Genomic instability associated with DNA replication stress is linked to cancer and genetic pathologies in humans. If not properly regulated, replication stress, such as fork stalling and collapse, can be induced at natural replication impediments present throughout the genome. The fork protection complex (FPC) is thought to play a critical role in stabilizing stalled replication forks at several known replication barriers including eukaryotic rDNA genes and the fission yeast mating-type locus. However, little is known about the role of the FPC at other natural impediments including telomeres. Telomeres are considered to be difficult to replicate due to the presence of repetitive GT-rich sequences and telomere-binding proteins. However, the regulatory mechanism that ensures telomere replication is not fully understood. Here, we report the role of the fission yeast Swi1Timeless, a subunit of the FPC, in telomere replication. Loss of Swi1 causes telomere shortening in a telomerase-independent manner. Our epistasis analyses suggest that heterochromatin and telomere-binding proteins are not major impediments for telomere replication in the absence of Swi1. Instead, repetitive DNA sequences impair telomere integrity in swi1Δ mutant cells, leading to the loss of repeat DNA. In the absence of Swi1, telomere shortening is accompanied with an increased recruitment of Rad52 recombinase and more frequent amplification of telomere/subtelomeres, reminiscent of tumor cells that utilize the alternative lengthening of telomeres pathway (ALT) to maintain telomeres. These results suggest that Swi1 ensures telomere replication by suppressing recombination and repeat instability at telomeres. Our studies may also be relevant in understanding the potential role of Swi1Timeless in regulation of telomere stability in cancer cells.
In every round of the cell cycle, cells must accurately replicate their full genetic information. This process is highly regulated, as defects during DNA replication cause genomic instability, leading to various genetic disorders including cancers. To thwart these problems, cells carry an array of complex mechanisms to deal with various obstacles found across the genome that can hamper DNA replication and cause DNA damage. Understanding how these mechanisms are regulated and orchestrated is of paramount importance in the field. In this report, we describe how Swi1, a Timeless-related protein in fission yeast, regulates efficient replication of telomeres, which are considered to be difficult to replicate due to the presence of repetitive DNA and telomere-binding proteins. We show that Swi1 prevents telomere damage and maintains telomere length by protecting integrity of telomeric repeats. Swi1-mediated telomere maintenance is independent of telomerase activity, and loss of Swi1 causes hyper-activation of recombination-based telomere maintenance, which generates heterogeneous telomeres. Similar telomerase-independent and recombination-dependent mechanism is utilized by approximately 15% of human cancers, linking telomere replication defects with cancer development. Thus, our study may be relevant in understanding the role of telomere replication defects in the development of cancers in humans.
Citation: Gadaleta MC, Das MM, Tanizawa H, Chang Y-T, Noma K-i, Nakamura TM, et al. (2016) Swi1Timeless Prevents Repeat Instability at Fission Yeast Telomeres. PLoS Genet 12(3): e1005943. https://doi.org/10.1371/journal.pgen.1005943
Editor: Li-Lin Du, National Institute of Biological Sciences, CHINA
Received: October 27, 2015; Accepted: February 25, 2016; Published: March 18, 2016
Copyright: © 2016 Gadaleta et al. This is an open access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited.
Data Availability: The data regarding ChIP-seq are available at GEO (http://www.ncbi.nlm.nih.gov/geo/) with accession number GSE74487.
Funding: This work was supported by National Institutes of Health (GM077604 to EN; GM078253 to TMN; and DP2-OD004348 to KiN http://www.nih.gov), the Aging Initiative at Drexel University College of Medicine (to MCG http://www.drexel.edu/medicine/Research/Student-Research/Aging-Initiative/) and the G. Harold & Leila Y. Mathers Charitable Foundation (to KiN http://www.mathersfoundation.org). Support for sheared resources utilized in this study was provided by Cancer Center Support Grant (CCSG, http://www.cancer.gov) P30CA010815 to the Wistar Institute. The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.
Competing interests: The authors have declared that no competing interests exist.
Eukaryotic cells must accurately replicate their genetic information every cell cycle. However, this process is challenged by the presence of natural impediments throughout the genome that can halt replisome progression, potentially causing genomic instability, a hallmark of cancer and other hereditary disorders [1–4]. These natural impediments are termed replication fork barriers (RFBs) and are typically classified into two groups. The first group arises from non-histone DNA-binding proteins, such as fork-blocking proteins found at eukaryotic rDNA genes, the fission yeast mating-type locus, and long terminal repeats (LTRs) [5–9]. The second group includes DNA secondary structures such as G quadruplexes, hairpins, and triplex DNA, which are often found at repetitive or palindromic DNA sequences [10–15]. Although these RFBs present obstacles for DNA replication, the nature of these barriers and the mechanisms by which the cell ensures the smooth passage of the replisome through each RFB are not fully understood.
Key to the replisome regulation at RFBs is the fork protection complex (FPC), which is composed of the Timeless and Tipin proteins in mammalian cells. The functions of the FPC are conserved throughout evolution, reflecting its fundamental role in genome stability [16, 17]. The FPC travels with the replisome during DNA replication, stabilizes stalled forks, and promotes full activation of the DNA replication checkpoint [18–25]. The FPC also plays a critical role at several RFBs. In the fission yeast Schizosaccharomyces pombe, Swi1 (Timeless orthologue) and Swi3 (Tipin orthologue) are necessary for programmed fork termination and pausing at RTS1 (replication termination site 1) and MPS1 (mat1 pausing site 1) at the mating-type locus (mat1), respectively, leading to an imprinting event required for mating-type switching [5, 26, 27]. Swi1 and Swi3 are also required for site-specific replication fork arrest at the Ter1-3 sites within the intergenic spacer of the rDNA repeats . Furthermore, Swi1 prevents recombinogenic lesions at RFBs localized at tRNA genes in fission yeast .
In addition to the RFBs described above, studies in yeast and human cells have shown that telomeres form specialized chromatin structures that cause replication fork pausing during telomere replication [30–32]. Telomeres are nucleoprotein structures at the ends of linear chromosomes in eukaryotes. Repetitive G-rich sequences at telomeres can form G-quadruplex structures that may hinder DNA replication. Telomeres also recruit heterochromatin proteins and telomere-specific proteins that form the shelterin complex [33–35]. Such structures may cause genomic instability during DNA replication if this process is not properly regulated.
In fission yeast, the RNA interference (RNAi) pathway initiates heterochromatin formation, leading to Clr4-dependent histone H3 methylation and subsequent recruitment of Swi6, the orthologue of heterochromatin protein 1 (HP1) [36, 37]. At telomeres, heterochromatin establishment can occur by an additional pathway that uses Taz1, a component of the shelterin complex, which regulates telomerase activity and inhibits DNA damage response at telomeres . Taz1 contains a Myb DNA-binding domain, associates with telomeric repeats, and plays a role in efficient replication of telomeres . In mammalian cells, deletion of TRF1, a Taz1 orthologue, results in inefficient telomere replication when monitored by DNA combing, while overexpression of TRF1 can also lead to fork stalling at telomere repeats [40, 41]. These results suggest that the shelterin complexes including Taz1/TRF1 play a critical role in regulation of telomere replication. Previously, we have found that Timeless (Swi1 orthologue) interacts with TRF1, a component of shelterin, and prevents telomere shortening and fork collapse at telomeres in human cells . In S. cerevisiae, loss of Tof1 (Swi1 orthologue) or its partner Csm3 (Swi3 orthologue) causes an increase in telomere-size heterogeneity but not significant telomere shortening . These findings suggested a role of the FPC in telomere replication. However, whether the function of the FPC at telomere is conserved throughout evolution is not known, nor is it known what features of telomeres actually present the barrier to the DNA replication process.
In this study, we investigated the role of Swi1 in fission yeast telomere maintenance. We show that Swi1 deletion results in telomere shortening, accumulation of DNA damage, and increased recombination at telomeres. Our results suggest that the primary obstacle for unstable replisomes lacking Swi1 may lie in the repetitive nature of the telomeric DNA and not in the presence of heterochromatin or non-histone DNA-binding proteins. We also show that the telomere shortening in swi1Δ cells is likely caused by replication problems and not by defects in telomerase recruitment. Furthermore, we show that swi1Δ cells more frequently utilize alternative lengthening of telomeres (ALT)-like mechanisms than wild-type cells to amplify telomeric/subtelomeric regions in the absence of telomerase to maintain telomeres. Taken together, our analyses reveal novel and conserved roles of the FPC in telomere maintenance and in replication fork stabilization at repetitive DNA regions. Considering that approximately 10–15% of all human cancers activate ALT pathways to maintain telomeres [44, 45] and that ALT was recently shown to occur even in normal mammalian somatic cells in vivo , our results may be relevant in understanding how Swi1Timeless ensures telomere stability and prevents ALT activation in subsets of human cancers.
Swi1 prevents DNA damage at telomeres
We previously found that swi1Δ cells accumulate spontaneous Rad52 DNA repair foci during DNA replication . Rad52 recombinase binds single-stranded DNAs (ssDNAs) at sites of DNA damage and is required for DNA repair [48, 49], indicating that swi1Δ cells accumulate DNA lesions. However, it was unknown whether these Rad52 foci are localized randomly throughout the genome or at specific chromosome loci in swi1Δ cells. Since human Timeless, the ortholog of S. pombe Swi1, is involved in preventing telomere damage , we hypothesized that Rad52 is preferentially recruited to telomeres in swi1Δ cells. To address this hypothesis, we performed ChIP-seq analysis of Rad52 using wild-type and swi1Δ cells endogenously expressing Rad52 fused to 12 tandem copies of the Pk epitope (Rad52-12Pk). We previously reported that Rad52-12Pk is functional as rad52-12Pk cells showed no significant change in DNA damage sensitivity, and Rad52-12Pk was recruited to the mat1 locus in wild-type cells .
Interestingly, Rad52-12Pk ChIP-seq analysis showed that subtelomeric regions have increased Rad52 binding in swi1Δ cells compared to wild-type cells (Fig 1A). In order to confirm the specific enrichment of Rad52 at subtelomeric regions, we compared Rad52 enrichment between subtelomeres and other chromosome regions (Fig 1B). For this purpose, we divided the entire genome into non-overlapping 2-kb windows and compared Rad52 enrichment at each 2-kb window between swi1Δ and wild-type samples. We accounted 20-kb from each chromosome end as a subtelomere region (ten 2-kb windows from a chromosome end). We excluded rDNA regions from the analysis because Rad52 is enriched at rDNAs in swi1Δ cells (described later). The box plots for log2 ratios of Rad52 enrichment showed a significant increase of Rad52 association at subtelomeres over other chromosome regions in swi1Δ cells (Fig 1B).
(A) Genome-wide (ChIP-seq) analysis of Rad52 distribution at the subtelomeres (left arm of chromosome 1) in asynchronous cultures of wild-type (green) and swi1Δ (blue) cells. Enrichment of Rad52 is displayed as enrichment scores (y-axis). Chromosome coordinates [x-axis, in megabases, (Mb)] were downloaded from the S. pombe Genome Project (Sanger Center: www.sanger.ac.uk/Projects/S_pombe). The strains used for our experiments are both heterothallic h+ strains. (B) Box plots for log2 ratios of Rad52 enrichment at subtelomeric regions vs other regions. The boxes were limited by the 25th and 75th percentiles, with the black lines representing the median ratios between swi1Δ and wild-type. The whiskers are extended out to the most extreme data points that are at most 1.5 times the interquartile range from the box. The black circles represent outliers. The p-value was evaluated by Mann-Whitney U test. (C) ChIP assays showing Rad52 enrichment at telomeres in wild-type and swi1Δ cells. Rad52-12Pk was immunoprecipitated from the indicated cells, and associated DNA was subjected to competitive multiplex PCR to amplify DNA fragments from the TAS1 region and a gene-free region (GFR2), which was used as an internal amplification control. Chromatin association of Rad52-12Pk at TAS1 was presented as relative enrichment over the association at GFR2. Data are expressed as the mean of three independent experiments. Error bars represent the standard deviation. p-value was determined by two-tailed Student's t-test. (D-E-F) Wild-type and swi1Δ cells expressing Rad52-YFP and Taz1-mCherry were grown in minimal medium at 25°C until mid-log phase. Nuclei (n = 102) were analyzed for the percentage of TIF-positive nuclei in (D) as well as for the total number of Rad52-YFP and Taz1-mCherry foci in (E). Accumulation of Rad52-YFP foci (E) and a significant increase in TIF-positive nuclei were observed in the swi1Δ cells (D). Data shown is the mean of three independent experiments. Error bars represent the standard deviation. p-values were determined by two-tailed Student's t-test. (F) Representative microscopic images. Pink arrows indicate TIFs.
To address the role of Swi1 in telomere maintenance, we also performed PCR-based ChIP analysis of Rad52 at telomeres. We found that in wild-type cells, Rad52 enrichment at subtelomeres (the TAS1 region) was approximately 3 times more than that at a control locus (Fig 1C, see Fig 2A for location of TAS1 subtelomeric region), indicating that telomeres are inherently difficult to replicate and are prone to generating ssDNA. These results are in agreement with previous reports showing differential arrival of the leading- and lagging-strand DNA polymerases and an S phase-specific increase in RPA recruitment at telomeres [51, 52]. Importantly, Rad52 binding at the TAS1 region was further increased in swi1Δ cell (Fig 1C), suggesting the role of Swi1 in limiting Rad52 accumulation at telomeric regions. To further substantiate this result, we conducted a telomere-dysfunction induced foci (TIF) assay that examines co-localization of Rad52 and a telomere maker, Taz1. For this purpose, Rad52 and Taz1 were fused to yellow fluorescent protein (YFP) and mCherry, respectively, and expressed from their own promoters at their chromosomal loci. We counted over 100 nuclei and determined the ratio of TIF-positive nuclei in each cell culture. This analysis revealed that swi1Δ cells present a higher amount of TIF-positive nuclei than wild-type cells (Fig 1D and 1F). swi1Δ cells did not show any significant difference in the number of Taz1 foci; however, they displayed more Rad52 foci overall than wild-type cells (Fig 1E and 1F). Therefore, it was possible that the elevated TIF-positive nuclei seen in the swi1Δ culture was a consequence of increased stochastic DNA damage events occurring throughout the genome. To exclude this possibility, we next calculated the ratio of TIF events to total Rad52 foci. TIF occurred in 5.19% and 11.08% of Rad52 foci in wild-type and swi1Δ cells, respectively (see S1A Fig), indicating that telomeres undergo increased DNA damage in the absence of Swi1. In addition, we observed the occurrence of Rad52 foci lateral to Taz1 foci in swi1Δ cells (S1B Fig). This may reflect the Rad52 enrichment found at subtelomeres in our Rad52 ChIP-seq experiments (Fig 1A), and subtelomeric regions are also susceptible to DNA damage. However, these Rad52 foci lateral to Taz1 foci were not considered as TIFs in our analysis. Thus, increase in DNA damage occurring at telomeric/subtelomeric regions is likely to be even more severe than suggested by our analysis of TIF-positive cells. Taken together, our results established the critical role of Swi1 in preventing DNA damage at telomeres in fission yeast.
(A) Schematic diagram showing the position of the ApaI restriction site at S. pombe telomeres and the TAS1 (Telomere-Associated Sequences) region . Terminal telomeric repeats are shown in red. The position of the telomeric probe used in this study is marked in green. (B) Southern blot analysis of ApaI-digested genomic DNA from independently isolated strains of the indicated genotypes. Each strain was passaged at least 8 times before DNA isolation, in order to allow for telomere length stabilization. ApaI-telomere fragments were detected with a telomere-specific DNA probe. (C) swi1Δ cells were transformed with the pJK148-Swi1 plasmid or with the control vector pJK148. Transformants were isolated and passaged at least 8 times before genomic DNA preparation. Southern blot analysis of the ApaI-telomere fragments was performed as described above. Telomeres of two or three independent isolates from each transformation are shown. (D) Swi1 is recruited to TAS1 in a replication-dependent manner. swi1-13Myc cdc25-22 cells were synchronized at the G2/M boundary by incubation at 36°C for 3 h and then released into fresh YES medium with or without 15 mM hydroxyurea (HU), an inhibitor of DNA replication. Cells were collected at the indicated times and processed for Swi1-13Myc ChIP, and telomere association of Swi1 was determined by real-time PCR as described . Swi1-13Myc was associated with TAS1 as cells replicate DNA. Previously determined peaks of binding for leading (Pol ε) and lagging (Pol α and Pol δ) strand DNA polymerase  are indicated. Addition of HU, which prevented telomere replication, inhibited Swi1-13Myc recruitment at TAS1. (E) Southern blot analysis of ApaI-telomere fragments from the indicated cells was performed as described in B.
Swi1 is required for telomere length maintenance
Although the role of the FPC in telomere maintenance has been suggested [16, 42, 53], mechanistically how Swi1 regulates telomere length is unknown. In order to understand the role of the FPC in telomere replication, we first investigated the role of the Swi1-Swi3 FPC in telomere length maintenance. Cells were consecutively streaked at least 8 times on YES plates at 3-day intervals (~33 doublings per streak) in order to stabilize telomere lengths after deletion mutants were generated. To detect telomere fragments, the genomic DNA from several independent isolates of FPC mutants was digested with ApaI (Fig 2A) and analyzed by Southern blot (Fig 2B). Consistent with previous reports [42, 53], swi1Δ cells had much shorter telomeres when compared to wild-type cells (Fig 2B). In addition, we found that swi3Δ cells carry short telomeres similar to swi1Δ (Fig 2B). Telomere lengths in swi1Δ and swi3Δ cells were similar to those in rad3Δ and rad26Δ mutants, already known to harbor significantly short telomeres [54–56] (Fig 2B). Telomere shortening in swi1Δ cells was rescued by transforming swi1Δ cells with a plasmid vector containing the swi1+ gene but not with a control vector (Fig 2C), indicating that the loss of telomeric repeats is directly caused by loss of Swi1 and can be reversed by reintroducing a fully functional FPC. Furthermore, a cell cycle-ChIP analysis found that Swi1 is specifically recruited at telomeres during S phase and that addition of HU, which have been previously established to inhibit late-S phase replication of telomeres , eliminated Swi1 recruitment (Fig 2D). These observations suggested that the Swi1-Swi3 FPC is important for proper replication of telomeres to ensure telomere length maintenance in fission yeast.
The FPC stabilizes replication forks and mediates activation of the replication checkpoint [18, 21, 47]. In the latter function, Swi1 is required for proficient activation of the checkpoint kinase Cds1. However, previous reports indicated that Cds1 has no role in telomere length maintenance [54, 56, 58]. Consistently, we also observed that cds1Δ cells do not show telomere shortening (Fig 2E). In the absence of Swi1, cells accumulate replication stress, leading to Chk1-dependent G2/M delay, and swi1Δ chk1Δ cells shows growth defects and are much more sensitive to genotoxic agents than either single mutant . Therefore, we tested whether telomere length in swi1Δ cells is affected by loss of Chk1. However, there was no further shortening of telomere length in swi1Δ chk1Δ cells compared to swi1Δ cells (Fig 2E). Thus, we concluded that Swi1-mediated telomere length maintenance does not rely on Swi1’s role in regulation of checkpoint kinases Chk1 and Cds1.
Swi1 ensures replication of repetitive DNA
Several telomeric features can hamper the passage of the replication machinery and cause telomere damage and shortening. G-quadruplexes, repetitive DNA, heterochromatin, and the potential to form t-loop structures have been suggested as possible obstacles for the replication machinery; however the concrete nature of the telomere barrier remains elusive. We hypothesize that swi1 deletion results in an unstable replisome that will be more vulnerable to these obstacles. Since previous studies have found that lagging-strand synthesis at fission yeast telomeres is substantially delayed compared to leading-strand synthesis [52, 59, 60], the FPC could be especially important for protecting integrity of replisome at telomeres until lagging-strand synthesis is successfully completed.
To determine whether Swi1 generally functions in maintaining integrity of repetitive DNA sequences, we first tested the role of Swi1 during replication in maintaining stability of E. coli LacO array derived from the pSV2-DHFR-8.32 vector . This array contains 32 direct repeats of a 317-bp DNA fragment. Each fragment includes 8 direct repeats of a 36-bp DNA sequence containing the LacO operator and a 29-bp linker sequence; thus, this LacO array has 256 repeats of the 36-bp DNA sequence . In order to investigate whether the LacO repeats interfere with the replication process, we used S. pombe strains that carry the LacO array at the ade3+ or ade1+ locus [62, 63] as these loci are not associated with known repeat DNA sequences [64, 65]. These strains were initially designed to express the LacI-GFP fusion protein that binds the LacO repeats inserted at ade3 or ade1 loci. Since LacI-GFP may affect replication of the LacO array , we removed the LacI-GFP transgene from these strains by genetic crossing before the swi1+ gene was deleted. Absence of LacI-GFP expression was confirmed by fluorescent microscopy.
Immediately after the swi1 deletion was introduced into the strains that carry the LacO array, segregants were passaged by restreaking multiple times on YES plates in order to stabilize repeat length. Southern blot analyses using a LacO repeat-specific probe show that wild-type cells maintained the LacO repeat length (~8 kb and ~6 kb in strains carrying the LacO array at ade3 and ade1 loci, respectively) even after cells were passaged multiple times (Fig 3A). In contrast, swi1Δ cells displayed dramatic shortening of LacO repeats integrated at the ade3 locus indicative of repeat instability. The effect of swi1 depletion on LacO repeat instability was clear at the earliest passage and became more prominent with the consecutive streaks. We also observed considerable repeat instability that resulted in both longer and shorter LacO repeats when the construct was integrated at the ade1 locus, suggesting that Swi1 is involved in replication and/or maintenance of repeat DNA sequences independently of the repeat location (Fig 3A). Such instability appears to cause DNA damage as swi1 deletion resulted in a significant enrichment of Rad52 at the LacO repeats while no difference was found at a non-repetitive locus such as rec8 (Fig 3B). We also found similar results at rDNA repeat regions, where loss of swi1 caused increased DNA damage as represented by elevated recruitment of Rad52 at rDNA repeats (Fig 3C). This is consistent with the fact that swi1Δ cells have a shorter chromosome III [67–70], which contains rDNA repeats in S. pombe. These results suggest that Swi1 is required for preventing DNA damage at repeat DNA regions. In particular, our findings indicate that Swi1 plays a critical role in proper replication of LacO as well as rDNA repeats.
(A) Southern blot analysis using a LacO probe on genomic DNA extracted from wild-type or swi1Δ cells carrying the LacO array. Genomic DNA was prepared after 1 or 8 restreaks after the indicated strains were generated, digested with StuI and separated on a 0.4% agarose gel. Similar results were obtained with another independent swi1Δ ade1::LacO strain. A wild-type strain with no LacO repeats was used as a control for potential background hybridization. (B) Rad52 is enriched at LacO repeats but not at the meiotic gene rec8 where no replication obstacles are expected. ChIP assays of Rad52-12Pk were performed on cell extracts prepared form the indicated cells. The immunoprecipitated DNA was subjected to competitive multiplex PCR to monitor the association of Rad52-12Pk with the LacO tract and the rec8 gene, using the gene-free region 2 (GFR2) and GFR3 as internal amplification control loci, respectively. Chromatin association is presented as described in Fig 1C. Swi1 deletion significantly enhanced Rad52 recruitment at LacO repeats, while no significant difference was found at the rec8 locus. Statistical analysis of three independent experiments was performed as described in Fig 1C. (C) Swi1 deletion causes DNA damage at rDNA repeats. ChIP assays show enrichment of Rad52-12Pk at rDNA repeats in wild-type and swi1Δ cells. swi1Δ cells display a 2-fold increase in Rad52 binding at rDNA compared to wild-type. ChIP and competitive multiplex PCR were performed using primers specific for the rDNA (rDNA_2) and a gene-free region (GFR2). Statistical analysis of three independent experiments was performed as described in Fig 1C.
The aforementioned results suggest that repetitive DNA presents a replicative obstacle in swi1Δ cells. Since telomeres are composed of highly repetitive DNA, we hypothesized that telomere shortening observed in swi1Δ cells could be attributable to the repetitive nature of telomere DNA. The presence of DNA ends at telomeres could complicate interpretation of our analysis because the end-replication problem, telomerase recruitment, and recombination among chromosome ends can all affect telomere length. Thus, to specifically investigate contribution of Swi1 in maintaining telomere repeat stability, we studied the stability of a single synthetic internal telomere tract (~300 bp) within an episomal plasmid (Fig 4A).
(A) Schematic diagram of pAS-SK-telo plasmids. (B) Wild-type and swi1Δ cells were transformed with either the empty pAL-SK plasmid or the pAL-SK carrying a 300 bp. telomere tract in normal (+) or reverse (-) orientation relative to the replication origin of the plasmid. Recovered plasmid from 10 yeast colonies was amplified in bacteria, and 10 bacterial colonies per treatment were analyzed by restriction digestion with PvuII in 3% agarose gels stained with EtBr. Each column represents and independent bacterial colony. Size markers are shown and expected restriction fragment size is shown in bold.
We generated pAL-SK plasmids carrying a single 300-bp telomere tract (leu1::telomere) inserted in either forward (+) or reverse (-) orientation with respect to the position of the replication origin in the plasmid. These plasmids represent the natural (+) and inverse (-) orientation of the telomeric repeats in reference to the replisome movement (Fig 4A). To allow for plasmid replication in the presence or absence of Swi1, wild-type and swi1Δ cells were transformed with either the empty plasmid or the plasmid carrying the telomere tract in either orientation. Recovered plasmid was amplified in bacteria, and 10 bacterial colonies per treatment were analyzed by restriction digestion with PvuII.
As shown in Fig 4B, both wild-type and swi1Δ mutant strains were able to amplify the empty plasmid as all colonies analyzed displayed the expected restriction fragment length. Interestingly, the restriction pattern of the pAL-SK-telo(-) plasmid obtained form swi1Δ cells was significantly altered in six out of the 10 colonies analyzed, while the same plasmid obtained from wild-type cells showed the expected band size in all cases. Restriction analysis of the recovered pAL-SK-telo(+) plasmids showed the expected fragment lengths in most of the colonies from both wild-type and swi1Δ mutants strains (Fig 4B). Although these results might seem contradictory as the pALSK-telo(+) plasmid carries the native repeat orientation, it is important to note that we obtained a very low number of colonies for swi1Δ cells transformed with the pALSK-telo(+) plasmid (<10 E. coli colonies per transformation) in comparison to all other treatments (50–100 colonies per transformation). One possible explanation of this observation is that replication of the pAL-SK-telo(+) plasmid could generate toxic intermediates that are unfavorable for growth of swi1Δ cells. It is likely that, as a result of this toxicity, the colonies obtained represent a small subset of yeast cells that carried an unaltered pAL-SK-telo(+) plasmid. Nevertheless, these results are consistent with a notion that Swi1 is critical for replication of repetitive DNA sequences, independently of location and DNA sequence. Furthermore, our data suggests that telomeric repeats, in either orientation, are a significant replication obstacle for Swi1-depleted cells, but their presence in native conformation might be most detrimental for cells. Our data are in agreement with experiments done with trinucleotide repeats where it was shown that the stability of trinucleotide repeats in bacterial, yeast, and cultured mammalian cells depend on their orientation with regard to replication origins [71–74]. Thus, our results indicate that repetitive DNA at telomeres is an important source of instability in the absence of Swi1.
Heterochromatin-related proteins and shelterin are not major obstacles for DNA replication in the absence of Swi1
Similar to the endogenous telomere ends, the telomere tract in the pAL-SK-telo plasmids can recruit telomere-binding proteins such as shelterin components and heterochromatin . Therefore, it was possible that replisome progression through telomeric repeats might be blocked by telomere-binding factors such as shelterin components and heterochromatin related proteins in swi1Δ cells. If so, removal of these features from telomeres would rescue the telomere shortening phenotype of swi1Δ cells.
To disrupt heterochromatin, we deleted genes required for heterochromatin formation. These genes include swi6+ and clr4+, which encode proteins homologues to human HP1 [76, 77] and Suv39 family of histone methyltransferases [78–80], respectively. swi6 or clr4 deletion failed to shorten telomere length in southern blots of ApaI fragments (Fig 5A and 5B), in agreement with related studies [81, 82]. When Swi1 was removed from swi6Δ or clr4Δ cells, telomeres were shortened to the extent of the telomere length in swi1Δ cells (Fig 5A and 5B). Thus, disruption of these HP1-related heterochromatin proteins failed to alleviate telomere shortening of swi1Δ cells. These results suggest that heterochromatin does not cause observable telomere damage and thus does not present a severe obstacle to the DNA replication process.
(A-B) Loss of heterochromatin-related proteins does not rescue telomere-shortening phenotype of swi1Δ cells. Southern blot analysis of telomere fragments from the indicated mutants. At least two independent segregants of the double deletion mutants were examined. Genomic DNA was prepared after 1, 4, or 8 restreaks after the indicated strains were generated. ApaI-telomere fragments were detected using a telomere-specific probe as described in Fig 2B. (C) Telomere shortening still occurs in the absence of shelterin components when swi1 is deleted. Cells with the indicated genotypes were passaged at least 8 times and subjected to Southern blot analysis as described in Fig 2B.
The shelterin complex, which directly associates with telomeres, has been shown to facilitate replication of telomeric repeats in fission yeast cells [39, 60]. However, previous studies in budding yeast have reported that telomere-binding proteins can become a barrier to DNA replication process [31, 83]. Because the replisome is unstable in swi1Δ cells, we tested whether shelterin could act as a replication obstacle in the absence of Swi1. Loss of shelterin components including Taz1, Poz1, and Rif1 resulted in telomere lengthening when compared to wild-type cells as seen in ApaI-telomere length analysis (Fig 5C). This is consistent with previous findings showing that shelterin can act as a negative regulator of telomerase [84–86], as well as with a protective role of Taz1 against activation of homologous recombination (HR)-based telomere lengthening [87, 88]. We then determined telomere length of swi1Δ taz1Δ, swi1Δ poz1Δ, and swi1Δ rif1Δ strains. swi1 deletion led to considerable telomere shortening in poz1Δ and rif1Δ cells and less dramatic but still significant telomere shortening in taz1Δ (Fig 5C), indicating that Swi1 is still important for telomere length maintenance even in the absence of shelterin subunits that inhibit telomere extension.
Swi1 plays a telomerase-independent role in promoting telomere repeat length maintenance
Our analysis of telomere-repeat stability within episomal plasmids in swi1Δ cells (Fig 4) suggested that inability of swi1Δ cells to maintain stable repetitive telomere repeats may contribute to telomere shortening in swi1Δ cells. However, since telomerase recruitment is coupled to replication of telomeres by replicative DNA polymerases, it was possible that loss of FPC might prevent efficient recruitment of telomerase, leading to telomere shortening. Thus, we decided to examine the recruitment of telomerase to telomeres in swi1Δ cells. As shown in Fig 6A, ChIP assays revealed that Trt1 recruitment was significantly elevated in swi1Δ cells when compared to wild-type cells. This is consistent with previous studies showing that telomerase is selectively recruited at shorter telomeres in fission yeast .
(A) Strains of the indicated genotypes were engineered to express Trt1-G9-5FLAG . ChIP results show that telomerase is preferentially recruited at short telomeres in swi1Δ mutants compared to wild-type length telomeres. Telomerase recruitment was monitored by competitive multiplex PCR at two different subtelomeric regions: Tel3s and TAS1. GFR1 (for Tel3s) and GFR2 (for TAS1) were amplified as internal control regions in multiplex PCR reactions. Trt1 enrichment at Tel3s and TAS1 over control regions was determined. Data is shown as relative fold enrichment in comparison to WT. Error bars represent the standard deviation obtained from three independent experiments. (B) trt1Δ taz1Δ and trt1Δ taz1Δ swi1Δ cells were passaged at least 8 times, and Southern blot analysis of ApaI-digested genomic DNA was performed as described in Fig 2B. (C) Genetic interaction between Swi1 and Rad3-Rad26 in telomere maintenance. Genomic DNA was isolated form the indicated cells, and telomere southern analysis was performed as described in Fig 2B.
Interpretation of epistasis analysis between swi1Δ and shelterin subunit mutant (taz1Δ, poz1Δ and rif1Δ) is complicated due to the fact that telomerase can indeed still act on telomeres to extend telomeres in the absence of Swi1. Thus, to evaluate whether the Swi1 indeed plays a telomerase-independent role in maintaining telomere length, we then sought to evaluate effect of eliminating Swi1 in cells that lack telomerase. Since telomerase (trt1+) deletion frequently leads to telomere loss and generation of survivor cells that eliminate telomeres by circularizing chromosomes , we utilized a taz1Δ trt1Δ double mutant strain, which stably maintains heterogeneous telomeres via recombination-dependent, ALT-like telomere maintenance mechanism [87, 88].
Telomeres in taz1Δ trt1Δ cells were much longer than those in wild-type cells, which is consistent with the ALT-like phenotype of taz1Δ trt1Δ cells (Fig 6B). Importantly, swi1Δ taz1Δ trt1Δ triple mutant cells carried shorter telomeres than taz1Δ trt1Δ cells, suggesting that telomere shortening due to swi1 deletion is not caused by a defect in telomerase activity. Interestingly, swi1Δ cells rapidly undergo telomere shortening within the first passage after swi1 deletion, and the telomere length becomes stable afterwards. In striking contrast, trt1Δ cells displayed a much slower and progressive telomere shortening (S2 Fig) . Taken together, we conclude that Swi1 is involved in telomere length maintenance independently of telomerase activity.
Rad3-Rad26 and Tel1-MRN (Mre11-Rad50-Nbs1) kinase complexes are redundantly required for telomerase recruitment at telomeres by promoting phosphorylation of the threonine 93 residue of Ccq1 [90, 91]. Thus, in the absence of Tel1, Rad3-Rad26 becomes essential for telomerase recruitment as rad3Δ tel1Δ and rad26Δ tel1Δ double mutants lose telomeres [56, 58]. To understand the relationship between Swi1 and Rad3-Rad26, we constructed swi1Δ tel1Δ double mutants cells. If Swi1 contributes to Rad3-Rad26-dependent telomerase recruitment, we expect that swi1Δ tel1Δ cells would have shorter telomeres than swi1Δ cells. However, tel1 deletion had no effect on the telomere length of swi1Δ cells (Fig 6C), suggesting that Swi1 is unlikely to be required for Rad3-Rad26’s ability to promote telomerase recruitment. Such conclusion is entirely consistent with our earlier ChIP analysis, which suggested that Swi1 is not necessary for telomerase recruitment (Fig 6A).
On the other hand, we found that telomere length of swi1Δ rad26Δ cells is similar to that of either single mutant (Fig 6C), suggesting that the telomere length maintenance defect observed in rad26Δ is epistatic to swi1Δ. Since previous genetic analysis indicated that Rad3-Rad26 contributes to telomere protection function that appears to be distinct from Rad3-Rad26’s role in telomerase recruitment , we suggest that Rad3-Rad26’s ability to protect telomeres is mediated by Swi1.
Short telomeres in swi1Δ cells are maintained by telomerase and not by homologous recombination
Although telomeres rapidly shorten after the loss of Swi1, swi1Δ cells do not lose all telomeric repeats. Instead, they stably maintain short telomeres even after extensive passages. Because Rad52 recruitment is increased in swi1Δ cells, it was possible that recombinational telomere maintenance pathways might maintain telomeres in the absence of Swi1. Therefore, we inactivated homologous recombination (HR) by deleting rad51+ or rad52+ and determined the effect of these deletions on telomere length. As shown in Fig 7, telomere length of rad51Δ and rad52Δ cells was similar to that of wild-type cells. Importantly, when we deleted rad51+ or rad52+ from swi1Δ or swi3Δ cells, cells still showed short telomeres similar to those in swi1Δ cells (Fig 7). These results indicate that HR is not the major pathway used to maintain short telomeres in swi1Δ cells and further suggest that telomerase is functional in swi1Δ cells.
Deletion of swi1 causes an increase in emergence of ALT-like survivors with amplified telomere/subtelomere regions in the absence of telomerase
The elevated recruitment of telomerase in swi1Δ cells and the ability of these cells to maintain telomeres in HR-deficient backgrounds suggest that short but stable telomeres in swi1Δ cells are maintained by telomerase. This notion prompted us to investigate the physiological consequences of telomerase loss in swi1Δ cells. To inactivate telomerase, we first utilized an est1-deletion background because the telomerase regulatory subunit Est1 is essential for telomerase-dependent telomere maintenance in fission yeast . We deleted swi1+ from est1+/est1Δ diploid cells and generated a swi1+/swi1Δ est1+/est1Δ diploid strain, from which we obtained haploid est1Δ, swi1Δ and est1Δ swi1Δ strains. As expected from previous studies , all est1Δ strains underwent extreme telomere shortening (Fig 8A and 8B). When telomere length of multiple swi1Δ est1Δ strains was monitored, some strains also had extremely short telomeres. However, a strikingly higher proportion of swi1Δ est1Δ strains developed long and heterogeneous telomeres (Fig 8A and 8B), a feature reminiscent of ALT activation in humans [94, 95] and type-II survivors in S. cerevisiae and Kluyveromyces lactis [96–98].
(A) swi1 deletion significantly increases the chances of telomerase negative cells to undergo ALT-like telomere maintenance. Representative image of telomere Southern blot analysis of wild-type, swi1Δ, est1Δ and est1Δ swi1Δ cells. Multiple segregants with the same genotypes were analyzed after at least 11 passages. ApaI-digested DNA was hybridized with the telomere-specific probe as described in Fig 2B. Representative results are shown. (B) Quantification of the independent segregants analyzed for each genotype and classification depending on their telomere phenotype.
To further confirm this phenomenon, we also deleted telomerase catalytic subunit trt1+. Because we were unable to obtain viable swi1Δ trt1Δ cells when we attempted to obtain double mutant cells by gene deletion or genetic cross of trt1Δ and swi1Δ strains, we chose to cross swi1Δ cells with trt1Δ taz1Δ cells to obtain viable swi1Δ trt1Δ cells. Wild-type, swi1Δ, taz1Δ and swi1Δ taz1Δ trt1Δ segregants obtained from the tetrad dissection displayed the expected telomere phenotypes (S3 Fig). Interestingly, again, many of swi1Δ trt1Δ double mutant strains showed long and heterogeneous telomeres whereas most of trt1Δ mutants had extremely short telomeres or lost telomeres (Fig 8B and S3 Fig). The number of ALT-like telomeres observed in the trt1Δ strains was higher than expected from trt1-deficient strains (Fig 8B). This is probably due to the presence of long telomeres in the taz1Δ trt1Δ strain that was used to generate trt1Δ segregants. Taken together, these results suggest that, in the absence of telomerase, short telomeres caused by replication fork instability become templates for recombination-dependent (ALT) maintenance of telomeres. Our findings also suggest that Swi1 protects telomeres from hyper-recombination when telomerase is absent.
In this work, we identified a novel role of Swi1 in preventing repeat instability during DNA replication in S. pombe. More specifically, our investigation revealed that loss of FPC causes telomere instability during replication, which may contribute to telomere shortening in swi1Δ cells. Telomeric repeats rather than other telomeric features present a significant obstacle for the replisome and thus render telomeres difficult to replicate. In addition, our results also suggest that Swi1Timeless prevents recombination-dependent ALT-like telomere amplification in the absence of telomerase. Based on these results, we propose that the role of the FPC could be further exploited in the context of mammalian models as a potential link between genomic instability and ALT-dependent tumorigenesis.
The FPC’s role in telomere replication and telomere length maintenance
Swi1 deletion renders S. pombe cells highly sensitive to fork-stalling agents and causes extensive accumulation of spontaneous Rad52 DNA repair foci during S phase, indicating that Swi1 stabilizes stalled replication forks . Rad52 foci may represent DNA damage at specific chromosome loci that are more difficult to replicate when Swi1 is depleted. These loci include rDNA repeats and telomeres as they are enriched with Rad52 (Fig 1C, Fig 3C). In addition, swi1Δ cells accumulate broken forks at rDNA loci and show elevated levels of TIFs (Fig 1D and 1F) . We therefore suggest that these genomic regions are among the hot spots of DNA damage in swi1Δ cells.
It is possible that stalled or slowed forks at rDNA- or telomere-repeat regions need to be stabilized by Swi1, in order to prevent fork collapse. Importantly, Swi1 coordinates leading- and lagging-strand synthesis at the replication fork [47, 70]. Furthermore, the recruitment of the lagging-strand polymerase (Pol δ) at telomeres is significantly delayed when compared to the leading-strand polymerase (Pol ε) in wild-type cells [52, 59, 60]. Therefore, we propose that loss of Swi1 leads to extensive uncoupling of leading- and lagging-strand synthesis, causing telomeres to adopt unusual open configurations that are prone to fork collapse and DNA damage.
Telomere damage was linked to the occurrence of telomere shortening in swi1Δ cells. Telomere length in swi1Δ strains was comparable with that in rad3Δ and rad26Δ cells. In fission yeast, Rad3ATR and Rad26ATRIP form a complex that is essential for cell cycle arrest by activation of both Cds1Chk2 and Chk1Chk1 kinases responsible for the DNA replication and damage checkpoints, respectively . Swi1 is also involved in full activation of the Cds1 checkpoint kinase in S. pombe . However, our epistasis analysis indicates that both Swi1-Swi3 and Rad3-Rad26 complexes maintain telomere length independently from their role in the activation of downstream checkpoint kinases Cds1 and Chk1 (Fig 9). Our genetic data also suggest that the FPC and Rad3-Rad26 are in the same pathway for telomere length maintenance (Fig 9). Although Rad3-Rad26 phosphorylates the threonine 93 residue of Ccq1 to facilitate telomerase recruitment at telomeres [90, 91], Swi1 appears to play no role in telomerase recruitment as swi1Δ cells showed an increased level of telomerase at telomeres (Fig 6A). Since our previous genetic analysis indicated that Rad3-Rad26 contributes to telomere protection , and this protective function appears to be distinct from it’s role in telomerase recruitment, we suggest that telomere protection function of Rad3-Rad26 is medicated by Swi1 (Fig 9).
Identifying the telomeric replicative obstacles in FPC deficient cells
swi1 deletion causes contraction of rDNA repeats [68, 70]. In this study, we demonstrated that swi1Δ cells harbor short telomeres and undergoes repeat loss and instability associated with the LacO array, indicating that the primary replicative obstruct in swi1Δ cells is repeat DNA sequence.
In E. coli, LacO arrays bound by the LacI protein block replication by forming a site-specific protein–DNA complex that serves as an RFB [100, 101]. In mammalian cells, insertion of LacO repeats generates fragile sites in metaphase chromosomes . This also appears to be dependent on LacI repressor proteins that form RFBs by binding to the LacO repeats . Furthermore, studies in S. pombe showed that the LacI-LacO system leads to replication fork block and DSBs , further suggesting the role of protein-DNA complexes in replication interference. Consistently, in our present study, LacO arrays induced only a mild increase in Rad52 recruitment when LacI was not present in wild-type cells. However, Rad52 was further accumulated at LacO repeats in swi1Δ cells even in the absence of LacI (Fig 3B), suggesting that Swi1 is required for replication of repeat DNA. Considering that the induction of DNA damage response at the LacO arrays bound by LacI occurs as a consequence of DNA replication , the repetitive nature of repeat sequences poses an initial layer of replication problems that is counteracted by Swi1. As in the case of the LacI-LacO RFB, protein-DNA RFBs may provide another layer of replication stress that further complicates replisome passage even in wild-type cells.
Although our studies demonstrated that repetitive DNA is the primary replication problem in the absence of Swi1, it is important to note that several other characteristics of the telomeres may further complicate telomere replication. In budding yeast, the replication fork pauses at telomeres, and this pausing is intensified in the absence of Rrm3 helicase . Furthermore, the presence of Rap1 bound to the telomeric sequences has been suggested to be a component of the telomere replication barrier . In fission yeast, Taz1 is required for efficient telomere replication, and Poz1 and Rap1 also contribute to the completion of telomere replication by promoting timely accumulation of the lagging-strand DNA polymerase and the Stn1-Ten1 complex at telomeres [30, 31, 39]. In addition, the presence of heterochromatin and the potential to form t-loop structures may provide an additional barrier to the passage of the fork . Therefore, further research is necessary to fully understand the composition of the telomeric barrier in fission yeast as well as the replication factors involved in overcoming this barrier. Future studies should focus on the mechanisms by which these telomere features add additional layers of difficulty to the passage of the replication fork.
Possible implications for a role of the mammalian FPC in telomere regulation
Approximately 10–15% of cancer cells including glioblastomas and osteosarcomas  are able to escape replicative senescence by activating the recombination-dependent ALT pathway in the absence of any detectable telomerase activity . Although the prevalence of ALT telomeres is well established, the factors or events that trigger certain cancer cells to activate ALT pathways over telomerase reactivation are not well understood. Accordingly, there are no treatments targeting ALT specifically in cancer cells and, in addition, these tumors are predicted to be resistant to anti-telomerase therapies .
Our results show that Swi1-deficient cells display increased association of Rad52 recombinase, and that loss of Swi1 promotes recombination-based survival in cells lacking telomerase. Therefore, telomere damage during DNA replication may enhance DNA repair processes using the homologous recombination machinery. It is possible that this pathway provides a more robust and efficient response to drastic telomere shortening than telomerase reactivation, in order to maintain telomere length after a rapid and significant telomere repeat loss.
A recent paper showed that cancer cells bearing ALT telomeres are sensitive to ATR inhibitors. This is because ALT telomeres have elevated levels of RPA-coated ssDNA, which is known to recruit ATR . Our findings in S. pombe are in agreement with this work, as loss of Swi1 generates long stretches of ssDNA at the stalled forks [21, 70]. Consistently, Chk1, an effector kinase downstream of Rad3ATR is activated in swi1Δ cells . It is therefore conceivable that Rad3ATR activation in Swi1-deficient cells mediates the formation ALT telomeres observed in swi1Δ est1Δ and swi1Δ trt1Δ cells. Future investigations are warranted to test this possibility and further address the role of Swi1Timeless in preventing ALT-dependent cancers.
Materials and Methods
The methods used for genetic and biochemical analyses of fission yeast have been previously described [107, 108]. For telomere length assays, yeast cells were grown at 32°C on solid YES (yeast extract with supplements) plates. To ensure stabilization of the telomere length, cells were streaked on YES plates every 3 days at least 8 consecutive times prior to genomic DNA preparation. Microscopic analyses of fluorescent proteins, Western blotting, and drug sensitivity assays were performed as described in our earlier studies [21, 47, 68, 109].
S. pombe strains and plasmids
The S. pombe strains used in this study were constructed using standard techniques [107, 108], and their genotypes and sources are listed in S1 Table. To construct episomal plasmids that carry a telomere tract, a 300 bp S. pombe telomere fragment was subcloned from pTELO plasmid  into the PvuII site of the pAL-SK plasmid , which carries the LEU2 gene, resulting in pAL-SK-Telo (+) and pAL-SK-Telo (-). To express Rad52-YFP (originally called Rad22, but recently renamed as Rad52 in S. pombe) as a sole source of Rad52 from the native promoter, pJK210-Rad52CT-YFP  was linearized at the AflII site, which is localized within the DNA sequence that encodes the C-terminal (CT) domain of Rad52, and inserted at the rad52 locus of S. pombe strains. rad52Δ (rad52::hphMX6) was generated by a two-step PCR method , to replace the rad52 open reading frame with the hphMX6 gene. cds1Δ (cds1::hphMX6) was generated by a one-step marker switch method  using cds1::kanMX6 . taz1-mCherry (taz1-mCherry::hphMX6) was also generated by the two-step PCR method, to construct a mCherry tag at the C-terminus of taz1. Plasmids used as template for the PCR-based gene disruption and gene tagging have been previously described for pFA6a-hphMX6  and pFA6a-5FLAG-kanMX6 . pFA6a-mCherry-hphMX6 was constructed by replacing the BglII-EcoRI kanMX6 fragment in pFA6a-mCherry-kanMX6  with hphMX6 fragment. pJK148-Swi1 was constructed by inserting the 3.6 kb genomic fragment containing the swi1+ gene into the SacI/BamHI site of pJK148 .
Mutations and epitope-tagged genes have been previously described for swi1Δ (swi1::kanMX6, swi1::natMX6) [47, 69], rad3Δ (rad3::ura4+, rad3::kanMX6) [67, 117], rad26Δ (rad26::ura4+) , tel1Δ (tel1::ura4+, tel1::LEU2) , cds1Δ (cds1::ura4+) , chk1Δ (chk1::ura4+, chk1::kanMX6) [67, 118], clr4Δ (clr4::kanMX6) , bdf2Δ (bdf2::hphMX6) , taz1Δ (taz1::ura4+, taz1::LEU2) , trt1Δ (trt1::his3+) , rad52Δ (rad52::LEU2) , swi1-5FLAG (swi1-5FLAG::kanMX6), swi1-13Myc (swi1-13Myc::kanMX6), rad52-YFP (rad52-YFP::ura4+) , rad52-12PK, trt1-G11-9FLAG , ade3::[kanr-ura4+-lacO], ade1::[kanr-ura4+-lacO] [62, 63]. Strains containing the following gene deletions were obtained from National BioResource Project Japan and used to generate various strains used in this study: swi6Δ (swi6::kanr, FY13724), est1Δ (est1::kanMX, FY14265), poz1Δ (poz1::hyg, FY18508), and rif1Δ (rif1::ura4+, FY14160).
Genomic DNA was digested overnight with the indicated restriction enzymes, and separated on an agarose gel using 1x Tris-Acetate-EDTA buffer. DNA from the agarose gel was transferred to a Hybond-XL membrane (GE Healthcare, Little Chalfont, UK) using buffer containing 0.5 M NaOH and 1.5 M NaCl. The membrane was then UV cross-linked using an XL-1000 UV Crosslinker (Spectronics, Westbury, NY) and incubated with a DNA probe labeled with [α-32P] dCTP. Hybridization was carried out overnight in Church buffer at 65°C as described . Membranes were exposed for 2 days to a Phosphorimager screen, and detection of telomere or LacO repeats was done using a Storm 840 Phosphorimager (GE Healthcare). The DNA probe for the detection of telomere repeats by Southern blotting has been described previously . For detecting LacO repeats, the 316-bp XbaI fragments that contain LacO repeats were excised from the pSV2-DHFR-8.32 plasmid  and used as a probe. The 448-bp PvuII fragment from the pJK148 backbone  was used as a probe to detect the DNA fragment containing the internal telomere tract.
Chromatin immunoprecipitation (ChIP) assay
ChIP assay and its quantification in all figures except for Fig 2D were carried out as described previously [123–125] with modifications. Briefly, exponentially growing cells were fixed in 3% paraformaldehyde, and chromatin was sheared into 500 to 700-bp fragments using a Misonix Sonicator 3000 (Qsonica, Newtown, CT). Chromatin-associated proteins were then immunoprecipitated using mouse monoclonal anti-V5/Pk SV5-Pk1 (AbD Serotec, Kidlington, UK) or anti-FLAG M2 (Sigma-Aldrich, St. Louis, MO) antibodies in combination with Protein G-coupled Dynabeads (Life Technologies, Carlsbad, CA). DNA extracted from the immunoprecipitates was subjected to PCR analysis, and the PCR products were separated on a 4% polyacrylamide gel. The gel was stained with SYBR Green I (Life Technologies) and analyzed with Storm 840 Phosphorimager (GE Healthcare). Relative enrichment of the target sequences was calculated by multiplex PCR including primers that amplify a gene-free region (GFR)  as internal control as described previously [123–125]. ChIP assay described in Fig 2D was performed using the anti-myc 9E10 monoclonal antibodies (Cell Signaling Technology, Danvers, MA) as previously described [90, 92, 127]. PCR primers used in our ChIP studies are listed in S2 Table.
ChIP sequencing was performed as described  with some modifications. ChIP samples from non-tag control (SP1173), rad52-12PK (Y4250) and rad52-12PK swi1Δ (Y4256) strains were obtained from asynchronous cultures as [128, 129]. Quality of the ChIP samples was assessed by PCR using primers that are designed to amplify tel3s (10 μM), rDNA (2.5 μM, 10 μM), and rec8 (10 μM) loci. DNA amount was quantified using Qubit dsDNA HS assay kit (Invitrogen) and a Qubit 2.0 Fluorometer (Invitrogen). For each sample, 3.1 ng of DNA were used for library preparation. The library preparation for Illumina sequencing was done using NEBnext ChIP-seq Library Prep Master Mix Set for Illumina (New England Biolabs) following their protocol. Final DNA samples were quantified using Qubit dsDNA HS assay kit (Invitrogen) and a Qubit 2.0 Fluorometer (Invitrogen), and 120 ng of library DNA for each sample was submitted to the sequencing facility for analysis using Illumina HiSeq2000 (Illumina). Sequences were processed by the Illumina analysis pipeline version 1.6.1, and aligned to the fission yeast sequence (version ASM294v1.18). Data was visualized with Integrated Genome Browser 
Telomere dysfunction-induced focus (TIF) analysis by fluorescent microscopy
Cells expressing Rad52-YFP and Taz1-mCherry from their own promoters were grown at 25°C in Edinburgh minimal medium (EMM) with necessary supplements until mid-log phase. Cells grown at 25°C have more stable fluorescence with lower background signals. Live-cell imaging analysis of Rad52-YFP and Taz1-mCherry localization was performed using an Olympus PROVIS AX70 microscope equipped with a Retiga EXi camera (QImaging, Surrey, BC, Canada). Images were acquired with iVision software (BioVision Technologies, Exton, PA) and analyzed with ImageJ software (National Institutes of Health, Bethesda, MD). At least 100 cells were counted for each experiment.
(A) To obtain the TIF ratio over total Rad52 foci, the number of total TIF events was divided by the total number of Rad52 foci in wild-type and swi1Δ cells. The TIF ratio in swi1Δ cells was more than double that of wild-type cells. (B) Representative microscopic images of the lateral localization of Taz1 and Rad52 are shown. Pink arrows indicate the occurrence of lateral localization events. These lateral cases were not considered as TIFs.
(A-C) Quantification of signal intensity of representative Southern blots of ApaI digested telomere fragments from wild-type (A), swi1Δ (B) and trt1Δ (C). Each image shows data of telomere lengths from DNA obtained after 1, 4, or 8 restreaks. Telomere fragments were detected using a telomere-specific probe as described in Fig 2B. Signal intensity quantification was performed with ImageJ software.
S3 Fig. swi1Δ trt1Δ cells show ALT-like phonotype.
Southern blot analysis of telomere fragments from the indicated mutants. Strains were obtained by tetrad dissection. Genomic DNA was prepared after 1, 4, or 8 restreaks after the indicated strains were generated. ApaI-telomere fragments were detected using a telomere-specific probe as described in Fig 2B. A representative result is shown.
S1 Table. S. pombe strains used in this study.
We thank Atsunari Tanaka, Chiaki Noguchi, Prajakti Awade, and Jose Luis Fernandez-Garcia for technical assistance; Paul Lieberman, Jane Clifford, Mauricio Reginato, and Christian Sell for comments and advise; Antony Carr, Paul Russell, Kenneth Sawin, and National BioResource Project Japan for S. pombe strains and plasmids. Members of the Noguchi laboratory are thanked for their support and encouragement. Illumina sequencing analyses were supported by the Wistar Institute Genomics Facility.
Conceived and designed the experiments: MCG TMN EN. Performed the experiments: MCG MMD YTC EN. Analyzed the data: MCG HT KiN TMN EN. Contributed reagents/materials/analysis tools: MCG MMD HT YTC KiN EMM EN. Wrote the paper: MCG EN.
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