattern shown by proteins involved in the repair of meiotic DNA double‐strand breaks (DSB), we did not detect any focal NSMCE2 staining in leptotene. In contrast, a distinct NSMCE2 staining was detected in pachytene spermatocytes, which coincided with regions of weak SCP3 signal (Fig 1B). This localization is reminiscent of proteins that accumulate at regions of incomplete synapsis of meiotic chromosomes such as BRCA1 (Scully et al, 1997b). Consistently, NSMCE2 colocalized with BRCA1 along the non‐homologous regions of the XY chromosomes during pachytene (Fig 1C). The accumulation of NSMCE2 at sex chromosomes is also evident by immunohistochemistry (IHC) of testes, where XY chromosomes form a compact structure known as the “sex body” on spermatocytes (inset, Fig 1A). Earlier studies reported a similar accumulation of SMC5 and SMC6 at the sex chromosomes (Taylor et al, 2001; Gomez et al, 2013) and also failed to detect any DSB‐related localization of the complex during meiosis. Moreover, the recruitment of BRCA1 to the XY chromosomes during spermatogenesis is unrelated to DNA breaks, since the same localization is present on cells lacking the SPO11 nuclease (Mahadevaiah et al, 2008). In summary, the distribution of NSMCE2 during spermatogenesis suggests that NSMCE2 is recognizing structures that are also recognized by BRCA1, but which are different from meiotic DSB.
To determine whether this colocalization between NSMCE2 and BRCA1 was also present in somatic cells, we performed immuno‐stainings on mouse embryonic fibroblasts (MEFs). BRCA1 accumulates at endogenous foci during replication, but relocalizes to DSB upon DNA breakage (Scully et al, 1997a; Tashiro et al, 2000). NSMCE2 colocalized with endogenous BRCA1 foci in unchallenged wild‐type MEFs (Fig 1D). However, and in contrast to BRCA1, NSMCE2 did not form ionizing radiation (IR)‐induced foci (Fig 1E and F). Previous studies in yeast suggested that NSMCE2 might be involved in the handling of recombinogenic structures induced by alkylating agents (Branzei et al, 2006). To investigate whether a similar response operates in mammals, MEFs were exposed for 1 h to methyl methanesulfonate (MMS) and let to recover for 24 h in the absence of the drug. These conditions promoted the accumulation of NSMCE2 foci that colocalized with BRCA1 (Fig 1D and E). The induction of NSMCE2 foci was not linked to the alkylating nature of the drug, since it could also be seen in response to other drugs that perturb DNA replication, such as poly‐ADP ribosyl transferase (PARP) inhibitors (Fig 1E). Moreover, catalytic inhibition of TOPO2A generated NSMCE2 foci, further suggesting that the complex can be recruited to specific sites on DNA in the absence of DNA breaks (Appendix Fig S2). In support of this, whereas NSMCE2 and H2AX phosphorylation (γH2AX) colocalized in response to MMS, NSMCE2 failed to colocalize with IR‐induced γH2AX foci, a bona fide marker of DSB (Rogakou et al, 1999) (Fig 1F). In summary, NSMCE2 accumulates at endogenous structures, which are distinct from DSB and which can be induced with reagents that challenge DNA replication and/or promote the accumulation of topological defects.
NSMCE2, but not its SUMO ligase activity, is essential for mouse development
In order to evaluate the role of NSMCE2 in vivo, we generated Nsmce2‐deficient animals. To this end, we took advantage of a murine ES cell line in which one Nsmce2 allele had been altered by insertion of a promoterless Gene Trap (clone AA0032; Sanger Institute Genetrap Resource). The mutation (Nsmce2GT) generates a chimeric cDNA containing the first 88 amino acids of NSMCE2 followed by a β‐geo coding sequence and thus lacks the SUMO ligase domain (Fig 2A and B). By using inverse PCR, we mapped the insertion at intron 3/4 of Nsmce2, which enabled genotyping. No Nsmce2GT/GT mice were born, and we also failed to detect homozygous mutant embryos at 13.5 or 10.5 dpc (Appendix Table S1). In contrast, 2.5 dpc Nsmce2GT/GT embryos were obtained at Mendelian ratios. However, upon 36 h of in vitro culture, a number of embryos rapidly degenerated, which were found to be Nsmce2GT/GT (Fig 2C and D). To determine the cause of death, we cultured 2.5 dpc embryos for 12 h to prevent their full degeneration. Nsmce2GT/GT embryos were identified by the absence of NSMCE2, as measured by immunofluorescence (Fig 2E). Whereas cells from wild‐type (wt) embryos were of similar shape and size and mitotic figures were rarely found, mutant embryos accumulated irregularly sized or multilobulated nuclei, as well as cells with condensed chromosomes, all of which would be consistent with defects in chromosome segregation. Supporting this view, some cells from 2.5 dpc Nsmce2GT/GT morulae presented an abnormal size (Fig 2C), consistent with an imbalanced segregation during the first embryonic cycles. Altogether, our data suggest that the early embryonic lethality found on Nsmce2‐deficient mice is due to segregation abnormalities that limit cell division during the first developmental stages.
The only known activity of NSMCE2 is a SUMO E3 ligase conferred by its C‐terminal Siz/PIAS‐RING (SP‐RING) domain. To evaluate the role of the NSMCE2 SUMO ligase activity in mammals, we generated a knock‐in mutant allele in which C185S and H187A mutations were introduced on the SP‐RING domain (Nsmce2SD) (Fig 3A and B). In vitro NSMCE2 auto‐SUMOylation assays using wild‐type and mutant NSMCE2 protein (cloned directly by RT–PCR from the corresponding mouse strains) confirmed the inactivating nature of the mutations (Appendix Fig S3). The mutation did not alter NSMCE2 protein levels, the stability of the SMC5/6 complex, nor its capacity to form MMS‐ or MMC‐induced foci (Fig 3C and D; Appendix Fig S4). Moreover, and in contrast to NSMCE2 deficiency, Nsmce2SD/SD animals were viable and fertile and showed no alteration of their lifespan (Fig 3E and F). Whereas in vitro assays using overexpressed NSMCE2 and SUMO detected some residual activity of the mutant protein upon SUMO1 (but not SUMO2) overexpression, this could derive from the endogenous wild‐type NSMCE2 that is present on the HEK293T cells used for these assays. In addition, the mutation introduced in these mice was first described and has been widely used in yeast as a SUMOylation‐deficient model (Andrews et al, 2005; Branzei et al, 2006; Pebernard et al, 2008b; Takahashi et al, 2008; Kegel et al, 2011). Hence, and whereas we cannot formally discard that some residual activity remains on Nsmce2SD/SD cells, our data reveal that the SUMO ligase activity of NSMCE2 is largely dispensable in mice.
Nsmce2 is a haploinsufficient tumor suppressor
In contrast to Nsmce2GT/GT, Nsmce2 heterozygous mice were viable and fertile with no apparent phenotype. However, Nsmce2GT/+ mice showed a decreased lifespan, which was associated with a higher incidence of tumors (Fig 4A and B). PCR analyses on tumors (n = 7) from Nsmce2 heterozygous animals revealed that they always kept a wild‐type Nsmce2 copy, suggesting that a reduced dosage of NSMCE2 is responsible for this phenotype. In order to investigate the impact of Nsmce2 haploinsufficiency, we analyzed the behavior of Nsmce2GT/+ primary cells. Nsmce2 heterozygous MEFs presented an ~50% reduction in NSMCE2 protein levels (Fig 4C). This reduction correlated with higher rates of spontaneous mitotic recombination as measured by sister chromatid exchanges (SCE) (Fig 4D). In addition, Nsmce2GT/+ MEFs showed evidences of improper chromosome segregation such as a higher incidence of micronuclei or polynucleated cells (Fig 4E and F). Hence, Nsmce2 is a haploinsufficient tumor suppressor in mice, which is associated with increased rates of mitotic recombination and chromosome mis‐segregation on heterozygous cells.
NSMCE2 suppresses recombination and facilitates segregation in MEFs
To overcome the limitations imposed by the essential nature of NSMCE2, we developed an Nsmce2 conditional allele where exon 3 is flanked by loxP sites (Nsmce2lox) (Fig 5A). We first used this allele in combination with a 4‐hydroxytamoxifen (4‐OHT)‐inducible Cre recombinase that is under the control of the ubiquitin promoter (Ub.CreERT2) (Ruzankina et al, 2007). To study the consequences of Nsmce2 nullyzygosity, Ub.CreERT2/Nsmce2lox/lox MEFs were generated. Upon exposure to 4‐OHT, Nsmce2lox/lox MEFs lost the expression of NSMCE2 (Fig 5B), and this was found to be essential at the cellular level as seen by clonogenic assays (Fig 5C). In agreement with Western blot data, immunofluorescence (IF) analyses revealed the loss of MMS‐induced NSMCE2 foci on 4‐OHT‐treated Ub.CreERT2/Nsmce2lox/lox MEFs (Fig 5D). Interestingly, NSMCE2‐depleted cells presented large amounts of BRCA1 foci, indicative of increased recombination. Consistently, NSMCE2‐deficient MEFs presented a significant increase in SCE levels even in the absence of exogenous agents (Fig 5E and F). Moreover, and similar to observations in BLM‐deficient cells (Wechsler et al, 2011), the increased SCE rates observed on NSMCE‐deficient cells were dependent on the MUS81 nuclease (Appendix Fig S5). Given that NSMCE2 was previously proposed to promote, rather than suppress, recombination at telomeres (Potts & Yu, 2007), we specifically evaluated inter‐telomeric recombination rates (T‐SCE) using chromosome orientation FISH. In agreement with the overall increase in recombination, NSMCE2‐deficient cells presented increased rates of T‐SCE (Fig 5G) which, however, did not led into any significant change on overall telomere lengths (Fig 5H and I). Finally, and in agreement with the segregation defects found on Nsmce2GT/GT embryos, NSMCE2‐deficient MEFs presented a significant accumulation of micronuclei and intercellular DNA bridges as well as cells with major segregation defects (Fig 5J; Appendix Fig S6). In contrast to the roles of NSMCE2 in segregation and recombination, high‐throughput microscopy analyses failed to detect any obvious impact of NSMCE2‐deficiency on the repair of DSB, as measured by the kinetics of appearance and disappearance of IR‐induced 53BP1 foci (Appendix Fig S7). Altogether, these data further support that NSMCE2 plays an essential role in limiting recombination and facilitating chromosome segregation in mammalian cells.
Nsmce2 deletion in adult mice leads to accelerated aging
To investigate the consequences of NSMCE2 deficiency in an entire organism, Nsmce2+/+ and Nsmce2lox/lox animals carrying the UQ.CreERT2 transgene were exposed to 4‐OHT. First, 14.5 dpc embryos were treated in utero for three consecutive days by intraperitoneal injections of 4‐OHT on pregnant mothers. Nsmce2lox/lox embryos showed intrauterine dwarfism that was accompanied by an overall loss of cellularity, more notorious on some specific organs such as the thymus (Fig 6A; Appendix Fig S8). Interestingly, NSMCE2 deletion on the developing thymus led to a significant accumulation of cells in mitosis, which once again could be consistent with segregation defects (Appendix Fig S8). However, given that the tamoxifen treatment prevents delivery, no born mice could be obtained regardless of the genotype. To analyze the impact of NSMCE2 deficiency on live mice, mice were fed with a 4‐OHT‐containing diet starting at weaning. The strategy reduced NSMCE2 expression on all tissues analyzed (Appendix Fig S9), an effect that was less pronounced on organs with higher turnover such as the spleen, probably reflecting a competitive disadvantage of NSMCE2‐depleted cells. At the organism level, Nsmce2 deletion led to a progressive and generalized progeroid syndrome to which animals succumbed within less than a year (Fig 6B; Appendix Fig S10; Movies EV1 and EV2). In addition, NSMCE2 deletion led to a number of pathologies that are also found on Bloom patients including altered pigmentation (Fig 6C), a reduced percentage of fat (Fig 6D), and progressive anemia (Fig 6E). Furthermore, NSMCE2 deficiency also led to a dramatic accumulation of micronuclei on proliferating tissues such as the intestinal crypts (Fig 6F; Appendix Fig S11). In summary, NSMCE2 deletion in adult mice leads to a generalized progeroid syndrome that presents several of the cellular and phenotypic hallmarks of Bloom's syndrome.
Independent roles of BLM and NSMCE2 in B lymphocytes
Given the similarities between NSMCE2 and BLM deficiency, we finally explored the potential relationship between these two pathways. To do so, and due to the essential nature of Blm and Nsmce2 in mice, we simultaneously deleted both genes in B lymphocytes with the help of a CD19.Cre allele (Rickert et al, 1997). Given that splenic B cells are in G0, lymphocyte cultures provide a unique system where to study DNA replication in a synchronously dividing population. Like previously observed on Nsmce2SD/SD cells (Fig 3), NSMCE2 deletion in B cells did not abrogate the formation of SMC5/6 complexes (Appendix Fig S12). Interestingly, whereas like MEFs or early embryos NSMCE2‐deficient B cells showed evidences of mis‐segregation, DNA fiber analyses revealed that DNA replication was not affected by NSMCE2 loss (Fig 7). Accordingly, NSMCE2 (or BLM) deficiency did not have a profound impact on spleen B‐cell percentages and mutant B cells were able to grow ex vivo. However, the combined deletion of Blm and Nsmce2 led to a severe synthetic lethal interaction evidenced by the reduced spleen size of double‐mutant mice (Fig 8A) and the acute loss of B cells on double‐mutant spleens (Fig 8B). Importantly, B cells lacking both NSMCE2 and BLM presented an additional increase in spontaneous SCE levels when compared to the individual mutants (Fig 8C). Moreover, double‐mutant B cells presented a remarkable increase in cell size, which was detectable by flow cytometry (Fig 8D) and even by visual inspection of the cultures (Fig 8E). This increase in cell size coincided with the presence of large and irregular multilobulated nuclei on Blm/Nsmce2 double‐mutant cells, indicative of severe segregation defects. Collectively, these data suggest that NSMCE2 and BLM suppress mis‐segregation and recombination through independent pathways. Further supporting this concept, MMS‐induced BLM and NSMCE2 foci do not colocalize (Appendix Fig S13). Altogether, we propose that NSMCE2 and BLM independently facilitate chromosome segregation and limit recombination in mammalian cells, with each complex recognizing a different subset of substrates.
On the essential roles of the SMC5/6 complex
All subunits of the SMC5/6 complex are essential in yeast (Zhao & Blobel, 2005). Likewise, a recent work revealed that SMC6 is essential for mouse development (Ju et al, 2013). The only example where vertebrate cells can tolerate deletion of a complex member is the chicken B‐cell line DT40, where SMC5‐ or NSE2‐deficient cells can be generated (Stephan et al, 2011a). This might reflect species‐specific roles or the fact that lymphoid cells are specially tolerant to the deletion of essential genes related to replication‐borne genomic instability such as Brca1 (Bunting et al, 2010). Consistently, Nsmce2 or Blm‐deleted mouse B lymphocytes could also be grown ex vivo. Nevertheless, B cells only undergo a few division cycles ex vivo and the pleiotropic phenotypes observed on NSMCE2‐deleted adult mice argue for an overall essential role of this pathway in mammalian cells. In addition, the finding that Nsmce2 heterozygous tumors retain the wild‐type copy and that Nscme2 is also essential for the growth of immortalized MEFs argues that the pathway might also be essential for cancer cells. What is then the basis for this essential role?
On one hand, some studies have suggested that the SMC5/6 complex plays a role in promoting recombinational repair, which was based on early findings that detected the recruitment of SMC6 to a nuclease‐induced DNA break (De Piccoli et al, 2006). More recent data have also detected the complex at recombination sites during yeast meiosis (Lilienthal et al, 2013; Xaver et al, 2013). Along these lines, siRNA‐mediated depletion of SMC5/6 complex members in human cells has been shown to diminish inter‐sister recombination rates, particularly at telomeres (Potts et al, 2006; Potts & Yu, 2007; Wu et al, 2012). In contrast to this view in promoting recombination, a careful analysis of the recombinatorial repair of meiotic breaks in yeast SMC5/6 mutants shows normal DSB repair kinetics (Lilienthal et al, 2013). Likewise, our analysis of 53BP1 foci shows no major deficiency in overall DNA repair kinetics on NSMCE2‐deficient cells. On the contrary, rather than an absence of recombination between sister chromatids, we consistently observed a significant increase in SCE rates on Nsmce2‐mutant cells, including at telomeres. This increase in recombination is in agreement with all previous data using genetically modified models including yeast, chicken, or mouse (Prakash & Prakash, 1977; Stephan et al, 2011a; Kliszczak et al, 2012; Ju et al, 2013). Whereas the complex might be dispensable for the initial steps of HR, we cannot rule out that it might be required for resolving inter‐sister chromatid links that might arise as products of recombination (i.e. Holiday Junctions). Accordingly, RAD51 deletion alleviates the growth defects of SMC5/6 mutants exposed to genotoxic agents (Chen et al, 2009; Chavez et al, 2011). Nevertheless, and regardless of a role in recombinational repair, HR is not essential in yeast and thus such an activity cannot account for the essential functions of the SMC5/6 complex.
In addition to HR, additional studies in yeast have revealed a role of the SMC5/6 complex in the resolution and/or disolution of joint DNA molecules (JM) (Torres‐Rosell et al, 2005; Branzei et al, 2006; Farmer et al, 2011; Copsey et al, 2013; Lilienthal et al, 2013; Xaver et al, 2013). Supporting the role of entangled DNA molecules, early works revealed a synthetic lethal interaction between SMC5/6 and topoisomerase mutants in yeast (Verkade et al, 1999). Moreover, the fact that catalytic inhibitors of TOP2A induce NSMCE2 foci (this study), together with a previous report showing that SMC6 colocalizes with TOP2A during meiosis (Gomez et al, 2013), further supports that the complex is recruited to substrates different to DNA breaks. This disentangling activity of SMC5/6 is also essential for the full completion of S‐phase, and similar to topoisomerase I mutants, SMC5/6 mutants have difficulties in completing DNA replication (Torres‐Rosell et al, 2007; Kegel et al, 2011). Whereas our DNA fiber analyses discards a general role of SMC5/6 on DNA replication, we cannot exclude that a more restricted role at certain loci (i.e. repetitive sequences) might facilitate the completion of DNA replication also in mammals, which could explain the segregation defects observed on Nsmce2‐deficient cells. In contrast to its proposed roles on HR, a role of the complex on the resolution of JM could explain all the phenotypes that we have observed on NSMCE2‐deficient cells. The accumulation of JM has two outcomes. First, some JM are resolved through the action of nucleases and subsequent recombination, which is the basis for SCE in mammalian cells. Second, if JM persist into mitosis, they constitute a barrier for chromosome segregation that can ultimately lead to mitotic catastrophe. The increased MUS81‐dependent SCE levels and severe chromosome segregation defects found on NSMCE2‐deleted MEFs and adult tissues support this view. In what regards to the role of SUMOylation, and in agreement with our findings, whereas Mms21 is essential for chromosome segregation during yeast meiosis, its SUMO ligase activity is not (Xaver et al, 2013). Whereas at this point we cannot discard that some residual SUMO ligase activity persists in Nsmce2SD/SD cells, the limited role of NSMCE2‐dependent SUMOylation could also simply reflect redundancy by alternative SUMO ligases. Consistently, the mild phenotypes of yeast Mms21 SUMOylation deficient strains on DNA damage‐induced SUMOylation or in suppressing recombination are greatly exacerbated upon deletion of additional SUMO ligases (Cremona et al, 2012; Albuquerque et al, 2013). Of note, whereas the SUMO ligase activity of NSMCE2 is dispensable for mouse lifespan and overall health in unchallenged conditions, it remains to be seen whether it becomes limiting in the context of DNA damage. Regardless of SUMOylation, a role on the dissolution of JM is consistent with the phenotypes observed on NSMCE2‐deficient cells and can account for the essential role of this complex in mice.
NSMCE2 operates independently of BLM
In mammals, JM elimination is mediated either by a pathway initiated by BLM (disolution), or through the action of mitotic structure‐specific nucleases such as MUS81 or GEN1 (resolution) (Mankouri et al, 2013). In yeast, many of the phenotypes observed on SMC5/6 mutants phenocopy those observed in sgs1 deficient strains, which has led to the suggestion that the complex could operate in JM disolution. Consistently, and similar to Sgs1, reexpression of Smc6 specifically in mitosis promotes the disolution of JM that accumulates on smc6‐deficient yeast cells (Bermudez‐Lopez et al, 2010). Despite the similarities between BLM and NSMCE2, early studies failed to link Smc5/6 to Sgs1 (Branzei et al, 2006). Moreover, and in agreement with our data, sgs1 deletion is synthetic sick with Mms21 deficiency in yeast (Chen et al, 2009), and double mutants present an increased accumulation of JM in mitosis (Torres‐Rosell et al, 2005) or meiosis (Copsey et al, 2013; Xaver et al, 2013). Finally, a recent work revealed that SMC6 knockdown in human cells leads to increased BLM foci (Gallego‐Paez et al, 2014). Together with our findings on NSMCE2‐ and BLM‐deleted B cells, these data support that NSMCE2 and BLM independently suppress recombination and facilitate segregation in mammalian cells.
One possibility to explain the independent roles of NSMCE2 and BLM would be that whereas both perform similar functions, they operate on different structures. Interestingly, whereas BLM foci are scattered throughout the nucleus, NSMCE2 foci form almost invariably around pericentromeric heterochromatin (Figs 1, 3 and 5; Appendix Figs S2 and S13). The same pericentromeric pattern has also been recently described for SMC6 during human spermatogenesis (Verver et al, 2014). This localization might suggest a preferential role of the SMC5/6 complex at repeats, given that centromeric sequences are the largest repeat of the mammalian genome. Consistently, several reports have observed a preferential localization of the Smc5/6 complex at repeat sequences in yeast and the complex is essential for the segregation of ribosomal DNA in S. cerevisiae, this being the largest repeat in the yeast genome (Torres‐Rosell et al, 2005, 2007; Zhao & Blobel, 2005; Lindroos et al, 2006; Chavez et al, 2010; Noel & Wellinger, 2011). Altogether, we propose that BLM and the SMC5/6 complex might perform similar functions, but with a preference toward structures that arise at repeated sequences in the case of SMC5/6.
Physiological impact of NSMCE2 deficiency
Whereas work in model organisms has suggested an important role for the SMC5/6 complex in safeguarding genomic integrity, the impact of this pathway on a mammalian organism remained largely unknown. Our work here reveals that whereas mild deficiencies on the complex might promote cancer development, more penetrant mutations might lead to accelerated aging. This transition from cancer to aging depending on the severity of the mutation has been previously observed on other genome integrity‐related pathways such as nucleotide excision repair or replication stress (Lopez‐Contreras & Fernandez‐Capetillo, 2010; Diderich et al, 2011). As to how a deficiency in NSMCE2 might promote cancer, one possibility is that this is a consequence of chromosomal rearrangements arising due to increased recombination rates. Supporting this view, Mms21 suppresses gross chromosomal rearrangements in S. cerevisiae (Albuquerque et al, 2013), and ChIP‐seq analysis of mouse B cells exposed to hydroxyurea revealed that SMC5 maps to regions frequently rearranged in human leukemias (Barlow et al, 2013). Interestingly, a recent report has revealed fusions involving NSMCE2 in acute myeloid leukemias (Chinen et al, 2014). The impact of these fusions on NSMCE2 activity remains unknown. Regarding the haploinsufficiency of NSMCE2, and even if our antibodies failed to detect the expression of a truncated NSMCE2 variant in Nsmce2+/GT cells, we cannot discard that our genetrap allele does express a smaller version of NSMCE2, which could have an effect on the observed phenotypes. Nevertheless, from the comparison between the findings made in Nsmce2+/GT versus nullyzygosity, it is clear that while milder deficiencies in the complex might promote cancer, more profound deficiencies will have severe detrimental effects at the organism level affecting multiple organs.
In what regards to aging, we can envision two non‐mutually exclusive mechanisms for the observed progeria. On one hand, NSMCE2 deletion might lead to the elimination of the mutant cells followed by a subsequent compensatory proliferation from non‐deleted wild‐type cells. This mechanism, previously proposed for the accelerated aging that arises upon deletion of the ATR kinase in adult mice (Ruzankina et al, 2007), would be supported by the lower reduction in NSMCE2 levels that is observed in organs with high turnover such as the spleen. Alternatively, or in addition, NSMCE2 deletion might promote the accumulation of abnormal cells due to inefficient chromosomal segregation, particularly in tissues with lower renewal rates, which could at some point compromise the functionality of the organ. Further studies on the organs of NSMCE2 depleted adult organs should be clarifying in this regard.
Finally, besides cancer, and regardless of the overall progeria, the use of NSMCE2‐deleted adult mice revealed a subset of phenotypes that are also found on BLM patients such as a reduced percentage of fat, altered pigmentation, and progressive anemia which, like in the case of BS cells, were associated with a significant increase in micronuclei on mutant tissues. Noteworthy, a recent report revealed the discovery of two human patients presenting reduced levels of NSMCE2 (Payne et al, 2014). Both human patients also presented dwarfism, altered pigmentation, and increased micronuclei, and whereas no obvious progeroid symptoms were reported, one of them died at 33 years of age from a sudden cardiovascular event. Of note, one of the mutations reported in humans also affected the SUMO ligase activity of NSMCE2. However, this mutation also severely reduced NSMCE2 levels so that the symptoms could be more related to the hypomorphism than to the SUMO ligase activity. Likewise, it is possible that the more severe disease we observe in mice versus what has been reported in human patients relates to the differences between nullyzygosity and hypomorphism. In any case, our work here has shed new light into the roles of the SMC5/6 complex in mammals and revealed that SUMOylation‐independent activities of NSMCE2 suppress recombination and micronuclei through a mechanism that operates independently of BLM and which is critical to prevent the onset of cancer and aging in mice.
Materials and Methods
The Nsmce2 genetrap strain was generated using the gene trap ES clone AA0032 from the Sanger Institute. Nsmce2SD knock‐in mice were generated by gene targeting, using a vector generated by recombineering (Genebridges, Dresden, Germany). Briefly, we introduced the mutations encoding C195S and H197A that inactivate the SUMO ligase activity of NSMCE2 (Andrews et al, 2005) into a targeting plasmid containing an FRT‐PGK‐neo‐FRT cassette. The neomycin resistance cassette was subsequently eliminated by crossing NSMCE2SD‐frt‐neo‐frt/+ mice with a strain expressing Flp recombinase from the β‐actin promoter (Rodriguez et al, 2000). Finally, the targeting vector for the generation of Nsmce2 conditional knockout mice was also obtained from Genebridges (Dresden, Germany). The targeting vector flanked exon 3 with loxP sequences and also contained an FRT‐PGK‐neo‐FRT that enabled selection in ES cells and which was later deleted as explained above. Blmlox/lox, CD19.Cre, UQ.CreERT2, and Mus81−/− mice have been previously described (Rickert et al, 1997; McPherson et al, 2004; Chester et al, 2006; Ruzankina et al, 2007). For Nsmce2 deletion in UQ.CreERT2 mice, animals were fed with a diet containing 400 mg of tamoxifen per kg (Harlan Tekland, Madison, USA). For intrauterine treatments, 14.5 dpc females were injected intraperitoneally for 3 consecutive days with 4‐OHT dissolved in corn oil, where embryos were isolated for further analyses. The percentage of fat was determined by dual energy X‐ray absorptiometry (DEXA) (Lunar PIXImus Densitometer, GE Medical Systems). All mice were kept under standard conditions at serum‐pathogen free facility of the Spanish National Cancer Centre in a mixed C57BL/6‐129/Sv background. All mouse work was performed in accordance with the Guidelines for Humane Endpoints for Animals Used in Biomedical Research and under the supervision of the Ethics Committee for Animal Research of the Instituto de Salud Carlos III.
Immunofluorescence and immunoblotting
Mouse spermatocyte IF was performed as described (Fernandez‐Capetillo et al, 2003). Briefly, spermatocyte spreads were treated for 3 min in 2% PFA and 0.03% SDS, washed in PFA 2%, and permeabilized for 1 min with 0.4% Photolo, Kodak. Preparations were subsequently stained following standard procedures using a blocking buffer containing 10% goat serum, 3% BSA, and 0.05% Triton X100. For embryo IF, mouse morulae were fixed with PTEMF buffer (0.2% Triton X100, 20 mM PIPES pH6.8; 1 mM MgCl2; 10 mM EGTA, 4% PFA) for 10 min at RT in a Microtest Plate (Greiner Bio‐One). Fixed morulae were next blocked in 3% BSA/PBS for 30 min and stained using standard procedures. For the detection of NSMCE2, BLM, and BRCA1 foci, a protocol that washes out the fraction of nucleoplasmic proteins previous to fixation was used as described before (Celeste et al, 2003). High‐throughput microscopy was performed by growing MEFs in μCLEAR bottom 96‐well plates (Greiner Bio‐One). Images were automatically acquired from each well with an Opera High‐Content Screening System (PerkinElmer) at 40× magnification and non‐saturating conditions. Images were segmented using the DAPI staining to generate masks matching cell nuclei from which the corresponding signals were calculated. Recombinant full‐length human NSMCE2 fused to GST was used to generate either rabbit polyclonal (VivoTecnia, Spain) or mouse monoclonal (Monoclonal Antibodies Unit, CNIO, Madrid) antibodies. The rabbit polyclonal antibody showed reactivity with human and mouse NSMCE2, whereas the monoclonal antibody only recognizes the human protein. Antibodies were purified using Affi‐Gel columns (Bio‐Rad) previously coated with immobilized GST‐NSMCE2 protein. γH2AX (Upstate Biotechnology, 05‐636), 53BP1 (Novus Biologicals, 100‐304A2), β‐ACTIN (Sigma, A2228), TUBULIN (Sigma, T9023), and SCP3 (Abcam, ab15093); BRCA1 (provided by Andre Nussenzweig); SMC5 (Biothyl, A300‐236A); and SMC6 (provided by Alan Lehmann) were used. Western blot analyses were performed using the LICOR platform (Biosciences).
Embryos or adult organs were fixed in formalin and embedded in paraffin for subsequent processing. Consecutive 2.5‐μm sections were treated with citrate for antigen recovery and processed for IHC with antibodies to NSMCE2 (described above), KI67, γH2AX, or activated caspase 3 (Upstate Biotechnology). Hematoxylin was used to counterstain. IHC samples were scanned with a MIRAX digitalized system (Zeiss).
MEF and B‐cell analyses
MEFs were isolated from 12.5 dpc embryos using standard procedures. For B‐cell cultures, resting splenic B lymphocytes were isolated from 8‐ to 12‐week‐old WT or mutant spleens with anti‐CD43 microbeads (anti‐Ly48; Miltenyi Biotech) and cultured with standard protocols. For SCE analyses, cells were cultured in the presence of 5′‐bromo‐2′‐deoxyuridine (BrdU; Sigma) at a final concentration of 10 μM and then allowed to replicate their DNA once for 24 h. Colcemide was added at 0.1 μg/ml during the last 5 h. Metaphases were prepared using a standard hypotonic/Carnoy procedure and subsequently treated with UV (355 nm) and Hoechst to counterstain nascent DNA strands. Slides were finally stained with a 1% Leishman solution diluted 2/3 in Gurr's buffer. Analysis of telomere lengths using Q‐FISH (Samper et al, 2000) or T‐SCE events using chromosome orientation FISH (CO‐FISH) (Gonzalo et al, 2006) was performed as described. NSMCE2lox/lox.Ub.Cre.ERT2+/T MEFs were treated with 1 μM 4‐Hydroxytamoxifen (4‐OHT, H7904, Sigma) 48 h before the correspondent assay.
NSMCE2 auto‐SUMOylation assay
FLP‐In™‐293 cells over‐expressing NSMCE2WT or NSMCE2C185S/H187A were transfected with plasmids containing SUMO1‐GFP or FLAG‐SUMO2 cDNAs using Lipofectamine 2000 (Invitrogen). Forty‐eight hours post‐transfection, cells were harvested and processed as following. For SUMO1‐GFP, lysates were treated according to the instructions of the μMACS GFP Isolation kit (Miltenyi Biotec). In the case of FLAG‐SUMO2, cells were lysed in protein lysate buffer (50 mM Tris–HCl pH 7,4; 150 mM NaCl; 1 mM EDTA; 1 mM EGTA; 270 mM sucrose; 1% Triton‐X100) and supplemented with a mix of protease inhibitors (Sigma‐Aldrich), Benzonase® (Merck), and 20 mM N‐ethylmaleimide (Sigma‐Aldrich). Precleared lysates were subsequently immunoprecipitated with magnetic anti‐FLAG beads (Sigma‐Aldrich) for 4 h at 4°C. After three washes in lysis buffer, immunoprecipitated samples were denatured in Nupage buffer and loaded on gradient 4–12% SDS–PAGE gels (Invitrogen). GFP (Roche), NSMCE2 (described above), Tubulin, and FLAG (Sigma) antibodies were used.
DNA fiber analysis
Exponentially growing cells were pulse‐labeled with 50 μM CldU (20 min) followed by 250 μM IdU (20 min). Labeled cells were collected, and DNA fibers were spread in buffer containing 0.5% SDS, 200 mM Tris pH 7.4, and 50 mM EDTA. For immunodetection of labeled tracks, fibers were incubated with primary antibodies (for CldU, rat anti‐BrdU; for IdU, mouse anti‐BrdU) and developed with the corresponding secondary antibodies conjugated to Alexa dyes. Mouse anti‐ssDNA antibody was used to assess fiber integrity. Slides were examined with a Leica DM6000 B microscope, as described previously (Mouron et al, 2013). The conversion factor used was 1 μm = 2.59 kb (Jackson & Pombo, 1998). In each assay, 200–300 tracks were measured to estimate fork rate and 300–500 tracks were analyzed to estimate the frequency of origin firing [first label origins (green‐red‐green) are shown as percentage of all red‐labeled tracks (CldU)] (Petermann et al, 2010).
AJ and PG‐M participated in the generation and analyses of NSMCE2 mouse models. FS participated on the analysis of BLM and NSMCE2 interaction and helped on the analysis of segregation, NSMCE2 foci, and DNA replication experiments. ET helped on the analysis of SUMOylation‐deficient mutants and performed SCE analyses on Nsmce2 and Mus81 double‐mutant MEFs. EL helped with biochemistry and analysis of Nsmce2‐mutant cells. MM helped on the characterization of Nsmce2‐mutant MEFs and B cells. SR and JM performed DNA fiber analyses. PM and MAB performed telomere analyses. OF‐C supervised the study and wrote the manuscript.
Conflict of interest
The authors declare that they have no conflict of interest.
The authors want to thank Jordi Torres and Mark O'Driscoll for comments on the manuscript. Work in OF laboratory related to this project was supported by Fundación Botín, by Banco Santander through its Santander Universities Global Division and by grants from MINECO (SAF2011‐23753 and SAF2014‐57791‐REDC), Howard Hughes Medical Institute, and the European Research Council (ERC‐617840). Work in JM laboratory was funded by a grant from MINECO (BFU2013‐49153P).
- © 2015 The Authors