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Spontaneous mitotic recombination is a potential source of genetic changes such as loss of heterozygosity and chromosome translocations, which may lead to genetic disease. In this study we have used a rad52 hyper-recombination mutant, rad52-Y66A, to investigate the process of spontaneous heteroallelic recombination in the yeast Saccharomyces cerevisiae. We find that spontaneous recombination has different genetic requirements, depending on whether the recombination event occurs between chromosomes or between chromosome and plasmid sequences. The hyper-recombination phenotype of the rad52-Y66A mutation is epistatic with deletion of MRE11, which is required for establishment of DNA damage-induced cohesion. Moreover, single-cell analysis of strains expressing YFP-tagged Rad52-Y66A reveals a close to wild-type frequency of focus formation, but with foci lasting 6 times longer. This result suggests that spontaneous DNA lesions that require recombinational repair occur at the same frequency in wild-type and rad52-Y66A cells, but that the recombination process is slow in rad52-Y66A cells. Taken together, we propose that the slow recombinational DNA repair in the rad52-Y66A mutant leads to a by-pass of the window-of-opportunity for sister chromatid recombination normally promoted by MRE11-dependent damage-induced cohesion thereby causing a shift towards interchromosomal recombination.
In living cells, DNA damage occurs as a result of cell metabolism, developmental processes and exogenous sources such as chemical agents or radiation. Repair of DNA damage is essential to prevent chromosome loss and cell death. In the budding yeast Saccharomyces cerevisiae, homologous recombination (HR) is the major pathway for repair of DNA double-strand breaks (DSBs). However, although DSBs are recombinogenic, they do not appear to be the main source of spontaneous mitotic HR [1,2]. Hence, mutants exist that recombine at wild-type or higher levels despite the fact that they are defective in DNA DSB repair. The nature of the lesions provoking HR is still poorly defined, but understanding the phenotype of mutants that separate DNA DSB repair from spontaneous HR will likely provide clues to the mechanisms of spontaneous HR. Many of the genes involved in this process were identified in yeast by screening for mutants sensitive to ionizing radiation . These mutants constitute the RAD52 epistasis group and include RAD50, RAD51, RAD52, RAD54, RAD55, RAD57, RAD59, RDH54, RFA1, MRE11 and XRS2 [4,5]. Amongst these genes in S. cerevisiae, disruption of RAD52 causes the most severe recombination defect.
The Mre11-Rad50-Xrs2 complex (MRX) is one of the earliest proteins detected at a DSB . The recruitment of MRX to a DSB results in a high local concentration of the complex as visualized by fluorescence microscopy as Mre11 focus formation . The MRX complex contributes to the initial processing of DSB ends into 3' single-stranded DNA (ssDNA) tails [7–10], which are essential for copying genetic information from an intact donor sequence during homologous recombination. Furthermore, recent studies have shown that the MRX complex is required for the postreplicative reestablishment of cohesion in response to genotoxic stress [11–14]. Notably, mre11 results in hyper-recombination between interchromosomal heteroalleles, but not between sister chromatids [15–18]. Importantly, the association of MRX with a DSB is transient and the dissociation of MRX from the site of DNA damage is concurrent with the appearance of ssDNA and recruitment of the Rad52 mediator protein , which in turn recruits the Rad51 recombinase to catalyze strand-invasion.
DSBs promote mitotic recombination and result in reciprocal exchange or gene conversion events [19,20]. Frequencies of gene conversion are highest near DSBs . Moreover, conversion tracts are usually continuous and if multiple markers at a DNA DSB are involved, a central marker is almost always co-converted if the flanking markers are converted [21–26]. Gene conversion in yeast involves mismatch repair (MMR) of heteroduplex DNA (hDNA) for both meiotic [27,28] and mitotic events [29–33]. Thus, the amount of homology at the DSB-ends, the direction of mismatch repair and the length of hDNA greatly influence recombinational repair.
The RAD52 epistasis group is also important for spontaneous mitotic recombination although this process is less well characterized and the requirements for individual genes depend on the assay suggesting the existence of multiple pathways [4,5]. Importantly, Rad52 is essential for all types of spontaneous mitotic recombination, whereas Rad51 function is required only for some types of recombination. Finally, genes outside of the RAD52 epistasis group also affect spontaneous mitotic recombination as illustrated by a recent genome-wide analysis of the genetic control of Rad52 foci . Some of these genes that affect recombination include factors that contribute to chromosome integrity by maintaining chromatin architecture and organization, regulating cell cycle and spindle checkpoints, and repairing DNA lesions via other pathways.
To gain insight into the mechanism(s) of spontaneous mitotic recombination, we analyzed the phenotype of a rad52-Y66A mutant that blocks the repair DNA damage induced by γ-irradiation, but is proficient for spontaneous mitotic recombination at a rate higher than wild type. This allele was generated by site-directed mutagenesis in an alanine scan of the conserved N terminus of Rad52 . It was subsequently shown that rad52-Y66A cells are deficient in the repair of a single DSB induced during mating-type switching and are sensitive to a top1-T722A mutation, which causes the accumulation of covalent topoisomerase-DNA intermediates that are frequently converted to DSBs . Further, the rad52-Y66A mutant is proficient for UV-induced heteroallelic recombination. The data presented here suggest that the rad52-Y66A hyper-recombination phenotype may result from a slowdown in DNA repair that leads to a loss of damage-induced cohesion prior to completion of repair, causing a shift from sister chromatid to interchromosomal recombination.
Yeast strains were manipulated using standard genetic techniques and media was prepared as described previously except that twice the amount of leucine was used (60mg/L) . All strains used in this study are listed in Table 4 and all are RAD5 derivatives of W303 [37,38]. Other genetic markers have been described previously .
The ctf4kanMX6 allele was amplified from the available yeast gene deletion library strain  using primers 5'-CATCCTCTTCATGTACTACTTATGTCCA and 5'- AAGAAATAAAGAACTTTGAATTGATGC. The resulting PCR was transformed into W1588-4C . The strategy for making a marker-free rad51 null (rad51Δ) strain was described previously . The mre11LEU2 and msh2URA3 alleles were kindly provided by Dr. Lorraine Symington. The msh2ura3HIS3 allele was made by transforming the msh2URA3 strain with the “marker swap” pUH7 plasmid .
A CEN-based plasmid harboring the ade2-n allele was constructed by first cloning an ADE2-containing BglII fragment from pRS417  into BamHI-digested YCp50 resulting in pWJ1190. Next, the ade2-n allele was gap-repaired onto AflII-digested pWJ1190 by transformation into W4091-4C resulting in plasmid pWJ1441.
To construct the single-copy pRS413-RAD52-YFP and pRS413-rad52-Y66A-YFP plasmids marked with HIS3, the RAD52 and rad52-Y66A alleles were first subcloned from pWJ646  and its Y66A derivative to the pRS413 vector  using restriction enzymes XhoI and XmaI. Next, gap-repair was used to move the yellow fluorescent protein (YFP) encoding sequence onto the linearized plasmids by transformation into strain W3749-14C to produce pRS413-RAD52-YFP and pRS413-rad52-Y66A-YFP.
Interchromosomal (C × C) recombination between non-functional ade2 heteroalleles was measured in diploid strains. The pair-wise combinations used for the analysis were ade2-n × ade2-a, ade2-1 × ade2-a and ade2-1 × ade2-n. The ade2 heteroalleles were previously described . Cells were plated on SC and SC-Ade plates.
Chromosome-plasmid (C × P) recombination was measured in a haploid strain carrying the ade2-a heteroallele at the endogenous site and the ade2-n heteroallele on a single-copy plasmid (pWJ1441). Cells were plated on SC-Ura and SC-Ura-Ade plates.
The procedure for measuring the rate of heteroallelic recombination was as described previously , except that the single colonies were inoculated into liquid media. The plating efficiency and the number of recombinants were determined by plating an appropriate number of cells. For each strain, eight to 20 independent trials were carried out and the corresponding recombination rates and their standard deviations were calculated according to the median method .
Recombination was also analyzed in patches of cells grown at 30°C for two days and replica-plated onto the appropriate selective media. The plates were scanned after a four-day incubation. RAD52/RAD52, RAD52/rad52-Y66A and rad52-Y66A/rad52-Y66A diploid cells were patched onto SC plates and replica-plated onto SC-Ade plates. Haploid and diploid strains transformed with pWJ1441 were patched onto SC-Ura plates and replica-plated onto SC-Ura-Ade.
Three to five trials were performed to measure γ-ray sensitivity of each haploid and diploid strain. Cells were grown in liquid YPD medium to a cell density of 107 cells/ml and briefly sonicated. Unless otherwise noted, the plates were incubated at 30°C for 3 days and the surviving colonies counted. Survival curves were produced as previously described .
Survival after UV-irradiation was measured in haploid and diploid strains by spot assays. Cells were grown in liquid SC-Leu media and exponential cultures were sonicated before plating. Ten-fold serial dilutions were made and 5 μl from each concentration was spotted onto SC-Leu plates prior to irradiation.
Cells were grown in liquid medium and analyzed by fluorescence microscopy as described . Live cell images were captured with a cooled Orca-ER CCD camera (Hamamatsu, Japan) mounted on a Zeiss Axioplan II microscope (Carl Zeiss, Thornwood, NY). All images were captured at 100-fold magnification using a Plan-Apochromat 100x, 1.4 NA objective lens. The illumination source was a 100W mercury arc lamp (Osram, Munich, Germany). For each field of cells, eleven fluorescent images at the relevant wavelength were obtained at 0.3 μm intervals along the Z-axis to allow inspection of all focal planes of nuclei. YFP was visualized using a band-pass filter set (Cat. # 41028, Chroma, Brattleboro, VT). Images were acquired with a 2% (time-lapse experiments) or 10% neutral density filter in place to reduce photobleaching. Image acquisition time for Rad52-YFP and Rad52-Y66A-YFP were 1000ms. Images were acquired using OpenLab software (Improvision, Lexington, MA).
A t-test was used to determine the significance of differences for the recombination rates between the different strains and for γ-ray survival differences between haploid and diploid strains. For the percentage of cells with a Rad52-YFP focus, the significance was determined by chi-square analysis.
To explore further the mechanism of spontaneous mitotic recombination, we analyzed the hyper-recombination phenotype of a γ-ray sensitive rad52-Y66A mutant . Heteroallelic recombination was measured for diploid wild-type, rad52-Y66A and rad52Δ strains using two previously described non-functional ade2 heteroalleles, ade2-a and ade2-n . Two assays were used to measure the rate of prototroph formation due to recombination between two interchromosomal heteroalleles (C × C) in diploid strains (Fig. 1A) and between chromosomal and plasmid sequences (C × P) in haploid strains (Fig. 1B), respectively. Compared to a wild-type strain, a rad52Δ strain has about a 100-fold lower rate of C × C recombination. In contrast, rad52-Y66A has an eight-fold increase in C × C recombination compared to wild type (Table 1). The hyper-recombination phenotype of rad52-Y66A is recessive since recombination in a heterozygous RAD52/rad52-Y66A diploid is comparable to that of the wild-type strain (Fig. 1C(I)). For the wild-type strain, the rate of spontaneous C × P recombination is ten-fold lower than for C × C recombination indicating that the genomic context of the heteroalleles is important for their availability during mitotic recombination (Tables 1 and and2).2). Spontaneous recombination in the C × P assay is reduced by more than 20-fold in a rad52Δ strain compared to wild type indicating that Rad52 function is required for C × P recombination (Table 2). Interestingly, the C × P recombination rate of rad52-Y66A is not significantly different from the wild type indicating that the rad52-Y66A hyper-recombination phenotype is specific to the C × C recombination assay.
It is possible that the difference between C × C and C × P recombination may be due to ploidy or heterozygosity at the mating-type locus. C × C recombination was measured in a MATa/MATα diploid strain whereas C × P recombination was determined in a MATa haploid strain. Both MATα rad52-Y66A ade2-a haploid and MATa/MATα rad52-Y66A/rad52-Y66A ade2-a/ade2-a diploid strains were transformed with a plasmid containing the ade2-n heteroallele and spontaneous recombination assayed in patches of cells. This experiment shows that the recombination levels in both strains are comparable to that of the MATa rad52-Y66A ade2-a haploid transformed with the same plasmid (Fig. 1C(II)). This result indicates that the lower rate of recombination between the C × P heteroalleles in a haploid strain is not mating-type specific nor due to ploidy.
Further, homozygous RAD52, rad52-Y66A and rad52Δ diploid and haploid strains were analyzed for their ability to repair γ-ray induced DNA damage (Fig. 1D). Survival curves show that both haploid and diploid rad52-Y66A strains are more sensitive to ionizing radiation than the wild type. In addition, both wild-type and rad52-Y66A diploids are significantly more resistant to γ-ray induced damage than the respective haploid strains, which is in contrast to the rad52Δ diploid that is more sensitive than the haploid (Fig. 1D). Further, we found that additional slow growing survivors of the irradiated rad52Δ diploid cells appear after 6 days. However, based on marker loss analysis these colonies are likely to have lost whole chromosomes as a result of the induced DNA damage rather than reflecting its repair. Although recombinational repair of DSBs occurs preferentially from the sister chromatid , a reasonable explanation for the increased resistance to γ-rays in the wild-type and rad52-Y66A diploid strains is that the repair of induced DSBs is additionally aided by the presence of the homologue. Taken together, the hyper-recombination phenotype of rad52-Y66A is independent of ploidy and is specific for heteroallelic recombination between chromosomes (C × C assay). A possibility is that recombination between C × C and C × P heteroalleles may have distinct requirements for RAD52.
To determine whether the difference between C × C and C × P recombination is specific to rad52-Y66A, we tested another hyper-recombination mutant from the RAD52 epistasis group. Compared to a wild-type strain, spontaneous C × C recombination in an mre11Δ mutant is induced eight- to ten-fold . This recombination rate is not increased further by the presence of the rad52-Y66A mutation (Table 1). Interestingly, C × P recombination in mre11Δ or rad52-Y66Amre11Δ is not significantly different from wild-type levels (Table 2). These data indicate that mre11Δ and rad52-Y66A display similar context-dependent hyper-recombination.
Since the difference between the two assays is not specific to rad52-Y66A, we decided to determine the requirements of heteroallelic recombination for Rad51, a RecA homologue and another member of the RAD52 epistasis group. Unlike mre11Δ and rad52-Y66A strains, the lack of Rad51 function significantly reduces C × C recombination by 30 to 50-fold compared to the wild type . rad52-Y66Arad51Δ and mre11Δ rad51Δ double mutants are as defective for recombination as the rad51Δ single mutant (Table 2). Therefore, the C × C events leading to the rad52-Y66A and mre11Δ hyper-recombination phenotype require Rad51 function. In addition, the rate of C × P recombination in rad51Δ, rad52-Y66Arad51Δ and mre11Δ rad51Δ strains is significantly reduced demonstrating that this type of recombination also requires Rad51 activity (Table 2).
To determine if the difference between C × C and C × P recombination assays extends outside of the RAD52 epistasis group, we measured recombination rates in two other previously reported hyper-recombination mutants, ctf4 and msh2 [51,52].
Msh2 is a key factor in mismatch repair (MMR). In addition, Msh2 helps to prevent genetic recombination between divergent sequences likely by binding mismatches and interacting with the recombination machinery to block, reverse and/or destroy mismatched intermediates [28,52–54]. C × C recombination in a msh2Δ strain shows a slight, but significant increase in the rate of recombination compared to wild type (Table 1). To determine if the C × C hyper-recombination phenotype of rad52-Y66A requires Msh2 function, the rad52-Y66Amsh2Δ double mutant was analyzed. The rate of prototroph formation between C × C heteroalleles in the rad52-Y66Amsh2Δ double mutant is synergistically increased over the rates of either single mutant to 24-fold over the wild-type rate (Table 1). The synergistic effect is specific for C × C recombination as it was not observed for C × P recombination (Table 2). The rad52-Y66Amsh2Δ hyper-recombination phenotype could be due to lack of functional Rad52 activity in a msh2Δ background. To assess this possibility, a rad52Δ msh2Δ strain was analyzed in the C × C assay. Whereas the recombination rate for msh2Δ is 20 × 10−7, the rate for rad52Δ msh2Δ is only 0.2 × 10−7 (Table 1). This result indicates that recombination in a msh2Δ strain requires Rad52 function. Moreover, the synergistic effect is not caused by an additional overall defect in DNA repair efficiency as the MSH2 deletion does not significantly increase the UV- or γ-ray sensitivity of rad52-Y66A (Fig. 2). Taken together, these data indicate that rad52-Y66A and msh2Δ stimulate recombination by different mechanisms.
CTF4 is required for sister chromatid cohesion and fidelity of chromosome segregation and was recently isolated in a genome-wide screen for mutations that increase spontaneous Rad52 foci [34,55–57]. Ctf4 is also a chromatin-associated protein that interacts with DNA polymerase α and may link sister chromatid cohesion to DNA synthesis . Cohesin is assembled at the time of DNA replication at centromeres and other cohesin binding sites [59–62]. Accordingly, ctf4 mutants display increased loss rates for chromosome III as well as for an artificial centromere-based circular chromosome . Similar to rad52-Y66A and mre11Δ, deletion of CTF4 increases recombination eight-fold for the C × C assay, which is consistent with the previously reported hyper-recombination phenotype of this mutant (Table 1) . To determine whether the hyper-recombination phenotype of rad52-Y66A is affected in a ctf4Δ background, the double mutant was analyzed. The C × C recombination rate of rad52-Y66A ctf4Δ is not significantly different from the rad52-Y66A rate. In addition, unlike the results obtained for rad52-Y66A and mre11Δ, ctf4Δ has an eight-fold increase over wild type levels for C × P recombination. This rate is significantly reduced two-fold in a rad52-Y66Actf4Δ strain (Table 2). These data suggest that ctf4Δ causes hyper-recombination by a different mechanism from rad52-Y66A likely by affecting both centromere function and global sister chromatid cohesion [55–57].
Previous studies have shown that fluorescently tagged Rad52 relocalizes from a diffuse nuclear pattern to distinct foci upon induction of DSBs. Focus formation occurs almost exclusively in S phase of mitotically growing cells . To investigate the effect of rad52-Y66A on focus formation, strains expressing Rad52-YFP and Rad52-Y66A-YFP were analyzed (Fig. 3). The localization of these proteins was investigated in rad52Δ diploid cells transformed with a single-copy plasmid carrying either RAD52-YFP or rad52-Y66A-YFP. Fluorescence microscopy shows that the level of spontaneous foci is significantly elevated for rad52-Y66A-YFP in both unbudded (G1) and budded cells (S/G2/M) (Fig. 3A and 3B). The levels of spontaneous Rad52 foci were also measured in a msh2Δ background. The experiment was performed in a rad52Δ msh2Δ diploid strain transformed with either the single-copy plasmid carrying RAD52-YFP or rad52-Y66A-YFP. The level of spontaneous Rad52-YFP foci in msh2Δ budded cells is not significantly different from the levels in a MSH2 background. However, the levels of spontaneous Rad52-Y66A-YFP foci in a msh2Δ strain are significantly lower than in a MSH2 background (Fig. 3B).
It is possible that changes in the levels of spontaneous Rad52 foci are the result of changes in the number of DNA lesions. Alternatively, the number of DNA lesions remains the same, but the length of time that the repair proteins remain at foci changes. To distinguish between these possibilities, time-lapse experiments were performed to measure the duration of foci (Fig. 3C). These experiments show that the median Rad52-YFP focus lasts 15 minutes and the median Rad52-Y66A-YFP focus lasts 84 minutes. In a msh2Δ strain, a Rad52-YFP focus lasts 12 minutes, whereas a Rad52-Y66A-YFP focus lasts 60 minutes. Moreover, the cumulative percentage of rad52-Y66A, msh2Δ and rad52-Y66A msh2Δ cells that form at least one Rad52 focus per cell cycle in the time-lapse experiments is not significantly different from that of wild-type cells (Fig. 3D). These data show that the increased duration of foci in rad52-Y66A is largely responsible for the higher frequency of foci observed in both MSH2 and msh2Δ cells (Fig. 3B). Compared to the MSH2 strain, the decrease in duration time of Rad52-Y66A-YFP foci in msh2Δ may be responsible for the lower frequency of foci seen in msh2Δ (Fig. 3B). Thus, our results suggest that rad52-Y66A does not result in an increase in the frequency of DNA lesions, but rather that recombination is slower in the rad52-Y66A mutant.
Lastly, we did not observe RAD52-YFP and RAD52-YFPmsh2Δ cells progressing through the cell cycle until the Rad52 focus disassembles. However, rad52-Y66A-YFP and rad52-Y66A-YFPmsh2Δ cells occasionally divide disregarding the presence of a repair focus likely due to adaptation to the DNA damage checkpoint. This result explains the occurrence of Rad52-Y66A-YFP foci in G1 cells, which is not observed in wild-type cells.
Long-lasting Rad52-Y66A foci indicate that the DNA repair proteins are associated with the site of DNA damage for a longer time than in wild-type cells. Prolonging this association could affect several aspects of recombination including crossover frequency, gene conversion tract length, and choice of donor template thereby causing the hyper-recombination phenotype observed in rad52-Y66A cells. If the hyper-recombination phenotype of rad52-Y66A cells were due to a change in crossover frequency or conversion tract length, we would expect the degree of hyper-recombination to vary with the distance between the heteroalleles, while a change in the choice of donor template should not vary with the distance between the heteroalleles. To evaluate these alternatives, spontaneous C × C recombination was measured between heteroallelic polymorphisms separated by ~200 bp or ~1150 bp. In the original C × C recombination assay discussed above, the polymorphic sites are separated by ~950 bp (Table 3, top). This analysis shows that the rad52-Y66A strain is hyper-recombinogenic to approximately the same degree independent of the length separating the ade2 polymorphisms (Table 3). The same trend is observed in the rad52-Y66A msh2genetic background, where mismatch repair is decreased (Table 3). These result suggests that the rad52-Y66A hyper-recombination phenotype is due to a change in the choice of donor template rather than a change in crossover frequency and/or conversion tract length.
An mre11Δ strain is unable to repair DNA damage induced by hydroxyurea (HU) , which causes the formation of replication-associated DSBs. To further explore the epistatic relationship between rad52-Y66A and mre11Δ, we tested the sensitivity of rad52-Y66A to HU. Indeed, we find that HU strongly impairs growth and colony formation for the rad52-Y66A strain (Fig. 2C).
Further, the similar phenotypes of rad52-Y66A and mre11Δ mutants led us to measure the rate of C × C recombination in an mre11Δ msh2Δ strain. If the mechanism by which rad52-Y66A and mre11Δ result in a hyper-recombination phenotype is similar, then the increase in recombination of a rad52-Y66A msh2Δ strain should be comparable to an mre11Δ msh2Δ strain. Indeed, the hyper-recombination rate of mre11Δ msh2Δ is the same as for rad52-Y66A msh2Δ (Table 1). In addition, the C × C recombination rate of the rad52-Y66A mre11Δ msh2Δ triple mutant is not significantly higher than either the rad52-Y66A msh2Δ or mre11Δ msh2 double mutants, further showing that rad52-Y66A and mre11Δ are in the same epistasis group (see section 3.2). Taken together with previous studies demonstrating that Mre11 is required for sister chromatid recombination [64,65], the results presented here support the conclusion that the hyper-recombination phenotypes of rad52-Y66A and mre11Δ could reflect the same underlying mechanism.
In the budding yeast S. cerevisiae, recombinational repair during mitotic growth relies on several DNA repair proteins, including those encoded by genes of the RAD52 epistasis group. In this study, we measured spontaneous heteroallelic recombination between two chromosomes (C × C) or between a chromosome and a plasmid (C × P). Interestingly, we find that the two configurations display different requirements. The rate of wild-type C × P recombination is ten-fold lower than the rate of C × C recombination. Several factors that could contribute to this difference are outlined below.
One possible explanation for the ten-fold difference may relate to the timing of the replication of the two heteroalleles since spontaneous recombination is likely to occur primarily during S phase . For example, some origins initiate DNA replication at the start of S phase , other origins fire slightly later during S , whereas still others fire during the second half of S phase [68,69]. Homologous chromosomes are under the control of identical replication origins which are likely to fire at the same time. On the other hand, DNA replication of the plasmid is controlled by a different origin which is likely to initiate at a different time. Thus, the differential timing of replication may make the plasmid and chromosome sequences available for recombination at different times thus lowering their potential to recombine. Another difference between chromosome and plasmid sequences is the length of homology. Chromosomes can potentially pair along their entire length, while the plasmid contains only 2.2 kb of homologous DNA with the chromosomal site. Thus, the shorter homology on the plasmid may be limiting. Finally, the difference between the two configurations may reflect the genomic context of the heteroalleles. For example, chromatin structure may be different between plasmid and chromosomal sequences, and the plasmid-borne ade2-n allele is likely to be spatially restricted due to its centromere-mediated anchoring at the spindle pole body . These possibilities in turn may reduce the probability of an interaction with the chromosomal ade2-a locus (Fig. 4A, top row).
Several issues were considered to explain the hyper-recombination phenotype of the rad52-Y66A mutant. The epistasis analysis of rad52-Y66A relative to other hyper-recombination mutants, msh2Δ, ctf4Δ and mre11Δ, shows that the Y66A mutation most closely phenocopies the mre11Δ deletion, which is defective in sister chromatid recombination (Fig. 4). The phenotypic similarities were further supported by its mre11Δ-like HU sensitivity. The partial rescue of γ-ray sensitivity in rad52-Y66A diploids further supports the notion that these cells frequently utilize the homologous chromosome as a template for repair instead of the sister chromatid. In addition, changing the distance between the heteroalleles does not affect the degree of hyper-recombination, suggesting that rad52-Y66A alters the choice of donor template rather than recombination crossover frequency and/or conversion tract length, although these parameters were not measured directly. Taken together, our data support the hypothesis that the rad52-Y66A mutant phenotype may result from the failure to repair damage using the sister chromatid, thereby increasing interchromosomal interactions that lead to hyper-recombination.
Tyrosine at position 66 of yeast Rad52 is highly conserved through eukaryotic evolution . No structural information is available for yeast Rad52, but in the X-ray crystal structure of human Rad52, the corresponding tyrosine 51 is burrowed below the DNA binding groove with little surface exposure [71,72]. Thus, the structural information indicates that this residue is unlikely to have direct contacts with DNA or other protein, but may rather be important for putative conformational changes during recombination. Consistent with this notion, the human Rad52-Y51A protein is proficient for DNA binding. Together with the separation-of-function phenotype of the yeast rad52-Y66A mutant, this information suggests that, rather than affecting the initial association with DNA, the Y66A mutation prevents a later step during homologous recombination. This step, which is dispensible for heteroallelic recombination, but important during the repair of IR-induced lesions, may be second-end capture [73,74].
In response to induced DNA damage, postreplicative cohesion is assembled in an MRE11-dependent fashion [11–14]. This assembly is likely to occur during the transient association of Mre11 with the site of DNA damage immediately upon its recognition. We previously showed that Mre11 dissociates from the site of DNA damage after approximately 20 minutes raising the possibility that damage-induced cohesion is not maintained in the event of persistent damage . Here we show that Rad52-Y66A-YFP foci often persist for several hours. If DNA damage-induced cohesion is relaxed upon dissociation of Mre11, before repair from the sister chromatid takes place, survival would be enhanced by redirecting repair towards the homologue resulting in interchromosomal recombination (Fig. 4B). Such a scenario might be beneficial to promote survival, even in wild-type cells, in the event that sister chromatid recombination cannot be completed due to damage of both sister chromatids.
This work was supported by The Danish Agency for Science, Technology and Innovation and the Villum Kann Rasmussen Foundation (ML), the Danish Research Council for Technology and Production Sciences (UHM), and the National Institutes of Health (GM50237 and GM67055 to RR). We thank Marisa Wagner for constructing the pWJ1190 plasmid and Lorraine Symington for sharing strains.
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