, Volume 128, Issue 3, pp 249–265 | Cite as

S. cerevisiae Srs2 helicase ensures normal recombination intermediate metabolism during meiosis and prevents accumulation of Rad51 aggregates

  • Laura J. Hunt
  • Emad A. Ahmed
  • Hardeep Kaur
  • Jasvinder S. Ahuja
  • Lydia Hulme
  • Ta-Chung Chou
  • Michael Lichten
  • Alastair S. H. GoldmanEmail author
Open Access
Original Article


We investigated the meiotic role of Srs2, a multi-functional DNA helicase/translocase that destabilises Rad51-DNA filaments and is thought to regulate strand invasion and prevent hyper-recombination during the mitotic cell cycle. We find that Srs2 activity is required for normal meiotic progression and spore viability. A significant fraction of srs2 mutant cells progress through both meiotic divisions without separating the bulk of their chromatin, although in such cells sister centromeres often separate. Undivided nuclei contain aggregates of Rad51 colocalised with the ssDNA-binding protein RPA, suggesting the presence of persistent single-strand DNA. Rad51 aggregate formation requires Spo11-induced DSBs, Rad51 strand-invasion activity and progression past the pachytene stage of meiosis, but not the DSB end-resection or the bias towards interhomologue strand invasion characteristic of normal meiosis. srs2 mutants also display altered meiotic recombination intermediate metabolism, revealed by defects in the formation of stable joint molecules. We suggest that Srs2, by limiting Rad51 accumulation on DNA, prevents the formation of aberrant recombination intermediates that otherwise would persist and interfere with normal chromosome segregation and nuclear division.


Budding yeast Meiosis Recombination Srs2 helicase Rad51 


The production of haploid gametes during meiosis requires the ordered segregation of the diploid genome, such that each chromosome is present as a single copy in daughter cells. This occurs through two successive nuclear divisions (meiosis I and meiosis II) that follow a single round of DNA replication. In most organisms, homologous chromosomes of different parental origin (called homologues), each comprising two sister chromatids held together by cohesin, are first paired and then synapsed end-to-end by a structure called the synaptonemal complex (SC; reviewed in Heyting 1996). Homologues become covalently linked by crossovers (COs), and this linkage allows their correct orientation on the meiosis I spindle, so they segregate to opposite poles during the first meiotic nuclear division. Sister chromatids are subsequently separated during meiosis II. In most eukaryotes, homologous recombination (HR) is critical during meiosis, both for the pairing and synapsis processes that bring homologues together, and for the formation of crossovers that allow their correct segregation (reviewed in Petronczki et al. 2003).

Meiotic HR is initiated by DNA double-strand breaks (DSBs), formed by the Spo11 protein (Keeney et al. 1997). DSBs are resected, in a process dependent on Sae2/Com1 (McKee and Kleckner 1997; Prinz et al. 1997) to form 3′ single-stranded DNA (ssDNA) capable of a homology search. During the mitotic cell cycle, HR requires the strand exchange protein Rad51, which displaces the ssDNA-binding RPA protein complex and mediates strand invasion into homologous duplex DNA (reviewed in Morrical 2015). The invading single strand displaces a strand of the homologous duplex and primes DNA synthesis to form a displacement loop (D-loop). D-loop collapse, followed by reannealing to ssDNA at the other break end, forms exclusively noncrossover (NCO) products in a process called synthesis-dependent strand annealing (SDSA; Nassif et al. 1994). Alternatively, capture of the second ssDNA by the D-loop forms a double Holliday junction (dHJ) intermediate, which can be resolved either as an NCO or as a CO (Szostak et al. 1983). During the mitotic cell cycle, most Rad51-mediated HR occurs between sister chromatids (Bzymek et al. 2010; Kadyk and Hartwell 1992), and events that involve homologues produce NCOs, rather than COs (Ira et al. 2003; Lichten and Haber 1989), thus reducing the risk of genome rearrangement and loss of heterozygosity.

In contrast, interhomologue COs are an important outcome of HR during meiosis, since they mediate proper homologue orientation and segregation. In many organisms, including budding yeast, meiosis-specific modifications of recombination encourage both strand invasion between homologues and production of a higher proportion of COs. This involves the expression of a second strand exchange protein, Dmc1 (Bishop et al. 1992). Rad51 is still present in meiotic cells, and is an essential cofactor for normal Dmc1 loading and strand invasion activity (Cloud et al. 2012). However, in budding yeast, Rad51 strand exchange activity is dispensable for recombination (Cloud et al. 2012), and is negatively regulated during meiosis by at least two known mechanisms involving the meiosis-specific kinase Mek1. Mek1 kinase is activated by binding to a phosphorylated form of the meiotic chromosome axis protein Hop1 (Niu et al. 2005), which is formed in the vicinity of meiotic DSBs by DNA damage response kinases (Carballo et al. 2008). Active Mek1 phosphorylates Rad54, a protein required for Rad51 to form stable strand invasion products, and prevents Rad54-Rad51 interaction (Niu et al. 2009). Mek1 also phosphorylates and stabilises the meiosis-specific Hed1 protein, which binds to Rad54 and prevents it from interacting with Rad51 (Callender et al. 2016).

Rad51 is also negatively regulated by the budding yeast Srs2 protein, a 3′ to 5´ DNA helicase/translocase of the UvrD family (reviewed in Niu and Klein 2017). Srs2 interacts with Rad51 filaments in vitro and strips them from DNA (Kaniecki et al. 2017; Krejci et al. 2003; Veaute et al. 2003). Loss of Srs2 activity in mitotic cells leads to DNA damage sensitivity, genome instability, reduced DSB repair efficiency and an increase in COs among repair products (Elango et al. 2017; Ira et al. 2003; Lawrence and Christensen 1979; Marini and Krejci 2010; Rong et al. 1991). As srs2 sensitivity to DNA damage is partially suppressed by deletion of RAD51, it is thought that srs2 mutant phenotypes relate to failures in Rad51 removal from ssDNA (Ira et al. 2003; Krejci et al. 2003). Srs2 also unwinds branched DNA structures in vitro, including those mimicking D-loop recombination intermediates, consistent with a role in promoting SDSA (Dupaigne et al. 2008; Kaniecki et al. 2017; Liu et al. 2017; Marini and Krejci 2012). However, this function has yet to be fully investigated in vivo. In meiosis, Srs2 activity is required for normal spore viability and meiotic progression, and srs2∆ mutants show reduced formation of COs and NCOs (Palladino and Klein 1992; Sasanuma et al. 2013a; b).

We have analysed further the importance of Srs2 function during meiosis and found that it is required for normal recombination intermediate metabolism and nuclear division. In srs2 mutants, Rad51 protein appears in aggregates after exit from pachytene, when the SC has been dissolved. These Rad51 aggregates are often associated with RPA, and arise only if programmed DSBs are formed and if Rad51 has full-strand exchange capability. srs2 mutants show partial defects in meiotic nuclear divisions, but cytological investigation of chromosomal segregation implies that sister centromere separation occurs normally. These data suggest that srs2 mutants suffer entanglements caused by abnormal interhomologue recombination intermediates. Consistent with this, we found evidence for defects in formation of stable interhomologue recombination intermediates. We propose that loss of Srs2-mediated negative regulation of Rad51 allows for defects in DNA interactions during pachytene, which later lead to defects that prevent normal nuclear division.


Sporulation is delayed and reduced in srs2 mutants, with decreased spore viability

Known meiotic defects caused by loss of Srs2 activity include nuclear division defects, reduced sporulation and reduced spore viability (Palladino and Klein 1992). We confirmed these phenotypes in our srs2 mutant strains, which included: srs2∆, which produces no Srs2 protein; srs2-101, which is mutated in the predicted ATP-binding site (Rong et al. 1991); and srs2-md, a replacement of the endogenous SRS2 promoter with the CLB2 promoter, where SRS2 is expressed in mitotic cells but not during meiosis (Chu et al. 1998).

All three srs2 mutants showed meiotic nuclear division defects. The fraction of cells completing both meiotic nuclear divisions was reduced from 94% in SRS2 strains to 60, 59 and 60%, respectively, in cells homozygous for srs2-md, srs2-101 and srs2Δ. In addition, nuclear division was delayed by approximately 1 h, and a substantial fraction (~ 20%) of srs2 mutant cells completed only one of the two nuclear divisions (Fig. 1a–e). Incomplete nuclear division could also be observed in srs2 strains, with nuclei remaining connected by chromosome bridges at times when nuclear division was complete in wild type (Fig. 1f). Spore viability is reduced in cells that complete meiosis, from 98% in wild type to 63–68% in srs2 mutants (Fig. 1g). Tetrad spore death patterns typical of defects specific to either meiosis I or meiosis II were not observed, suggesting that segregation failure is not specific to a single stage of meiosis (Fig. 1h).
Fig. 1

Sporulation defects caused by loss of Srs2 activity. a Examples of nuclear morphology. Symbols alongside each panel correspond to symbols used in graphs. be Meiotic progression. b In SRS2 strains, about 95% of cells progress through the two meiotic nuclear divisions. ce Progression through nuclear divisions is reduced to about 60% compared with wild type and is delayed by ~ 1 h; vertical arrows on x-axis indicate when 40% of cells had completed meiosis II. srs2 mutants also display persistent binucleate cells. SRS2, n = 7; srs2-md, n = 9; srs2-101, n = 5; srs2Δ, n = 3; error bars—standard error of the mean. f DNA bridges observed in srs2 mutants (example from 9 h, srs2-101). g Reduced spore viability in srs2 mutants. h Patterns of spore viability in tetrads from srs2 mutants are inconsistent with either meiosis I or meiosis II nondisjunction. SRS2, n = 5, 159 tetrads total; srs2-101, n = 2, 99 tetrads; srs2Δ, n = 2, 100 tetrads; srs2-md, n = 3, 139 tetrads; error bars in (g) indicates range

The spindle cycle continues in srs2 mutants despite nuclear division defects

During each round of meiosis, the spindle pole body (SPB, budding yeast centrosome equivalent) must duplicate, divide and migrate to opposite poles of the cell in order for the dividing chromosomes to be correctly drawn along the tubulin spindles at anaphase. Duplicated SPBs are initially connected by a bridge (Byers and Goetsch 1975), and spindle separation is controlled by activity of the cyclin-dependent kinase Cdc28/Cdk1 (Jaspersen et al. 2004). During the meiosis I to meiosis II transition, SPBs must be relicensed for duplication in a process regulated by the Cdc14 phosphatase (Fox et al. 2017). Thus, analysis of SPB division provides a useful indicator of meiotic cell cycle progression.

To monitor SPB division, we examined spread cells from strains expressing fluorescently tagged SPB (Cnm67-mCherry) and spindle proteins (GFP-Tub1), neither of which altered meiotic progression (Supplementary Fig. S2b). Cells were classified by number of SPB signals, as for nuclear division (Fig. 2a). As expected, due to SPB division preceding nuclear division, cells with two, three or four SPBs appeared slightly less than 1 h before cells with the same number of nuclei, with 96% of cells completing two SPB divisions by 9 h post-induction of meiosis (Fig. 2b, c). In the srs2-101 strain, cells that had accomplished SPB division and separation increased with wild-type timing until 6 h and then increased only slightly. By 9 h, more than 75% of cells had produced at least two separated SPBs, while only 60% of cells had completed the meiosis I nuclear division (Fig. 2b) and about 35% of cells had failed to complete the two SPB and nuclear divisions (Fig. 2c). Most notably, a significant population of srs2 cells had divided SPBs but contained only an undivided nuclear signal. The fraction of cells with this phenotype reached a maximum at 6 h, with 32 and 24% of srs2-101 and srs2Δ cells, respectively, compared with 8.0% in wild type (Fig. 2e). This observation, that loss of Srs2 activity results in a significant population of cells with divided SPBs but undivided nuclei, suggests that these cells are attempting to progress through meiosis II despite the nucleus failing to divide correctly in meiosis I. However, it should also be noted that about a quarter of the population does not undergo even the first round of meiotic SPB separation.
Fig. 2

Altered nuclear division and spindle dynamics in the absence of Srs2 activity. a Classifications used during analysis of spindle pole body (SPB) and nuclear (DAPI) division. b, c Fraction of cells completing both meiotic nuclear (blue) or SPB divisions. Unlike nuclear division (see also Fig. 1), SPB division is not delayed in srs2-101 (nuclear division data from Fig. 1; SPB analysis, n = 2; error bars—range). d Combining nuclear and SPB analysis reveals two distinct populations of cells that have completed both SPB divisions: class IIIa, cells with at least two nuclei, as expected for cells with divided SPBs, and class IIIb, cells with only a single nucleus, despite having divided SPB signals. Scale bar, 6 μm. e Loss of Srs2 activity is associated with an increased frequency of class IIIb nuclei, which have completed SPB division but have failed to divide nuclei (SRS2, n = 2; srs2-101, n = 2; srs2∆, n = 1; error bars—range)

Sister centromeres separate in the absence of Srs2, despite failures in nuclear division

To investigate the nature of the nuclear division failure in srs2 strains, we monitored sister chromatid separation, using strains that expressed a fusion between the Tet repressor and GFP (TetR-GFP) and that were heterozygous for a Tet operator array (tetO, 224 repeats) inserted near the centromere of chromosome V. In such strains, the separation of the tetO/TetR signals is a proxy for sister centromere separation. In wild-type cells, a single signal is visible until meiosis II, when this signal divides into two signals, which then segregate into two of the four nuclei present at the tetranucleate stage (Fig. 3a).
Fig. 3

Sister chromatid separation observed during meiosis using a tet repressor-GFP fusion and heterozygous tet operon repeats at the URA3 locus. a Representative images showing progression of sister chromatid segregation through meiosis in wild-type cells. Scale bar, 5 μm. b Representative images of SRS2 (6 and 7 h) and srs2-md (6 and 8 h) cells with divided spindle pole bodies. Even when the nucleus fails to divide, separated tetO/TetR signals can be observed suggesting sister chromatids have separated. Scale bar, 5 μm. c Percent of mononucleate cells that have divided SPBs and contain divided TetR-GFP signals (i.e. class IIIb cells, see Fig. 4e). n = 2, except for SRS2 at 8 h for which class IIIb cells were only observed in one experiment; error bars denote range

Cells with divided SPBs but one nucleus (i.e. class IIIb cells, see Fig. 2d) were analysed for tetO/TetR signal separation. Interestingly, most class IIIb cells in the srs2-md strain had two tetO/TetR signals, despite the nucleus failing to divide (Fig. 3b, c). Although fewer wild-type cells displayed single nuclei at late time points in meiosis, it is notable that the tetO/TetR signals in these cells also were usually separated. This suggests that even when nuclear division fails, the majority of sister centromeres are separating correctly, at least where measured close to pericentromeric DNA on chromosome V. Similar analysis of a strain with homozygous tetO inserts also indicates that 4 SPB signals are frequently observed in srs2 strains (EAA and ASHG, unpublished observations), suggesting that centromeres on both homologous chromosomes and sister chromatids separate.

Loss of Srs2 function in meiosis leads to Rad51 aggregate formation

As Srs2 is thought to regulate mitotic recombination by removing Rad51 from ssDNA nucleoprotein filaments and allowing repair by SDSA (Andersen and Sekelsky 2010), we hypothesised that the meiotic nuclear division failure seen in srs2 cells may be due to entanglements caused by a failure to remove Rad51. We therefore analysed Rad51 distributions in nuclear spreads using immunofluorescence. Cells were classed into three groups: those with no Rad51 signal; those with only small Rad51 signals (< 0.39 μm in any direction), hereafter called ‘Rad51 foci’; and those with large Rad51 signals (> 0.39 μm), which we here refer to as ‘Rad51 aggregates’ (Fig. 4). srs2-md mutants were observed to accumulate Rad51 aggregates at later times during meiosis (4 h onward); these aggregates were rarely seen in wild-type cells (Fig. 4c). Similar Rad51 aggregate accumulation is observed in srs2-101 (Supplementary Fig. S2b) and in srs2∆ mutants (Sasanuma et al. 2019). A substantial fraction of srs2 cells also display persistent Rad51 foci, at times when these foci have disappeared from wild type (Fig. 4b).
Fig. 4

Mutants lacking Srs2 activity form Rad51 aggregates. a Detection of Rad51 in nuclear spreads; blue, DAPI/DNA; red, α-Rad51. Cells were categorised as: (i) cells with no Rad51 signal, (ii) cells with Rad51 foci and (iii) cells with large Rad51 aggregates. Scale bar, 5 μm. bsrs2 mutants show a persistent Rad51 signal (either foci or aggregates). csrs2 mutants display Spo11-dependent Rad51 foci. dsrs2 mutants display Spo11-dependent Rad51 aggregates. (SRS2, n = 3; srs2-md, n = 5; srs2-md spo11, n = 1; error bars—standard error of the mean)

Meiotic DSB formation requires Spo11 transesterase activity, which is abolished by loss of the reactive OH group at the catalytic tyrosine (spo11-Y135F). Both aggregate formation (Fig. 4c) and nuclear division defects of srs2 mutants are suppressed by spo11 mutation (Supplementary Fig. S2a, Sasanuma et al. 2019), indicating that both Rad51 aggregates and barriers to nuclear division form as a consequence of abnormal DSB repair in the absence of Srs2.

Meiotic phenotypes of srs2 depend on Rad51-mediated strand invasion

Rad51 protein has two activities with the potential to contribute to aggregate formation during meiosis in srs2 mutants. Rad51 forms a filament on ssDNA, which then catalyses invasion of homologous duplex DNA through a second DNA binding site. rad51-II3A mutants, which lack this second binding site, are competent for filament formation but defective in strand invasion (Cloud et al. 2012). During meiotic recombination in budding yeast, Rad51 acts as a co-factor in filament assembly but not strand invasion with a meiosis-specific homologue, Dmc1, and rad51-II3A mutants are competent for meiotic DSB formation and homologous recombination (Cloud et al. 2012). If the phenotypes observed in srs2 mutants were due to a defect in removing Rad51 from meiotic recombination intermediates, then aggregates should still form in srs2 rad51-II3A double mutants. Because rad51-II3A and srs2-101 or srs2Δ mutants are synthetically lethal (T-CC, EAA and ASHG, unpublished observations), we combined the meiotic-depletion srs2-md allele with rad51-II3A. Only ~ 4% of srs2-md rad51-II3A cells contained Rad51 aggregates, as compared to 15–25% of srs2-md RAD51 cells (Fig. 5b). This indicates that aggregate formation depends on Rad51’s ability to bind a second DNA molecule, rather than retention of Rad51 filaments. Since Rad51 strand exchange activity is not normally required for meiosis, this suggests that Rad51 aggregates derive from ‘off-pathway’ events, rather than from normal meiotic recombination intermediates.
Fig. 5

Analysis of the Rad51 aggregation phenotype. a Deletion of MEK1 does not suppress aggregate formation, indicating that an interhomologue bias for strand invasion is not required. b Rad51 aggregates do not form in rad51-II3A or ndt80∆ mutants, indicating that both Rad51-mediated strand invasion and exit from pachytene are required for aggregate formation. c Deletion of SAE2 does not prevent aggregate formation, suggesting that normal DSB processing is not required. Interestingly, a small fraction of sae2Δ cells form aggregates at later time points in a SPO11-dependent manner. (SRS2, n = 3; srs2-101, n = 3; srs2-101 mek1Δ, n = 2; mek1Δ, n = 2; srs2-md, n = 5; srs2-md ndt80Δ, n = 1; srs2-md rad51-II3A, n = 3; srs2-md sae2Δ, n = 4; sae2Δ, n = 3). Error bars—standard error of the mean, except for srs2-101 mek1∆ and mek1∆, where they denote range

Rad51 aggregation is independent of MEK1-dependent interhomologue bias

To test whether Rad51 aggregates that form in srs2 mutants arise from normal interhomologue meiotic recombination intermediates, we examined mutants lacking Mek1, a meiosis-specific kinase that is a major effector of the bias towards use of the homologue, rather than the sister chromatid, during meiotic DSB repair (Niu et al. 2005). Deletion of MEK1 did not rescue the aggregation phenotype of srs2-101 mutants, suggesting Rad51 aggregates are not caused by a failure in the processing or resolution specifically of interhomologue recombination intermediates (Fig. 5a).

Rad51 aggregate formation is independent of Sae2

As Rad51 aggregate formation depends on Spo11-DSB formation and the ability of Rad51 to bind a second DNA molecule, we hypothesised that Rad51 aggregation should also be dependent on DSB resection. To test this, we performed analysis in cells lacking Sae2, which is required for normal resection of Spo11-induced DSBs prior to strand invasion. Surprisingly, however, deletion of SAE2 did not prevent the formation of aggregates, which at late time points were instead slightly increased in srs2-md sae2Δ double mutants compared to srs2-md alone (Fig. 5c). Rad51 aggregates were also observed in sae2Δ SRS2 cells at later time points, all be it at lower levels (Fig. 5c), and these aggregates were also Spo11 dependent (data not shown). The proportion of aggregates seen at late time points in srs2-md sae2∆ double mutants reflected the sum of levels seen in the single mutant cells, consistent with an independent contribution from the two single mutations (Fig. 5c). Thus, Rad51 aggregate formation does not require normal meiotic DSB resection.

Rad51 aggregates form after exit from pachytene

Since analysis of srs2 rad51-II3A and srs2 mek1 double mutants suggested that Rad51 aggregates form as the consequence of abnormal meiotic recombination, it was of interest to determine the stage of meiosis at which aggregation occurs. Rad51 immunofluorescence was combined with visualisation of the synaptonemal complex (SC) using GFP-tagged Zip1 (White et al. 2004), a component of the tripartite structure that forms along the length of homologous chromosomes during the pachytene stage of meiotic prophase and provides a framework that assists the process of homologous recombination (Heyting 1996; Yang and Wang 2009). Once recombination is completed, cells exit pachytene in a process that requires gene expression driven by the Ndt80 transcription factor (Chu and Herskowitz 1998). The SC is disassembled and recombination intermediates resolve, leaving the crossover products of recombination to maintain connections between homologues (Sourirajan and Lichten 2008; Zickler and Kleckner 1999, 2016). As expected, Rad51 foci were found in wild-type cells with either Zip1 foci or long regions of synapsis, but were absent from cells lacking Zip1 signal. However, srs2 mutants displayed Rad51 foci in Zip1-positive cells and prominent Rad51 aggregates in cells that lacked any Zip1 signal, suggesting that aggregates form after cells exit pachytene (Fig. 6). To confirm this, we examined ndt80Δ mutants, which arrest in pachytene with fully synapsed homologues and duplicated but unseparated SPBs (Xu et al. 1995). Rad51 aggregates were absent from both srs2-md ndt80∆ cells (Fig. 5b) and srs2-101 ndt80 cells (data not shown) at all times. These results indicate that, in srs2 mutants, Rad51 aggregate formation occurs after the cells exit from pachytene, and thus after meiotic recombination would be complete in wild-type cells.
Fig. 6

Analysis of Rad51 aggregates in cells expressing Zip1-GFP, a synaptonemal complex protein. a Representative images of srs2-101 cells with punctate or elongated Zip1-GFP signals (3 and 5 h, respectively) with clear Rad51 foci. b Representative images of Zip1-negative srs2-101 cells at 5 h. Cells can be classified as having no Rad51 signal, large aggregates of Rad51 or elongated thread-like aggregates of Rad51. Aggregates of Rad51 can be observed in srs2-101 cells in the absence of a synaptonemal complex

RPA colocalises with Rad51 aggregates

The ssDNA that is formed by DSB resection is initially coated with replication protein A (RPA), a heterotrimeric complex that is essential for viability (Brill and Stillman 1991; Chen et al. 2013). Although RPA binding to ssDNA is important for formation of active Rad51 filaments, RPA is displaced during filament formation. Thus, Rad51 and RPA foci are at times adjacent to each other but rarely are truly colocalised (Gasior et al. 1998; Hays et al. 1998). However, a substantial fraction of Rad51 aggregates that form in srs2-md colocalise with either a focus or an aggregate of RPA (Fig. 7a, b). Detailed analysis of Rad51 and RPA signals at 5 h post-induction of meiosis in srs2-md cells confirmed that foci of RPA and Rad51 generally do not colocalise, but Rad51 and RPA are frequently colocalised in aggregates, with more than 90% of Rad51 aggregates colocalising with RPA (Fig. 7c), consistent with the suggestion that the Rad51 aggregates that form in srs2 mutants reflect the presence of abnormal recombination events.
Fig. 7

Rad51 aggregates frequently colocalise with RPA. a Representative images of: (i) a nucleus with both Rad51 and Rfa1 foci, with minimal colocalisation and (ii) a Rad51 aggregate colocalised with Rfa1. b RPA colocalisation with Rad51 foci across a time course. Colocalisation between Rad51 foci and Rfa1 is infrequent. c RPA colocalisation with Rad51 aggregates in the same experiment. Almost all Rad51 aggregates that form in srs2-md cells colocalise with either foci or aggregates of Rfa1; > 100 nuclei were scored for all time points, except for SRS2, 7 h and srs2-md, 0 h (70 and 72 nuclei, respectively)

Altered recombination intermediates in srs2 mutants

The above analysis indicates that aggregates of Rad51 do not form until cells exit from pachytene, which is also the time that dHJ-containing recombination intermediates (joint molecules (JMs)) are resolved as COs (Allers and Lichten 2001; Sourirajan and Lichten 2008). To test the suggestion that Rad51 aggregate formation might be associated with abnormal JM metabolism, molecular analysis of recombination intermediates and products was performed, using a DNA isolation method that preserves dHJ intermediates (Allers and Lichten 2000). Southern blots were used to detect events at a URA3-ARG4 recombination reporter (Jessop et al. 2005) inserted on the left arm of chromosome III (Jessop et al. 2005; Fig. 8; Supplementary Fig. S3a). While DSB levels were similar in srs2 and SRS2 strains (Supplementary Fig. S3b), a marked deficit in levels of detectable JMs (4- to 7-fold) was observed in srs2 mutants (Fig. 8a, b). Despite the apparent reduction in JMs, which are crossover precursors (Allers and Lichten 2001), crossovers were recovered at similar levels from wild-type and srs2 mutant cells (Fig. 8c).
Fig. 8

Differences between recombination intermediates (JMs) formed in the presence and absence of Srs2 activity. a Southern blots of XmnI digests of DNA from the indicated time after initiation of meiosis, probed to detect joint molecules (dHJ—double Holliday junctions; mcJM, multichromatid joint molecules) at a recombination reporter on chromosome III (see Fig. Fig. S1). b Quantification of blots from SRS2 (n = 5, data from (De Muyt et al. 2012; Kaur et al. 2015) and one additional replicate; error bars denote SEM), srs2-101 (n = 5; error bars denote SEM) and srs2-md (n = 2; error bars denote range). JM recovery is markedly reduced in the absence of Srs2 activity. c Crossovers are formed at similar levels in the presence and absence of Srs2 activity, despite the marked difference in JM recovery. Noncrossovers are recovered at ~ 50% greater levels in srs2 mutants than in wild type. d Detection of JMs, as in (a), in psoralen-crosslinked DNA samples. Bands marked with an asterisk are the products of crosslink-induced partial XmnI digestion. e Quantification of three gels from two sporulations; error bars denote SEM. Psoralen crosslinking restores parity in JM recovery to srs2 mutants. f Crossovers and noncrossovers from crosslinked samples. g Detection of JMs, as in (a), from JM resolution-defective ndt80 mutants. h Quantification of gels. n = 2; error bars denote range. Total JM appearance in srs2 mutants is delayed and reduced ~ 2-fold, but mcJMs are similar in SRS2 and srs2. i fraction of JMs that are mcJMs

We considered two possible explanations for how steady-state levels of JMs could be reduced so markedly without substantially affecting CO levels. First, JM resolution might be accelerated, such that the average JM lifespan in srs2 mutants was four to eight times shorter than in wild type. Second, JMs formed in srs2 mutants might contain structural differences (such as nicked Holliday junctions) that make them unstable, either in vivo or during the DNA purification protocol used here. To test the first suggestion, JMs were measured in DNA isolated from resolution-defective ndt80∆ mutants using the same protocol, and were found to be both delayed and substantially reduced in srs2 ndt80∆ relative to SRS2 ndt80∆. Thus, at least some of the difference between SRS2 and srs2 must be due to factors that affect JM structure or stability, rather than resolution. Consistent with this suggestion, loss of Srs2 activity resulted in a substantial increase (1.6-fold, average of 6–9 h) in the fraction of JMs in resolution-defective ndt80∆ mutants that contained more than two chromatids (multichromatid JMs; Fig. 8).

To test the second suggestion of increased lability of JMs formed in srs2 mutants, the DNA isolation protocol was modified to include psoralen crosslinking, which has the potential to preserve otherwise unstable intermediates (Kaur et al. 2018). The addition of psoralen crosslinking resulted in recovery of JMs in similar levels from SRS2 and srs2 strains (Fig. 8e), supporting the suggestion that Srs2 activity is important for normal JM formation and stability.


While multiple studies have examined roles for the multifunctional S. cerevisiae helicase Srs2 in DNA replication, repair and recombination during the mitotic cell cycle (Niu and Klein 2017), considerably less is known about Srs2’s function during meiosis. Previous studies had shown that loss of Srs2 activity causes delays and defects in meiotic nuclear division, as well as reduced sporulation and spore viability (Palladino and Klein 1992; Sasanuma et al. 2013b). Our current study and an accompanying study (Sasanuma et al. 2019) have identified recombination abnormalities in meiosis I prophase that are likely the cause of abnormal nuclear division in srs2 mutants.

We find that srs2 mutants display multiple meiotic defects at both the cellular and molecular level, regardless of whether the mutants examined confer a chronic loss of Srs2 activity (srs2∆ and srs2-101) or a loss of Srs2 specifically during meiosis (srs2-md). These and other srs2 mutant phenotypes are Spo11 dependent (Fig. S2a, c; Fig. 4; Sasanuma et al. 2019), indicating that abnormal recombination intermediates are a likely cause. A minority of srs2 mutant cells (21–27%) do not divide their nuclei (Fig. 1) and do not separate SPBs (Fig. 2c), consistent with a DNA damage-induced meiotic progression arrest before exit from pachytene. Cells that do exit from pachytene and progress to nuclear division do so with an ~ 1 h delay (Fig. 1), even though SPB separation occurs with normal timing during meiosis I and meiosis II (Fig. 2b, c). These cells display DNA bridges (Fig. 1f), sister centromere separation without nuclear division (Fig. 3), meiosis II SPB separation and spindle formation within a single nuclear mass (Fig. 2d, e) and substantial spore inviability (Fig. 1g, h). These latter phenotypes suggest frequent recombination-dependent chromosome entanglements preventing nuclear division, as is observed in other mutants that are unable to properly resolve recombination intermediates (De Muyt et al. 2012; Jessop and Lichten 2008; Kaur et al. 2015; Oh et al. 2008; Tang et al. 2015). In summary, the pleotropic nature of the meiotic nuclear division defects seen in srs2 mutants are consistent with abnormal recombination intermediates being present both before and after cells exit from pachytene.

Persistent abnormal recombination intermediates in srs2 mutants

Srs2 is thought to disrupt or prevent formation of Rad51-containing nucleoprotein filaments during the mitotic cell cycle (Niu and Klein 2017). The observation of persistent Rad51 aggregates in srs2 mutants (Fig. 4; Sasanuma et al. 2019) suggests that Srs2 has a similar function during meiosis. Interestingly, while aggregate formation does not require progression through meiosis I (Sasanuma et al. 2019), the absence of aggregates from ndt80∆ mutants, and from NDT80 cells with foci or linear arrays of the SC protein Zip1 (Figs. 5b and 6; Sasanuma et al. 2019), indicates that Rad51 aggregates do not form until cells have exited from pachytene and disassembled SC. Rad51 strand exchange activity is inhibited before pachytene exit (Subramanian et al. 2016), and Rad51 aggregate formation is greatly reduced in srs2 rad51-II3A mutants (Fig. 5b), which can form Rad51-DNA filaments but not catalyse strand exchange activity (Cloud et al. 2012). Thus, the appearance of Rad51 aggregates after exit from pachytene indicates that Rad51 strand exchange activity is necessary for this srs2 mutant phenotype. Notably, the frequent colocalisation of aggregates of Rad51 and the RPA subunit Rfa1, observed in srs2 mutants but rarely during normal meiosis (Fig. 7), suggests these aggregates form on abnormal recombination intermediates, most likely associated with stalled recombination events that are impeding normal nuclear division.

We applied two tests to determine if the Rad51 aggregates were likely to be associated with normal or abnormal recombination events. First, we deleted the Mek1 kinase, which during normal meiosis directs repair of Spo11-DSBs away from the sister chromatid and towards the homologue (Callender et al. 2016; Niu et al. 2005; Niu et al. 2009). Secondly, we deleted Sae2, which is required for resection of Spo11-DSB ends during meiosis I prophase (McKee and Kleckner 1997; Prinz et al. 1997). Rad51 aggregation still occurred in mek1∆ srs2 and in sae2∆ srs2 (Fig. 5a, c), indicating that neither interhomologue strand invasion nor Sae2-mediated single-strand resection are required for post-pachytene Rad51 aggregation in srs2 cells. Of particular note is the accumulation of Rad51 aggregates in resection-defective sae2∆ srs2 mutants; to account for this aggregate formation, we suggest that post-pachytene activation of Sae2-independent resection or helicase activities expose ssDNA at previously unresected DSBs, which can then participate in Rad51-mediated strand invasion.

In summary, these observations further support the hypothesis that the cytologically visible phenotypes of srs2 mutants might reflect the loss of suppression of Rad51 activity after pachytene (Fig. 9). Rad51 then decorates ssDNA from either or both the abnormal processing of normal intermediates created before and remaining after pachytene or abnormal recombination intermediates created after pachytene.
Fig. 9

Control of Rad51 aggregation during meiosis. During pachytene and earlier stages of meiosis, Rad51 activity is inhibited by two mechanisms. In one, meiotic DSBs activate the Mek1 kinase, stabilising Hed1, which in turn prevents association of the Rad54 cofactor with Rad51. In the second, Srs2 removes excess Rad51, limiting Rad51 accumulation to foci at DSBs. After exit from pachytene, DSBs are absent and Mek1-Hed1 dependent inhibition of Rad51 is inactive but the Rad51-removing activity of Srs2 remains, preventing accumulation of Rad51 on chromatin. In srs2 mutants, neither Mek1-Hed1 nor Srs2-dependent mechanisms prevent Rad51 accumulation on chromatin and aggregates accumulate

The question remains open as to whether these abnormal intermediates arise as a consequence of srs2 mutant defects during early meiosis I prophase, when recombination normally occurs, or as a consequence of aberrant processing of residual lesions present after exit from pachytene, at the time when most DSB repair is complete.

Early defects in recombination intermediate formation in srs2 mutants

Analysis of recombination intermediates at a URA3-ARG4 recombination reporter revealed that, DSBs are formed and repaired with normal kinetics in srs2 mutants (Fig. S3b), and both crossover and noncrossover recombinants were formed in srs2 mutants at levels approximating those seen in wild type. Thus, in contrast with what is seen in studies of vegetatively growing cells, Srs2 does not appear to have either pro- or anti-crossover function during meiosis. However, JMs, which are crossover precursors, were recovered from srs2 mutants at reduced levels when DNA was extracted using a protocol that uses multivalent cations to stabilise JMs but at normal levels when DNA was also psoralen-crosslinked before extraction (Fig. 8). This suggests that the JMs present in srs2 mutant cells have structures differing from those in wild type, and that the former are differentially lost during extraction in the absence of crosslinking. Loss of Srs2 activity results in both delays and reductions in recovery of stable JMs accumulating in resolution-defective ndt80 cells, and the proportion of multichromatid JMs, which form when DSB ends interact with more than one repair template (Oh et al. 2007), is also increased. These findings suggest that many of the JMs formed in srs2 mutants have less-stable structures than JMs formed in wild-type cells, possibly reflecting a failure to form fully ligated double Holliday junctions. These unstable JMs may be derived from a yet uncharacterised Srs2-dependent, Dmc1-independent pathway for meiotic DSB repair, suggested by observations that more unrepaired DSBs accumulate in srs2 dmc1 double mutants than in SRS2 dmc1 (ASHG and T-CC, unpublished observations).

Concluding remarks

Taken together, our data and the data of Sasanuma et al. (Sasanuma et al. 2019) indicate that Srs2 has an important role in recombination biochemistry throughout meiosis I prophase (Fig. 9). We propose that a major function of Srs2 during meiosis is to limit residency of Rad51 on Spo11-initiated DSBs. In the absence of Srs2 activity, increased Rad51 occupancy may reduce the ability of DSB ends to complete dHJ formation, both because fewer binding sites are available for Dmc1 filament formation, and because Rad51 strand invasion activity is inhibited during early meiosis I prophase (Busygina et al. 2008; Callender et al. 2016; Niu et al. 2009; Tsubouchi and Roeder 2006). When srs2 mutant cells exit from pachytene, relief of this inhibition (Subramanian et al. 2016) might allow transient formation of fully ligated dHJ intermediates before resolution as crossovers; alternatively, recombination intermediates formed in srs2 mutants may not be fully ligated but can still can be resolved as COs upon exit from pachytene (Whitby 2005). We also suggest that, in srs2 mutants, Rad51 aggregates that form upon exit from pachytene reflect the persistence of lesions that seed further Rad51 accumulation in the absence of Srs2 translocase; whether these are aberrant events normally resolved by Srs2, unresolvable intermediates formed before exit from pachytene, or intermediates formed de novo by DSBs present after pachytene exit, remains to be determined. The frequent, Spo11-dependent formation of Rad51 aggregates in srs2 sae2 mutant cells (Fig. 5c), which are not expected to undergo resection or strand invasion before exit from pachytene, most likely reflects such post-pachytene DSB processing, either through DSB end destabilisation by high Rad51 residency or through end resection by nucleases or other activities that are derepressed after pachytene exit.

Srs2 belongs to the highly conserved UvrD helicase family, which has at least one representative in most organisms (Lorenz 2017; Niu and Klein 2017). Loss of the Srs2-like Fbh1 protein in Schizosaccharomyces pombe, which also has Rad51 removal activity, confers meiotic defects similar to those seen in budding yeast, including reduced spore viability, meiotic nuclear division defects, and persistent Rad51 foci, without affecting frequencies of crossovers or noncrossovers among viable progeny (Sun et al. 2011). Interestingly, the human Fbh1 orthologue, when expressed in budding yeast, suppresses many of the mitotic recombination defects and DNA damage sensitivity of srs2 mutants, suggesting that hFBH1 may have Rad51-removing activity, as well (Chiolo et al. 2007). It will be of considerable interest to determine the molecular defects underlying the similar mutant phenotypes of budding yeast srs2 and fission yeast fbh1 mutants, and to determine if the vertebrate protein has similar functions.

Materials and methods

Yeast strains

All yeast strains (Supplementary Table S1) are derived from SK1 (Kane and Roth 1974) by either transformation or genetic crosses. The srs2-md meiotic depletion allele (pCLB2-3HA-SRS2) inserts CLB2 promoter sequences and a triple influenza hemagglutinin epitope tag immediately upstream of SRS2 coding sequences and was constructed by amplification of pCLB2-3HA sequence from pAG335 (a gift from Monica Boselli) with primers containing 50 nt targeting the SRS2 locus. Srs2Clb2ptagF: GAGTATCATTCCAATTTGATCTTTCTTCTACCGGTACTTAGGG ATAGCAAtcgatgaattcgagctcg; Srs2CClb2ptagR: GTATTTAACTGGGATACTAAATGCAACCAAAGATCATTGTTC GACGACATgcactgagcagcgtaatctg, where lowercase letters correspond to plasmid sequences. CNM67-mCherry and GFP-TUB1 tag constructs were from AMY6969 and AMY6706, respectively (a gift from Adele Marston). Zip1-GFP has been described (White et al. 2004). The RFA1-GFP allele inserts GFP sequences immediately downstream of RFA1 coding sequences and was constructed by amplification of GFP sequence from pKT127 (Sheff and Thorn 2004) with primers containing 50 nt targeting the RFA1 locus: RFAChrGFP_F: GGGCTGAAGCCGACTATCTTGCCGATGAGTTATCCAAGGCTTTGTTAGCTggtgacggtgctggttta; RFAChrGFP_R: TTTCTCATATGTTACATAGATTAAATAGTACTTGATTATTTGATACATTAtcgatgaattcgagctcg, where lowercase letters correspond to plasmid sequences.

Spore viability

Spore viability was determined by tetrad dissection. Diploid strains were sporulated 1–3 days, 30 °C in patches on 1% (w/v) potassium acetate, 2% (w/v) agar plates, digested 15 min, 30 °C in 1 M sorbitol, 1% (w/v) glucose, 1 mg/ml zymolyase, dissected on YPAD agar (2% peptone, 1% yeast extract, 2% glucose, 0.004% adenine, 2% agar, all w/v) and incubated for 2 days at 30 °C.

Liquid sporulation

All incubation temperatures were 30 °C. All media components are w/v unless otherwise indicated. For cytological studies, an overnight YPAD broth culture, inoculated with a single colony on YPAD agar, was grown with aeration overnight, and then was diluted to an OD600 of ~ 0.3 in BYTA (1% yeast extract, 2% tryptone, 1% potassium acetate, 50 mM potassium phthalate) and incubated with aeration for 16 h. The culture was harvested by centrifugation, washed with 200 ml 1% potassium acetate, resuspended in 250 ml SPM (0.3% potassium acetate, 0.02% raffinose) with appropriate supplements to a final OD600 of ~ 1.9, and incubated with vigorous aeration. For molecular studies, sporulation in liquid was as described (Oh et al. 2009), using the ‘Lichten’ protocol.

Cytological methods

Nuclear divisions

Of a culture, 0.5 ml was mixed with 0.75 ml ethanol and stored at − 20 °C; 1 μl of 0.5 mg/ml 4′,6-diamidino-2-phenylindole (DAPI) was added, and samples were incubated at room temperature for 30 s. Cells were harvested by centrifugation, resuspended in 0.2 ml 50% glycerol, sonicated briefly if necessary to break up clumps and examined by epiflouresence microscopy. Cells with two nuclei were scored as having completed meiosis I and cells with three or four nuclei as having completed meiosis II.

Recombination protein foci

Of a culture, 4.5 ml was harvested by centrifugation and resuspended to 0.5 ml in 1.0 M sorbitol, pH 7. 1,4-Dithiothreitol and zymolyase were added to 24 mM and 0.14 mg/ml, respectively, and cells were spheroplasted by incubation at 37 °C for 20 to 45 min with agitation, until the majority of cells lysed when mixed with an equal volume of 1.0% (w/v) sodium N-lauroylsarcosine; 3.5 ml of Stop Solution (0.1 M MES, 1 mM EDTA, 0.5 mM MgCl2, 1 M sorbitol, pH 6.4) was added; cells were harvested by centrifugation, resuspended in 100 μl Stop Solution and distributed between four ethanol-cleaned glass microscope slides. Twenty microlitres of fixative (4.0% (w/v) formaldehyde, 3.8% (w/v) sucrose, pH 7.5) was added to each slide, followed by 40 μl of 1% Lipsol with light mixing. A further 40 μl of fixative was added, and the mixture was spread across the slide. All subsequent steps were at room temperature, unless otherwise indicated. Slides were incubated for 30 min in a damp chamber, and then allowed to air dry. Once dry, slides were washed in 0.2% (v/v) PhotoFlo (Kodak) and then in water and allowed to air-dry slightly. Slides were washed once in 0.025% Triton X-100 in phosphate-buffered saline (PBS) for 10 min and twice for 5 min in PBS. Slides were blocked with 5% skimmed milk (Sigma) in PBS for 1–4 h at 37 °C; excess liquid was removed and slides were placed horizontally in a damp chamber. Mouse anti-yeast Rad51 antibody (Santa Cruz, sc-133,089, 1:200 in 1% skim milk, PBS) was added at 150 μl/slide, and slides were incubated at 4 °C overnight. Slides were washed three times in PBS (5 min each) and incubated with secondary antisera (AlexaFluor594-conjugated goat anti-mouse antibody; Life Technologies A11005; 1:1000 in 1% skimmed milk, PBS), 150 μl per slide, for 1–2 h in a damp chamber. Slides were washed three times with PBS (5 min each), cover slips were affixed using Vectashield mounting medium with DAPI (Vector Laboratories), sealed with clear varnish and imaged on a DeltaVision microscope (z = 12–15, exposure times: RD-TP-RE = 1.0 s, DAPI = 0.05–1.0 s, FITC = 1.0 s for Rfa1-GFP colocalisation experiments). Images were deconvolved by SoftWoRx software using standard settings and the number of cells with Rad51 or Rfa1 foci or aggregates counted. Aggregates were identified as being at least 6 pixels (0.39 μm) wide, using ImageJ software.

Spindle pole bodies

To reduce disruption of the DAPI signal during the spreading process, cells were formaldehyde-fixed before spheroplasting; 0.5 ml of 37% (v/v) formaldehyde was added to 4.5 ml of meiotic culture, and cells were incubated at room temperature for 30 min. Cells were harvested by centrifugation, washed with 5 ml 1% (w/v) potassium acetate and were then processed as above for recombination protein detection through the PhotoFlo/water wash steps. Cover slips were affixed using Vectashield mounting medium with DAPI (Vector Laboratories), sealed with clear varnish and imaged on a DeltaVision microscope (z = 12–24, Exposure times: FITC = 1.0 s, RD-TP-RE = 1.0 s, DAPI = 0.05–1.0 s). Images were deconvolved by SoftWoRx software using standard settings and the number of RFP (SPB) foci and DAPI signals per cell were counted, using GFP tubulin as an additional signal where necessary.

Recombination intermediate and product analysis

DNA was extracted, displayed on Southern blots and hybridised with radioactive probe as described, either without (Oh et al. 2009); ‘Lichten lab’ protocol) or with prior psoralen crosslinking (Kaur et al. 2018). JMs were detected using XmnI digests probed with + 156 to + 1413 of ARG4 coding sequences. DSBs, NCOs and COs were detected using EcoRI-XhoI digests probed with + 539 to + 719 of HIS4 coding sequences. Radioactive signal on blots was detected using either a Fuji LAS-3000 or a GE Typhoon FLA-9500 phosphorimager and was quantified using Fuji Image Guage v4.22 software.

Protein extraction and western blots

Samples containing 5–10 OD600 of cells were harvested by centrifugation, washed in 1 ml water, and flash frozen in liquid nitrogen. The pellet was stored at − 80 °C for at least 2 h and was then resuspended in 150 μl of 1.85 M NaOH, 7.5% (v/v) β-mercaptoethanol and incubated on ice for 15 min. One hundred fifty microlitres of 55% trichloroacetic acid was added, and cells were incubated for a further 10 min. Cells were harvested by centrifugation for 10 min at top speed in a microfuge and resuspended in 250 μl of 200 mM Tris-HCl at pH 6.5, 8 M urea, 5% (w/v) SDS, 1 mM EDTA, 0.02% bromophenol blue, 5% (v/v) β-mercaptoethanol, with 10 μl of 25× protease inhibitor stock (Roche, 04693132001). If necessary, 10 μl of 1.5 M Tris HCl at pH 8.8 was added to maintain pH, as shown by the blue indicator in the suspension. Cells were heat shocked at 65 °C for 10 min, centrifuged for 1 min at top speed in a microfuge, and the supernatant was harvested. Protein samples were denatured at 95 °C for 5 min in appropriate loading buffer and loaded into precast SDS-PAGE gels (10% polyacrylamide; Biorad). Gels were run at 40 mA for 45 min in 1× running buffer (Fisher). Gels were assembled into a sandwich with Hybond C nitrocellulose membrane (Amersham) and Whatman 3MM blotting paper, and gel contents were transferred by semi-dry transfer (Thermo Scientific Pierce Power Blotter) using Pierce 1-Step Transfer Buffer for 7 min or by wet transfer in 0.025 M Tris Base, 0.15 M Glycine, 2% (v/v) methanol at 150 mA for 2 h or at 16 V overnight (Biorad MiniProtean Tetra Cell). Membranes were rinsed in water. If necessary, the membrane was incubated 30 s in Ponceau stain (Sigma), and then washed in PBST (Sigma). Membranes were incubated in 5% (w/v) skimmed milk in PBS at 4 °C for 2–20 h, then incubated in primary antibody in 1% (w/v) skimmed milk in PBS at the following concentrations for 2–20 h at 4 °C (anti-Srs2, Santa Cruz sc-1191, 1:2000; anti-PSTAIR, Sigma P6962, 1:2500). Membranes were washed 3× in PBS, 5 min each at RT, and incubated in horseradish peroxidase-conjugated secondary antibody in 1% (w/v) skimmed milk in PBS at the following concentrations for 30–120 min at RT (anti-goat, Santa Cruz sc-2020, 1:2500; anti-mouse, Santa Cruz sc-2005, 1:2500). Membranes were washed 3× in PBS, 5 min each at RT, incubated with 2 ml high sensititivity ECL detection solution (Millipore) and blots were visualised on a GeneGnome chemiluminsescence imaging system.



We thank Douglas Bishop, Monica Boselli, Bin Hu, Adele Marston and Akira Shinohara for strains, reagents, discussion and communication of results in advance of publication and Matan Cohen for technical assistance in preparing DNA samples. Imaging was performed using the DeltaVision microscope at the Wolfson Light Microscopy Facility, University of Sheffield. This work was supported by BBSRC BB/K009346/1 to ASHG and by the Intramural Research Program at the Center for Cancer Research, National Cancer Institute, National Institutes of Health.

Supplementary material

412_2019_705_MOESM1_ESM.jpeg (163 kb)
Supplementary Fig. S1 Srs2 loss during meiosis in srs2-md strains. Protein samples from mitotic (YPAD overnight), premeiotic (BYTA) or sporulation (SPM) cultures of SRS2 or srs2-md strains were displayed on SDS-PAGE gels, transferred to nitrocellulose and probed with anti-Srs2 or anti-PSTAIR as described in ‘Materials and methods’. Cells were shifted to SPM after 17 h of presporulation growth in BYTA. (JPEG 163 kb)
412_2019_705_MOESM2_ESM.jpg (223 kb)
Supplementary Fig. S2 a Progression defects in srs2 mutant cells require Spo11-induced double strand DNA breaks. While srs2-101 and srs2-md mutants show a failure to complete meiosis II, srs2-101 spo11-Y135F and srs2-md spo11-Y135F double mutants, which fail to form meiotic DSBs, restore progression to near wild-type levels (srs2-md spo11-Y135F, n = 3; srs2-101 spo11-Y135F, n = 2; data for SPO11 strains from Fig. 1). b Progression through meiotic nuclear divisions, expressed as percent of cells completing meiosis II, is similar in the presence (+ tags) or absence of CNM67-mCherry and GFP-TUB1 (SRS2 + tags, n = 2; srs2-101 + tags, n = 2; error bars—range; data for untagged strains from Fig. 1). c Rad51 aggregates form in srs2-101 mutants. (srs2-101, n = 3; srs2-101 spo11, n = 3; data for SRS2 from Fig. 4; error bars—standard error of the mean) (JPG 222 kb)
412_2019_705_MOESM3_ESM.jpeg (212 kb)
Supplementary Fig. S3 a Recombination reporter system used to detect recombination intermediates in XmnI digests and products in EcoRI/XhoI double digests (Jessop et al. 2005; Jessop and Lichten 2008). Grey arrows—URA3 and ARG4 genes; white box—63 nt telomere repeat sequence; vertical arrow—meiotic DSB hotspot. Inserts are at LEU2 (red) on one chromosome III and at HIS4 (blue) on the other. arg4-pal is an EcoRI-marked palindrome insertion for scoring noncrossovers. Relevant restriction sites are indicated. EcoRI/XhoI digests detect DSBs, NCO and CO products. XmnI digests detect interhomologue (IH-dHJs) and intersister double Holliday junctions (IS-JMs) and multichromatid JMs (mcJMs, only one example of many possible is shown). Schematic reproduced from Kaur et al. (2015); illustrative Southern blots are from an SRS2 diploid. b)DSB dynamics are not altered in srs2 mutants. DSBs were measured on Southern blots of EcoRI/XhoI digests of DNA from SRS2 (n = 5, data from De Muyt et al. 2012; Kaur et al. 2015 and one additional replicate; error bars denote SEM), srs2-101 (n = 5; error bars denote SEM) and srs2-md (n = 2; error bars denote range). (JPEG 211 kb)
412_2019_705_MOESM4_ESM.docx (49 kb)
Supplementary Table S1 (DOCX 49.4 kb)


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Open Access This article is distributed under the terms of the Creative Commons Attribution 4.0 International License (, which permits unrestricted use, distribution, and reproduction in any medium, provided you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made.

Authors and Affiliations

  1. 1.Department of Molecular Biology and BiotechnologyThe University of SheffieldSheffieldUK
  2. 2.Genome Damage and Stability Centre, School of Life SciencesUniversity of SussexBrightonUK
  3. 3.Immunology and Molecular Physiology Lab., Zoology Department, Faculty of ScienceAssiut UniversityMarkaz El-FathEgypt
  4. 4.Laboratory of Biochemistry and Molecular Biology, Center for Cancer ResearchNational Cancer InstituteBethesdaUSA
  5. 5.Department of Biochemistry and Structural Biology, UT Health San AntonioSan AntonioUSA
  6. 6.All First Tech Co., LtdTaoyuan CityTaiwan
  7. 7.Faculty of Life SciencesThe University of BradfordBradfordUK

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