• We are sorry, but NCBI web applications do not support your browser and may not function properly. More information
Logo of molcellbPermissionsJournals.ASM.orgJournalMCB ArticleJournal InfoAuthorsReviewers
Mol Cell Biol. Oct 2005; 25(20): 8887–8903.
PMCID: PMC1265769

Schizosaccharomyces pombe mst2+ Encodes a MYST Family Histone Acetyltransferase That Negatively Regulates Telomere Silencing


Histone acetylation and deacetylation are associated with transcriptional activity and the formation of constitutively silent heterochromatin. Increasingly, histone acetylation is also implicated in other chromosome transactions, including replication and segregation. We have cloned the only Schizosaccharomyces pombe MYST family histone acetyltransferase genes, mst1+ and mst2+. Mst1p, but not Mst2p, is essential for viability. Both proteins are localized to the nucleus and bound to chromatin throughout the cell cycle. Δmst2 genetically interacts with mutants that affect heterochromatin, cohesion, and telomere structure. Mst2p is a negative regulator of silencing at the telomere but does not affect silencing in the centromere or mating type region. We generated a census of proteins and histone modifications at wild-type telomeres. A histone acetylation gradient at the telomeres is lost in Δmst2 cells without affecting the distribution of Taz1p, Swi6p, Rad21p, or Sir2p. We propose that the increased telomeric silencing is caused by histone hypoacetylation and/or an increase in the ratio of methylated to acetylated histones. Although telomere length is normal, meiosis is aberrant in Δmst2 diploid homozygote mutants, suggesting that telomeric histone acetylation contributes to normal meiotic progression.

DNA is packaged into histone-containing nucleosomes and from there into higher order chromatin structures (45, 50). Not surprisingly, the enzymes that modify chromatin have diverse roles in the cell that affect multiple DNA-dependent events, including transcription, repair, and replication (8, 12, 32, 40, 43, 74). In particular, histones are subject to covalent modifications, including phosphorylation, methylation, ubiquitylation, sumoylation, and acetylation. These modifications create an epigenetic “histone code” that targets chromatin for transcriptional activation or repression, changes in genome stability, response to DNA damage, or differentiation (24, 32, 41, 76, 88).

Histone acetylation on lysine residues in the histone tails is the most extensively studied of these chromatin modifications. Acetylation on different lysines is achieved by a balance in activity of histone acetyltransferases (HATs) and histone deacetylases (27, 41, 75, 76). HAT enzymes can be divided into several broad groups based on their conserved sequence domains. Two large families are the GNAT group, including Gcn5/PCAF, and the Moz-Ybf2/Sas3-Sas2-Tip60 group (MYST) family, and there are several smaller groups, including the TAF1, CBP/p300, SRC-1, and HAT1 enzymes (14, 53).

The MYST family of HATs has been closely examined in the budding yeast Saccharomyces cerevisiae, which has three members: Esa1p, Sas2p, and Sas3p (2, 16, 21, 43, 74, 81). ScESA1 encodes an essential HAT that primarily modifies nucleosomal histone H4, and conditional mutants undergo RAD9-checkpoint-dependent arrest with 2C DNA content (16, 74). The protein is part of the NuA4 and piccolo complexes required for transcriptional activation as well as for double-strand break repair (2, 8, 11, 19). ESA1 interacts genetically with members of the nucleosome assembly complex SPN/FACT (26) and physically with DNA polymerase α (25, 26, 43, 67, 91, 92). In addition to its HAT domain, it contains a chromodomain, a motif implicated in assembly of large complexes on specific regions of chromatin (12). In contrast, ScSas2p and ScSas3p lack chromodomains. ScSas2p is part of the SAS-I protein complex and interacts with chromatin assembly factors (56, 68). As well as affecting silencing, ScΔsas2 suppresses temperature-sensitive (ts) mutations in the origin recognition complex (ORC) subunits ORC2 and ORC5 (21). ScSas2p antagonizes the silencing factor ScSir2p, such that sas2 mutants lead to wider distribution of Sir2-mediated silencing at telomeres (49, 78). ScSas3p is a component of the NuA3 complex which also interacts physically with the SPN/FACT complex (43). ScΔsas3 is synthetically lethal with ScΔgcn5, a GNAT family HAT, suggesting the proteins overlap to acetylate histone H3 (38).

In humans, there are additional members of the MYST family. These include Tip60p (which binds to and is repressed by the human immunodeficiency virus type 1 Tat protein), the Mozp (monocytic leukemia zinc finger) protein, which is involved in translocations in acute myeloid leukemia, and the related Morfp factor (32, 85). The recently identified Hbo1 protein also falls into this class (13, 40). All these proteins contain the conserved MYST domain. In addition, Tip60p contains a chromodomain; this motif is also found in ScEsa1p, making these likely orthologues. Mozp and Morfp contain PHD and H15 domains, while Hbo1p contains a zinc finger. These additional domains are not found in ScSas2p and ScSas3p, suggesting there may be some functional divergence between the fungal and metazoan MYST proteins.

Regulated histone acetylation and deacetylation is closely associated with transcriptional activity and particularly in the formation of constitutively silent heterochromatin (59). The protein complexes and histone modifications between heterochromatic regions in budding and fission yeast are different (39, 57). Silencing in S. cerevisiae is mediated by Sir-containing complexes, whereas silencing in Schizosaccharomyces pombe is mediated primarily by Swi6p-containing complexes (39). Fission yeast heterochromatin contains hypermethylated histone H3 K9, whereas budding yeast histone H3 K9 is not methylated (6, 61, 77). Furthermore, a recent report using histone mutants showed that the formation of Swi6-dependent heterochromatin at centromeres is mediated mainly by modifications of the histone H3 tail, whereas Sir3-dependent heterochromatin in budding yeast relies on hypoacetylation of H4 tails and, in particular, of H4 K16 (57). Thus, although both fission and budding yeast require specific histone modification and binding of specialized proteins to assemble heterochromatin, there are substantial differences in the actual modifications and proteins involved (57).

Recent studies also link histone acetylation with DNA replication proteins. The human MYST family member Hbo1p interacts with replication proteins Mcm2p and Orc1p (13, 40). Increased histone acetyltransferase activity correlates with the onset of DNA replication in rat liver cells (89), and histone acetylation facilitates replication elongation in vitro (1). Overexpression of a member of the Gcn5-containing HAT complex partially suppresses the ts phenotypes of an mcm5 mutant (20). Unexpectedly, some budding yeast mcm5 mutants also have defects in telomeric silencing (20), which may implicate replication proteins more directly with silencing.

Based on the differences in heterochromatin in fission and budding yeasts and our long-standing interest in replication, we looked for MYST family HATs in the fission yeast genome. We identified two, which we call Mst1p and Mst2p. Mst1p is an essential protein structurally similar to ScEsa1p and Tip60p. Mst2p is nonessential and clearly related to both ScSas2p and ScSas3p. In this report, we further analyze the phenotypes associated with Δmst2 and find that loss of Mst2p leads to an increase in telomere silencing. This effect appears to be independent of other S. pombe proteins that influence telomere structure and silencing, including Swi6p, Sir2p, Taz1p, and Rad21p. Instead, our data suggest that the ratio of acetylated to unacetylated histones changes the boundary of silencing at the telomere. The Δmst2 mutants suffer a disordered meiosis that might also reflect loss of normal telomere functions. This study suggests a distinct function for SpMst2p in the regulation of telomere function.


Strains and manipulations.

Strains used in this study are listed in Table Table1.1. Strains were grown and maintained on yeast extract plus supplements (YES) or Edinburgh minimal medium (EMM) with appropriate supplements, using standard techniques (60). Matings were performed on synthetic sporulation agar (SPAS) (35) plates for 2 to 3 days at 25°C. Temperature-sensitive cells were grown at 25°C, and non-ts cells were grown at 32°C. Transformations were carried out by electroporation (48). Double mutants were constructed by standard tetrad analysis or random spore analysis. G418 plates were YES supplemented with 100 μg/ml G418 (Sigma).

S. pombe strains used in this study

Disruption and tagging of mst1+ and mst2+.

To disrupt S. pombe mst1+ (SPAC637.12c) and mst2+ (SPAC17G8.13c) genes, their upstream and downstream regions were amplified by PCR using primers mst1/5′UTR-F (CCCCGAGCTCTTTCTGTTCACCCATACCTGTGGC/SacI overhang), mst1/5′UTR-R (GGGGGTACCGTCTCAATAAGTGGATACTTATTCC/KpnI overhang), mst1/3′UTR-F (AAAAAACTGCAGGTACAAAGAATGGATTAGATGCTGG/PstI overhang), and mst1/3′UTR-R (CCCCAAGCTTCCACTATAGACATCCCTGTACCAC/Hind III overhang) for mst1 and mst2/5′UTR-F2 (TTTAGAGCTCGCTAGTATTGTCTGGGATGACTTG/SacI overhang), mst2/5′UTR-R2 (GGGGGTACCTTTGAACTGGCTGTGGATTTC/KpnI overhang), mst2/3′UTR-F (AAAAAACTGCAGCTCTCATCATCTGGATTCCGTTTAG/PstI overhang), and mst2/3′UTR-R (CTAAAGCATGCAAAGGGGTAAGAATAGCATCAGTGG/SphI overhang) for mst2 and were subcloned into our pTZura4+ vector, creating pEBG78 for mst1 and pEBG79 for mst2. These plasmids were digested, and the corresponding disruption fragments were used to transform a ura4/ura4 wild-type diploid. Ura+ stable transformants were sporulated and analyzed. Δmst1::ura4+/mst1+ tetrad analysis showed two Ura viable spores and two inviable spores, presumably Ura+, indicating that mst1+ is an essential gene. Δmst2::ura4+ haploids were viable, and strains FY1889 and FY1890 were generated. Disruption of mst2 was confirmed by Southern blotting (unpublished data). To disrupt mst2 with kanMX6, plasmid pEBG95 was constructed by replacing the pEBG79 ura4+ gene with the kanMX6 cassette and then digested, and the disruption fragment was used to transform wild-type strain FY254. Stable G418-resistant transformants were isolated, generating FY2952 (Δmst2::kanMX6). Disruption of mst2 with kanMX6 was confirmed by PCR (unpublished data). Δmst2::ura4+ and Δmst2::kanMX6 cells behaved similarly in all physiological assays.

Strains FY1812 and FY1818 expressing Mst1-HA and Mst2-HA, respectively, from their own locus and endogenous promoter were constructed as follows. Plasmids pEBG72 (nmt-mst1-HA) and pEBG73 (nmt-mst2-HA) were constructed by PCR amplifying and subcloning mst1+ and mst2+ genes into the triple-hemagglutinin (HA)-tagging nmt expression vector pSLF172 (28). Next, plasmids pEBG72 and pEBG73 were digested with AccI/SmaI and HincIII, respectively, and the fragments containing the 3′ end of the tagged genes were subcloned into pJK148 (47), creating pEBG80 (mst1) and pEBG90 (mst2). Following linearization with BclI (mst1) and StuI (mst2), pEBG80 and pEBG90 were integrated into the mst1 or mst2 locus, respectively, creating a partial tandem duplication with the full-length copy expressing the tagged protein and an unexpressed gene fragment. Expression of the tagged proteins was confirmed by Western blotting (unpublished data).

The protein sequence alignment and phylogenetic tree for the MYST family members were generated using Clustal X (ftp://ftp-igbmc.u-strasbg.fr/pub/ClustalX/) and Phylip (http://evolution.genetics.washington.edu/phylip.html). BLAST 2 sequence alignment was used to calculate the percentage identities, similarities, and gaps between the MYST domains of Mst2p and the other MYST family members (84).

In situ chromatin binding assay.

An in situ chromatin binding assay was performed as described previously (31). Cells were mounted and stained with 4′,6-diamidino-2-phenylindole (DAPI). Microscopy was performed with a Leica DMR microscope. Images were captured with a Hamamatsu digital camera using Improvision Openlab software and assembled in Canvas 8.0 (Deneba).

UV, TBZ, HU, and MMS sensitivity assays.

Cells were grown to an A595 of 1, serially diluted fivefold, and spotted onto YES plates or YES plates containing 10 μg/ml thiabendazole (TBZ), 5 mM hydroxyurea (HU), or 0.005%, 0.007%, and 0.01% methyl methanesulfonate (MMS) and incubated for 3 to 5 days at 25°C or 32°C. For UV irradiation assays, 1,000 cells were plated in duplicate onto YES and immediately treated with the indicated doses of UV irradiation using a Stratalinker (Stratagene). Control plates were left untreated. Plates were incubated at 32°C for 2 to 3 days. Colonies were counted, and percentage survival was obtained relative to the number of colonies grown on the untreated control plates.

Silencing assays.

To analyze silencing using the ade6+ marker, mutant strains were crossed to wild-type cells that had the full-length ade6+ gene inserted in the different heterochromatic regions and a truncated ade6 gene at the ade6 endogenous locus (ade6ΔN/N). The presence of full-length ade6+ and ade6ΔN/N was verified by PCR using the following primers: ade6-F, 5′-CCAGGAAAGTGTTGAAAAAG, and ade6-R, 5′-CTTCAAACTGAGAAGTTGGG. Wild-type strains FY2328, FY2996, and FY2997, Δmst2 strains FY2364 and FY2365, Δsir2 Δmst2 strain FY2700, Δsir2 strain FY2702, Δtaz1 strain FY2367, Δmst2 Δtaz1 strains FY3298 and FY3299, Δswi6 strain FY3293, and Δmst2 Δswi6 strain FY3295 were used for telomeric silencing assays. For TM(cnt) centromeric region analysis, wild-type FY3036 and Δmst2 FY3039 strains were used, and for the outer repeat region (otr), wild-type FY2219 and Δmst2 FY2412 strains were used. For the mating type region, wild-type FY3001 and Δmst2 FY3003 strains were used. To analyze colony color, cells were streaked on EMM plates lacking leucine and uracil and containing a low concentration of adenine (low adenine; 7.5 μg/ml) and were incubated for 3 days at 32°C. To analyze telomeric silencing using the ura4+ reporter, Δmst2::kanMX6 mutants were crossed to cells carrying minichromosome Ch16-M23 with the ura4+ marker inserted immediately after the telomeric repeats, and for the analysis of the “native” telomere the mutants were crossed to cells with ura4+ inserted 300 bp from the left telomere of chromosome 1, tel1L::ura4+. For centromeric inner (imr) region silencing analysis, Δmst2::kanMX6 mutants were crossed to cells with ura4+ inserted in the imr region of centromere 1. Wild-type FY3043 and Δmst2 FY3044 were used for telomeric silencing assays using the ura4+ reporter. Wild-type FY1589 and Δmst2 FY3046 were used for inner centromeric silencing (imr::ura4+). Cells were grown to an A595 of 1, serially diluted fivefold, spotted onto YES, EMM-ura, or EMM supplemented with 1 mg/ml 5-fluoroorotic acid (5-FOA) and incubated for 3 to 4 days at 32°C.

Telomere length analysis.

Strains FY1421 (Δtaz1), FY1204 (Δrhp51), FY2056 (Δswi6), FY1889 (Δmst2), and FY258 (wild type) were grown for 50 generations, and genomic DNA was isolated. Fifteen micrograms of DNA was digested with EcoRI, separated on a 1% agarose gel, and analyzed by Southern blotting using as a probe the G-specific oligonucleotide 5′-GGGTTACAGGTTACAGGTTACA-3′ (17).

RNA purification and reverse transcriptase PCR (RT-PCR) analysis.

Cells were grown to an A595 of 0.5 to 0.7. Total RNA was extracted with the RNeasy kit (Invitrogen) following the manufacturer's instructions. RNA was quantified, and its integrity was checked by agarose gel. First, cDNA strand was prepared with equal concentrations of total RNA using the Superscript First Strand Synthesis System for RT-PCR kit (Invitrogen), following the manufacturer's instructions, and was used in PCR amplifications. The expression of the full-length ade6+ (tel::ade6+) and the truncated ade6ade6) gene were quantified by real-time quantitative PCR using SybrGreen (Applied Biosystems) as a marker for DNA amplification on an ABI Prism 7900HT apparatus (Applied Biosystems). Primers used specifically amplify full-length ade6+ or the truncated mini-ade6 (Table (Table2)2) and were designed with Primer Express software (Applied Biosystems). Quantified cDNA was used to obtain a standard curve to estimate the amount of DNA in each sample. Results are plotted as fold expression relative to the wild type after normalization to 18S rRNA values.

Quantitative PCR primers used in this study

Chromatin immunoprecipitation (ChIP) assay and real-time quantitative PCR analysis.

ChIP was performed as described previously (29). Antibodies used are as follows: anti-tetra-acetyl histone H4 (Upstate), anti-acetyl lysine 9 histone H3 (Upstate), and anti-dimethyl lysine 9 H3 (Upstate) were used to precipitate modified histones; rabbit anti-myc (Santa Cruz) was used to precipitate Sir2-myc; monoclonal anti-HA (Covance) was used to precipitate Taz1-HA, Rad21-HA, and Mst2-HA; and affinity-purified anti-Swi6 antibodies were used to precipitate Swi6p. Immunoprecipitated DNA was analyzed by real-time quantitative PCR using SybrGreen (Applied Biosystems) as a marker for DNA amplification on an ABI Prism 7900HT apparatus (Applied Biosystems). Values obtained with the untagged or no antibody immunoprecipitation were subtracted from the corresponding values. Input DNA was used to obtain a standard curve to estimate the amount of DNA in each sample. Data were graphed as the percentage of immunoprecipitated DNA with respect to the total input DNA used in each immunoprecipitation. Primer Express software (Applied Biosystems) was used to design primers used for real-time quantitative PCR analysis and are shown in Table Table22.

Meiosis time course.

Wild-type strains FY253 and FY258 and Δmst2 strains FY1889 and FY1890 were mated on SPAS plates for 12 h at 25°C and streaked onto plates lacking adenine to select for diploids. Colonies were streaked on YES and replica plated to YES plus phloxin B. Dark pink colonies (diploid cells) were isolated and streaked on YES. Eight independent Δmst2 diploids and four independent wild-type diploids were patched on SPAS plates at 25°C to induce meiosis and ethanol fixed after 15 h. Cells were stained with DAPI, and 200 asci per diploid were analyzed. Asci with more than four DAPI spots or unequal DAPI-stained bodies were considered “abnormal asci.” Normal asci were those with four equal DAPI-stained bodies. Cells were visualized with a Leica DMR microscope, and images were captured with a Hamamatsu digital camera and Improvision Openlab software (Improvision).


S. pombe has two distinct MYST family HAT proteins.

A series of BLAST searches using different MYST domain sequences revealed that S. pombe has two open reading frames, SPAC637.12c and SPAC17G8.13c, with high similarity to MYST family histone acetyltransferases. We named these two putative acetyltransferases Mst1p and Mst2p, respectively. The Mst2p sequence was first identified, but not molecularly characterized, by Reifsnyder et al. (70). Figure Figure1A1A shows a phylogenetic tree and a schematic representation of different MYST family acetyltransferases comparing S. pombe Mst1p and Mst2p with other MYST domain proteins. mst1+ codes for a 463-amino-acid protein, 70% similar to S. cerevisiae Esa1p. Like Esa1p and Tip60p, Mst1p has a chromodomain motif, which is implicated in chromatin association (12, 44). The mst2+ gene encodes a 407-amino-acid protein with homology restricted to the MYST domain and amino acid similarity ranging between 50 to 70% (Fig. (Fig.1A).1A). Mst2p does not contain a chromodomain or other motifs outside of the MYST/HAT domain, similar to S. cerevisiae Sas2p and Sas3p.

FIG. 1.
(A) Phylogenetic tree and schematic alignment showing the relationship between putative MYST family acetyltransferases, S. pombe (Sp) Mst1p (GenBank accession number ...

To characterize Mst1p and Mst2p function, we disrupted the corresponding genes by replacing the open reading frames with the ura4+ marker. Our results show that the mst1+ product is essential (Fig. (Fig.1B),1B), while that of mst2+ is not (data not shown). Similarly, in S. cerevisiae, ESA1 is essential, whereas the other MYST family members, SAS2 and SAS3, are not (16, 70, 74). In Fig. Fig.1A1A the phylogenetic tree shows that SpMst1p and ScEsa1p are closely related proteins, suggesting that they are functional homologs, although expression of ScESA1 could not rescue SpΔmst2 lethality (data not shown). Based on sequence analysis, we cannot clearly determine whether Mst2p corresponds to ScSas2p or to ScSas3p, or, given the absence of a third MYST protein in S. pombe, whether it shares functions with both S. cerevisiae proteins (Fig. (Fig.1A).1A). ScSas2p and ScSas3p are also different from one another (Sas3p is considerably larger). The absence of a third MYST protein in S. pombe may reflect important differences in chromatin organization in these two species.

Mst1p and Mst2p are nuclear and chromatin bound throughout the cell cycle.

To localize Mst1p and Mst2p we tagged the endogenous genes with simian virus 5 and HA epitopes and performed in situ chromatin binding assays (31, 46). Using this technique, we can visualize the localization of proteins in the cell and their association with chromatin. When permeabilized cells are treated with 1% Triton X-100 before fixation for immunofluorescence, proteins not tightly bound to chromatin are released from the nucleus. An example of this method can be visualized with the Mcm2-HA and Orp1-HA control proteins (Fig. (Fig.2A).2A). SpMcm2 is nuclear and binds chromatin at the end of M phase, staying bound through G1 and S (binucleate cells in S. pombe); SpOrp1p is nuclear and binds chromatin throughout the cell cycle. When cells are not treated with the detergent, Mcm2-HA and Orp1-HA are visualized in the nuclei of mononucleate (cells in G2 phase) and binucleate cells (cells in M/G1/S phase); when treated with 1% Triton X-100, Mcm2-HA is only in binucleates, but Orp1-HA is in both mono- and binucleate cells (Fig. (Fig.2A).2A). Both Mst1p and Mst2p behaved like Orp1-HA: they were localized in the nucleus and bound to chromatin throughout the whole cell cycle. Under these experimental conditions we saw no evidence for region-specific localization. The remainder of this report will address the function of nonessential mst2+, and further characterization of mst1+ will be described in a separate report.

FIG. 2.
(A) SpMst1p and SpMst2p are nuclear- and chromatin-bound throughout the cell cycle. The wild type (FY258) and strains expressing Mst1-HA (FY1812), Mst2-HA (FY1818), Mcm2-HA (FY798), and Orp1-HA (FY793) were permeabilized and washed with the indicated ...

Δmst2 genetically interacts with mutants that affect heterochromatin, cohesion, and telomere structure.

Haploid cells lacking mst2+ are viable and have a growth rate similar to that of wild-type cells (data not shown). We investigated whether Δmst2 cells were sensitive to disruptions in chromosome function by examining their sensitivity to a variety of drugs that perturb the cell cycle. We tested the spindle poison TBZ and DNA-damaging agents MMS (alkylating agent), bleomycin (mimetic of gamma irradiation), camptothecin (inhibitor of topoisomerase I), and UV irradiation as well as the DNA synthesis inhibitor HU (Table (Table3,3, Fig. Fig.2B).2B). We observed that Δmst2 cells are modestly sensitive to HU (Fig. (Fig.2B)2B) to about the same degree as a rad21ts strain with a defect in chromosome cohesion but not as sensitive as the checkpoint-defective Δrad3 or the replication mutant hsk1ts. Three different Δmst2 Δrad21ts double mutant isolates are also shown. Growth rate was particularly slow for isolate number 3, suggesting that there may be variability in the phenotype. These double mutants are as sensitive to HU as Δrad3 and hsk1ts cells (Fig. (Fig.2B).2B). Δmst2 mutants were also modestly sensitive to 0.01% MMS to the same degree as Δtaz1 (Fig. (Fig.2D).2D). Figure Figure2D2D also shows an example of higher MMS sensitivity for the double mutant Δmst2 Δtaz1. Two different isolates are shown that differ in growth rate and, because of the synthetic growth defect, grow more poorly than either single mutant on YES. At 0.007% MMS the double mutants start being affected by the MMS concentration, and at 0.01% almost no growth is detected (Fig. (Fig.2D).2D). Δmst2 cells were also modestly sensitive to UV irradiation (Fig. (Fig.2E);2E); again, this was not as severe as a checkpoint mutant Δrad3 but was clearly distinguishable from the wild type. We observed no phenotypes on TBZ and camptothecin plates or after treatment with 5 U/ml bleomycin (Table (Table3,3, Fig. Fig.2C,2C, and data not shown).

Δmst2 genetic interactionsa

To investigate genetic interactions, we crossed Δmst2 cells to mutant strains defective in different biological processes: (i) DNA replication, (ii) DNA damage, S-phase and spindle checkpoint control, and (iii) heterochromatin, cohesion, and telomere structure (Table (Table3).3). We first analyzed the viability of the double mutants; second, we analyzed the ability of the double mutants to grow at different temperatures; and finally we analyzed their sensitivity to HU, TBZ, or MMS compared to the single-mutant parents. We define a genetic interaction between Δmst2 and another mutant as the double mutant growing more poorly than either single mutant in any of the tested conditions listed above and described in Table Table3.3. Examples of genetic interactions are shown in Fig. 2B and D. We did not observe any obvious Δmst2 interactions with DNA replication mutants. However, genetic interactions were found between Δmst2 and rad21ts (9), eso1ts (83), and mis4ts (80), which disrupt sister chromatid cohesion; Δswi6 (22), which disrupts heterochromatin assembly; Δtaz1 (17), which affects telomere structure; and hsk1ts, which encodes a DNA replication kinase with pleiotropic effects on cohesion and repair (5, 30, 54, 82) (Fig. 2B and D, Table Table3).3). These were most striking in a severe slow-growth phenotype (“synthetic sick”) observed for Δtaz1 and taz1-GFP, in contrast to wild-type taz1+ strains. Importantly, this result also suggests that the Taz1-GFP protein is attenuated in function in some way. We also observed synthetic dosage lethality: Δmst2 was sensitive to overproduction of Swi6-GFP, a heterochromatin protein that localizes at centromeres, telomeres, and the mating type loci (22).

Since Taz1p, Swi6p, and proteins involved in cohesion all affect telomere function, we investigated the effect of Mst2p at the telomeres. We compared this to its effect at the centromere and mating type locus, two other well-characterized heterochromatic domains in fission yeast.

Mst2p is a negative regulator of silencing at telomeres.

Silencing in fission yeast has largely been studied in regions of heterochromatin at the telomeres, the centromeres, and the mating type loci (34). Although there are some factors specific for each region, they all share a common pathway that involves sequential deacetylation and methylation of histones, which allows binding of the Swi6/HP1 heterochromatin protein and association of cohesin proteins (6, 7, 61, 66). Swi6p and other components of this pathway are conserved in fission yeast and metazoans but are not found in budding yeast.

We investigated the role of Mst2p in heterochromatin silencing by analyzing the effect of Δmst2 mutation in the expression of a reporter gene when inserted at a telomere, mating type, or centromeric regions cnt (TM), imr, and dg. For telomeric silencing we used a strain that has the ade6+ gene inserted immediately proximal to the telomeric repeat of the minichromosome Ch16-M23 right telomere (62). This minichromosome is a 350-kb derivative of the original 530-kb Ch16-M23 minichromosome (64) and lacks telomere-associated sequence (TAS) elements. The expression of this gene is subjected to position effect variegation, and cells plated on low adenine can exhibit red-pink-white-sectored colonies (Fig. (Fig.3A;3A; see also Fig. S1 in the supplemental material) (3). Cells lacking mst2 and having ade6+ at the Ch16-M23 telomere were streaked on low-adenine plates lacking leucine to select for the minichromosome and were analyzed. Δmst2 cells show a deep red colony color, indicating that Mst2p negatively regulates telomeric silencing (Fig. (Fig.3A;3A; see also Fig. S1 in the supplemental material). The presence of the ade6+ gene and ade6ΔN/N was confirmed by PCR (Fig. (Fig.3B).3B). Similar results were observed for independent isolates, and the phenotype was complemented by plasmid-borne mst2-HA (data not shown). To analyze the expression of the ade6+ gene at the telomere in wild-type and Δmst2 cells, we purified total RNA and used random hexamers to prepare the cDNA strand. Two different amounts of cDNA were used in lineal PCR amplifications, and after 26 cycles only the truncated ade6 transcript (Δade6) could be amplified in wild-type and Δmst2 cells (Fig. (Fig.3B).3B). As a control we used a strain lacking the sir2 gene (see below) and carrying Ch16::LEU2+ tel::ade6+, where the expression of the full-length ade6+ gene at the telomere is derepressed. After 34 cycles, the expression of the full-length ade6+ gene at the telomere of wild-type cells was detected, while no amplification was observed in Δmst2 mutants (Fig. (Fig.3B).3B). We quantified the expression of both the full-length ade6+ gene at the minichromosome telomere and the truncated ade6 at its own locus by using real-time quantitative PCR. We designed primers that would only amplify the full-length ade6+ gene or the truncated one (Table (Table2)2) and used them in real-time quantitative PCR experiments (Fig. (Fig.3C).3C). Data represent fold expression relative to the wild type after normalization to 18S rRNA values. As shown in Fig. Fig.3C,3C, in wild-type and Δmst2 cells the truncated ade6 gene is similarly expressed, while the expression of the full-length ade6+ is approximately 25 times higher in wild-type cells. These results indicate that in Δmst2 cells the expression of the ade6+ gene at the telomere is specifically repressed while no effect is seen in the expression of the truncated ade6 gene located in ade6's own locus.

FIG. 3.
Mst2p negatively regulates telomeric silencing of ade6+. (A) Silencing assay using the ade6+ gene at the telomere of minichromosome Ch16. Wild-type (FY2997), Δmst2 (FY2364), Δtaz1 (FY2367), Δmst2 Δtaz1 (FY3298 ...

To further characterize fission yeast telomere heterochromatin, we analyzed the role of known telomeric proteins on the increased silencing observed in Δmst2. As shown in Fig. Fig.3A,3A, Δtaz1 mutants, which have a telomere silencing defect, showed variegation as reported previously (Fig. (Fig.3A)3A) (17, 63). To make the double mutant Δmst2 Δtaz1, we crossed FY2911 (Δmst2::kanMX6 Ch16 M23::LEU2+ tel::ade6+ ura4 leu1-32 ade6ΔN/N), which has a deep red color on low adenine, to FY1421 (Δtaz1::ura4+ ura4-D18 leu1-32 ade6). The red color observed in Δmst2 cells changed to pink when cells also lacked taz1 (Fig. (Fig.3A),3A), indicating that Taz1p is needed for the increased telomeric silencing observed in Δmst2 mutants.

It was recently shown that the S. pombe sir2+ gene is required for normal telomeric silencing (29, 72). Data from budding yeast suggest that ScSas2p antagonizes ScSir2p, and the increased silencing observed in some budding yeast Δsas2 strains reflects wider distribution of ScSir2p (49, 78). We analyzed the role of SpSir2p in the increased telomeric silencing observed in Δmst2 mutants. As predicted, cells lacking both sir2 and mst2 exhibit a white colony color when streaked in low-adenine plates lacking leucine, indicating that the increased silencing in Δmst2 cells remains Sir2p dependent (Fig. (Fig.3A3A).

S. pombe heterochromatin silencing is mediated primarily by Swi6p-containing complexes (39). As shown in Fig. Fig.3A,3A, Δswi6 cells as well as the double mutant Δmst2 Δswi6 show a white colony color when streaked on low-adenine plates lacking leucine, indicating that Swi6p is also needed for the increased silencing observed in Δmst2 cells.

We further investigated the role of Mst2p in telomeric silencing by analyzing the effect of a Δmst2 mutation (Δmst2::kanMX6) on the expression of a ura4+ reporter gene inserted immediately proximal to the telomeric repeat of minichromosome Ch16-M23 (62). This construct also lacks TAS elements. Silencing of ura4+ can be detected by decreased growth on medium lacking uracil or by increased growth on the toxic substrate 5-FOA; loss of silencing is manifested as increased growth on medium lacking uracil and decreased growth on 5-FOA (10). As shown in Fig. Fig.4A,4A, wild-type cells (Ch16 tel::ura4+) can grow on plates lacking uracil and adenine and do not grow on 5-FOA, indicating that in this construct the ura4+ gene located at the telomere is actively transcribed. Four different isolates were analyzed for Δmst2mst2::kanMX6) (Fig. (Fig.4A).4A). All isolates can grow as wild types on plates lacking uracil and adenine, suggesting that cells mutant for mst2 express the ura4+ gene inserted in the minichromosome telomere to levels similar to that of the wild type. Interestingly, all isolates can grow, to different extents, on 5-FOA, indicating that some cells are repressing the expression of the ura4+ gene, consistent with variegated expression. These results show that mst2 deletion causes a slight increase in telomeric silencing when using the ura4+ marker.

FIG. 4.
Mst2p negatively regulates telomeric silencing of ura4+. (A) Silencing assay using the ura4+ gene at the telomere of minichromosome Ch16. The wild type (FY3284) and different isolates of Δmst2 (1, FY3289; 2, FY3290; 3, FY3291; ...

Because the minichromosomes we used to analyze telomeric silencing have an unusual telomere that lacks the TAS sequences, it was important to compare these results to those obtained when the ura4+ gene was inserted in a normal telomere. Strain FY1592 has the ura4+ marker inserted in the TAS of the chromosome I left telomere (R. Allshire, personal communication). We asked whether deleting mst2mst2::kanMX6) would also affect the expression of ura4+ when using this telomeric construct. As shown in Fig. Fig.4B,4B, Δmst2 strains grow slightly less on plates lacking uracil and have slightly increased growth on 5-FOA, indicating that mst2 deletion causes a slight increase in telomeric silencing when using this construct. We further analyzed the expression of the full-length ura4+ gene at the telomeres and the truncated mini-ura4 in both these constructs (Fig. (Fig.4C).4C). No differences can be detected between wild-type and Δmst2 strains, although some cells can indeed grow on 5-FOA. These results show that by analyzing a population of cells where the majority is expressing the ura4+ gene from the telomere (growth without uracil), the few cells that silence the expression of the ura4+ marker (growth on 5-FOA) cannot be detected. The modest effects using the ura4+ marker contrast with the striking increase in silencing observed with the ade6+ gene on the minichromosome Ch16-M23 (Fig. (Fig.3),3), suggesting that the use of different promoters and reporter genes can reveal or mask the effect of a mutation.

To extend our analysis of the role of Mst2p in silencing, we also analyzed the effect of Δmst2 in the expression of the ade6+ gene at other heterochromatic regions: the mating type and the central domain, cnt, and the outer repeat, dg, of the centromere. No difference in colony color was observed between wild-type and Δmst2 cells when streaked on low-adenine plates (data not shown). Similarly, when using the ura4+ gene inserted in the centromeric inner (imr) region, there was no difference in growth on plates lacking uracil or with 5-FOA between wild-type and Δmst2 cells (Fig. (Fig.4B).4B). Similar results were observed for independent isolates (data not shown). Taken together, these results indicate that Mst2p is a negative regulator of telomeric silencing and does not affect heterochromatin at the centromere or the mating type.

Mst2p does not affect telomere length.

Silencing at telomeres is affected by general heterochromatin factors, such as Swi6p (4), as well as specific telomere factors that influence telomere length, such as Taz1p (17). Because Δmst2 cells have increased silencing at telomeres, we investigated telomere length in these mutants. We compared the telomere lengths of Δmst2 to telomeres in wild-type, Δtaz1, and Δswi6 cells. As a control for slight changes in telomere length we used Δrhp51 mutant cells. Figure Figure4D4D shows that Δmst2 telomere length is similar to that of the wild type and Δswi6 (23), indicating that Mst2p does not have a role in telomere length control. As previously shown, Δtaz1 has very long telomeres (17). We observe that Δrhp51 has slightly longer telomeres than the wild type; this is in contrast to a previous report (90) but has been seen by others (S. G. Pasion, personal communication) and could reflect some uncharacterized strain differences. These results show that the effect of Mst2p on telomere silencing is independent of telomere length control and, presumably, independent of Taz1p and suggests that Δmst2 and Δtaz1 have synthetic growth defects because they independently affect separate aspects of telomere function.

Mst2p does not affect the heterochromatic localization and distribution of Swi6p, Rad21p, Sir2p, and Taz1p.

Our silencing experiments indicate that Mst2p is a negative regulator of telomeric silencing and requires Sir2p and Swi6p for these effects. However, we found that mst2 affected expression of reporters in different telomere constructs quite differently. In an independent approach, we therefore examined the effect of Mst2p on normal wild-type telomeric chromatin unperturbed by any reporter constructs and created a map of histone modifications and localization and distribution of telomeric proteins by ChIP and real-time quantitative PCR (Fig. (Fig.5A).5A). This provides the first detailed census of proteins and histone modifications in the context of a normal, fully wild-type telomere. We compared this to the effect of Mst2p on centromeric and mating type heterochromatin regions (Fig. (Fig.5B5B).

FIG. 5.FIG. 5.
Mst2p positively regulates telomeric histone acetylation. ChIP and real-time quantitative PCR were carried out to analyze the heterochromatic localization and distribution of Swi6p, Rad21-HA, and Taz1-HA proteins as well as modified histones in wild-type ...

We designed primers to amplify different amplicons within a 20-kb region adjacent to the telomeric repeats of chromosomes 1 and 2, the four centromeric regions, cnt, imr, dg, and dh, of chromosome 1, and the K-repeat heterochromatin between mat2 and mat3 in the mating type region. As a control for a nonheterochromatic region, primers to the fbp1+ promoter were used. Transcription of the fbp1+ gene is regulated in response to glucose concentration in the medium. When S. pombe cells sense a high concentration of extracellular glucose, they activate the cyclic AMP-dependent kinase (protein kinase A) and repress transcription of genes such as fbp1+ (36, 37). In our assay, cells were grown in YES so that the fbp1+ gene would be in its repressed state.

We examined association of the telomeric proteins Swi6p, Rad21p, Sir2p, and Taz1p, which are known to be involved in telomeric silencing; we already showed that mutations in these show genetic interactions with Δmst2 (Table (Table33 and data not shown). We observed no difference between wild-type and Δmst2 cells in the localization and distribution of Swi6p, Rad21p, Taz1p (Fig. (Fig.5A),5A), and Sir2p (data not shown) (29) in any of the heterochromatic regions analyzed. Thus, within the resolution of this experiment, Mst2p does not influence the localization of known heterochromatin or telomere proteins, and its effects on silencing are likely to be mediated by other means or at a subtle level beneath our detection threshold.

Interestingly, we found Swi6p distribution in telomeres changed with the mating type, although the total amount of Swi6p in the cells was similar (see Fig. S2 in the supplemental material). h strains had ~3-fold more Swi6p in the telomeric region located 6.2 kb from the telomeric repeats, with a modest but still detectable difference observed in the 7.1-kb region (Fig. (Fig.5A).5A). Thus, in h strains Swi6p levels are low 0.38 kb from the telomeric repeats, slightly increase towards the 2.6-kb region, and show an abrupt increase at 6.2 kb before dropping back to levels similar to those in the 2.6-kb region (Fig. (Fig.5A).5A). Similar to h strains, h+ cells are enriched for Swi6p 0.38 kb from the telomere end and slightly increased 2.6 kb from the repeats, but at 6.2 and 7.1 kb the levels only slightly increased (Fig. (Fig.5A).5A). Swi6p localization and distribution have recently been reported for h+ cells (29). In light of this unexpected result, we analyzed silencing in h and h+ strains using Ch16-M23 tel::ade6+. No differences were observed in colony color after streaking cells onto low-adenine plates (see Fig. S1 in the supplemental material), which suggests that this difference in the levels of Swi6p does not affect silencing.

Rad21p levels are low proximal to the telomere end but start increasing 9 kb away from the repeats and reach a maximum level 12.2 kb from the telomere, after which they plateau (Fig. (Fig.5A).5A). Interestingly, although it was shown that Rad21p cohesin binding to heterochromatin is Swi6p dependent (7), these proteins do not have the same telomeric distribution; furthermore, there are no differences between h+ and h strains. However, at centromere I and the mating type region, Swi6p and Rad21p show similar distribution patterns, as expected (Fig. (Fig.5B)5B) (7, 69).

Taz1p is highly enriched close to the telomeric repeats (0.38 kb), drops in abundance in the region between 2.6 kb and 9 kb, and is almost undetected 10.6 kb away from the telomeric repeats (Fig. (Fig.5A).5A). Similar results were recently published by Sadaie et al. and Freeman-Cook et al. (29, 71). We found no difference in h and h90 strains. We also found no difference in Sir2p heterochromatin localization and distribution in mst2 compared to what we observed in the wild type (29 and data not shown).

Mst2p positively regulates telomeric histone acetylation.

Since Mst2p had no strong effect on distribution of telomeric heterochromatin proteins, we next analyzed histone modifications in heterochromatic regions. We used antibodies to acetylated histone H4 (H4Ac), acetylated lysine 9 histone H3 (H3K9-Ac), and methylated lysine 9 histone H3 (H3K9-Me) in ChIP experiments, followed by real-time quantitative PCR analysis. For H4 and H3 K9 acetylation we analyzed the same heterochromatic regions as described above for h and h+ strains; no differences between mating types were observed with either antibody. For H3 K9 methylation we only analyzed telomeric heterochromatin in h strains. When using this antibody no differences were observed between the wild type and Δmst2. Histone H3 K9 methylation increases with the distance from the telomeric repeats, following a similar pattern as the one observed for Rad21p (Fig. (Fig.5A5A).

Our analysis using H4Ac and H3K9-Ac antibodies showed that in wild-type cells, histone acetylation increases steadily with the distance from the telomeric ends with a pronounced transition to higher levels occurring between 15.6 and 16.9 kb. In Δmst2 mutants, histone acetylation also increases with the distance from the telomeric repeats, reaching a maximum in the 10.6- to 12.2-kb region (Fig. (Fig.5A).5A). However, the sharp transition to higher levels is not seen, and in the region beyond 16.9 kb, levels are reduced by ~2.5-fold (Fig. (Fig.5A).5A). Thus, Mst2p affects the acetylation state of this region. We examined the sequence in this transition region and found it contains a pseudogene (SPAc212.09c) with two frameshifts (93) (Fig. (Fig.5A).5A). In contrast, no difference in histone acetylation was detected between wild-type and Δmst2 cells in the centromeric and mating type regions (Fig. (Fig.5B).5B). This suggests that region-specific differences distinguish the telomeres from other heterochromatic loci.

Homozygous Δmst2 diploid cells have meiotic defects.

Silencing and ChIP experiments suggest that cells lacking mst2 have some telomere abnormalities. Telomeres are crucial during meiosis at several levels. Telomere-led movement, or “horse-tailing,” is necessary for correct chromosome pairing (94), and many telomere mutants disrupt normal meiotic progression (for examples see references 15, 18, and 63). Since many Δmst2 phenotypes presented above are subtle, we reasoned that meiosis might sensitize the cells to any Δmst2-associated telomeric defects. Wild-type and Δmst2mst2 diploids were induced to undergo meiosis, and after 15 h they were ethanol fixed and DAPI stained. As shown in Fig. Fig.6,6, Δmst2mst2 diploids have ~28% abnormal asci. The majority of the abnormal asci had more than four DAPI spots and unequal DAPI-stained bodies, suggesting that they have mis-segregated or fragmented their chromosomes during meiosis. Wild type/wild type was indistinguishable from Δmst2/wild-type heterozygous diploids, with only 6% abnormal asci, so there is no haploinsufficiency (Fig. (Fig.66 and data not shown). When intact spores from tetrads were dissected or released by random spore analysis, their viability was not significantly reduced, suggesting that the abnormal segregants were not packaged into recognizable spores. Analysis of recombination frequency in the his4-lys4 interval shows no obvious difference between wild-type and Δmst2 diploids (data not shown).

FIG. 6.
Δmst2 homozygote diploids have meiosis defects. Wild-type and Δmst2 homozygote diploids were isolated by mating h and h+ haploid cells and ade6-M210/ade6-M216 complementation. Eight independent Δmst2 diploids and ...

To investigate telomere positioning during meiosis in Δmst2 homozygote diploids, we attempted to visualize endogenous Taz1-GFP or overexpressed Swi6-GFP as described previously (42). However, both of these constructs were problematic. For Taz1-GFP, we crossed Δmst2 haploids with a strain expressing Taz1-GFP from its own locus, but as described in Table Table3,3, we observed a severe growth defect, which suggests that Taz1-GFP is attenuated in function. For Swi6-GFP, we transformed wild-type and Δmst2 haploids with a plasmid expressing Swi6-GFP from the weakest nmt promoter, but the Swi6-GFP expression was toxic for Δmst2 cells. Nevertheless, the disrupted segregation patterns we observe are consistent with defects in meiotic segregation that may represent disruptions in chromosome pairing or meiotic divisions.


In this work we have cloned the genes encoding both S. pombe MYST family histone acetyltransferases, mst1+ and mst2+. Both proteins are constitutively chromatin bound but appear to be broadly distributed and not confined to narrow regions. Interestingly, fission yeast has only two MYST family HATs, while S. cerevisiae has three. In S. cerevisiae, ScEsa1p is the catalytic subunit of the NuA4 and piccolo complexes, capable of acetylating histone H4 and H2A (2, 11, 16, 74). ScSas2p was recently shown to regulate the acetylation of histone H4 K16, preventing Sir3p binding and thus preventing further spreading of telomeric heterochromatin (49, 78). ScSas3p is the catalytic subunit of the NuA3 complex and, together with other HATs, including the Gcn5-containing complexes SAGA and ADA, is responsible for acetylation of histone H3 (33, 43, 51). It is significantly larger than Sas2p, so these genes do not appear to be simple duplicates.

Like its closest homolog, ScEsa1p, SpMst1p is essential for viability, while SpMst2p is not. Further evidence that SpMst1p is the orthologue of ScEsa1p comes from a recent paper characterizing fission yeast Alp5p (ScArp4p) showing that it can interact with SpMst1-myc protein in vivo and is required for global acetylation of histone H4 (58). It will be interesting to determine whether Mst1p is the responsible HAT for this histone H4 acetylation activity.

Which protein is the Mst2p functional homolog in S. cerevisiae? The budding yeast has two proteins with broadly similar structures. Our studies suggest that Mst2p has a role in telomere silencing similar to that of ScSas2p, but we showed that Mst2p affects levels of both histone H4 and H3 K9 acetylation, suggesting that it could be a histone H3 HAT like ScSas3p. However, we found that immunoprecipitated Mst2-HA protein has no HAT activity in in vitro assays (data not shown). Although some reports suggest that neither Sas2p nor the Sas2p-containing complex have HAT activity (2, 16, 43, 49, 56, 68, 74), recent studies showed that the SAS-I complex (Sas2p, Sas4p, and Sas5p) is capable of acetylating free histone H4 K16 and H3 K14 as well as nucleosomal histone H4 (73, 79). These data are consistent with a model that Mst2p is a bona fide histone acetyltransferase, although the identity of its target residues remains unproven.

Significantly, however, there are differences between SpMst2p and ScSas2p. Cells lacking Spmst2 are sensitive to HU, MMS, and UV irradiation (Fig. 2B, D, and E), but Scsas2 mutants are not (21, 68). Δsas2 suppresses some temperature-sensitive orc mutants (21), but Δmst2 does not (Table (Table3).3). Furthermore, we show that Δmst2 cells are not TBZ sensitive per se, but when combined with mutant genes that affect chromosome segregation that are TBZ sensitive, such as rad21ts, Δswi6, eso1ts, and mis4ts, their TBZ sensitivity is enhanced (Table (Table3).3). Thus, Mst2p may have a different spectrum of functions from ScSas2p, although they may overlap.

Cells lacking mst2 show sensitivity to agents including HU and MMS which cause replication fork stalling or pausing during S phase. This effect is synthetic with defects in other proteins, including Rad21p (cohesin), and suggests that Mst2p may play a broader role in genome stability, particularly during S phase.

Most strikingly, we find that Mst2p is a negative regulator of telomeric silencing. Both ade6+ and ura4+ markers are repressed when inserted close to a telomere. This effect was less striking when using constructs with the ura4+ marker at a telomere, suggesting that the use of different promoters and reporter genes can reveal or mask the effect of a mutation. Interestingly, as shown by the RT-PCR analysis, the ura4+ gene at the telomere in both constructs (Ch16 and “native telomere”) is highly expressed compared to the mini-ura4 (Fig. (Fig.4C).4C). In contrast, the ade6+ gene at the telomere of Ch16-M23 in wild-type cells is highly repressed compared to the mini-ade6 (Fig. (Fig.3B),3B), suggesting that the role of Mst2p as a negative regulator of telomere silencing is more evident when using markers with weaker or attenuated promoters. In contrast, we did not observe silencing defects in the centromere or mating type region (Fig. (Fig.5B5B).

In S. cerevisiae, Sas2p and Sas3p can function as either activators or repressors of transcription, depending on the gene context. Mutation of sas2 or sas3 restores silencing to a derepressed HMR locus but enhances silencing defects of the HML locus in a Δsir1 background (21, 70). Loss of sas2 decreases silencing of the URA3 gene when the reporter is inserted near the telomere of the left arm of chromosome VII but increased silencing of this same marker when inserted in the rRNA genes (56, 70). No telomeric functions have been detected for Sas3p (70). Recent reports suggest that ScSas2p can negatively regulate telomeric silencing (49, 78). These reports demonstrate that ScSas2p and ScSir2p have opposing effects on the acetylation of H4 K16 and are needed to maintain the boundary at telomeric heterochromatin (49, 78). However, we did not observe a change in SpSir2p distribution in a Δmst2 mutant (29) (data not shown), although Sir2p is required for silencing in a Δmst2 strain (Fig. (Fig.3A).3A). Thus, Mst2p does not appear to regulate Sir2p directly.

We carried out a detailed analysis of the protein composition and histone modifications of normal fission yeast telomeres I and II in wild-type and Δmst2 cells. We analyzed endogenous telomeres without integrated reporter genes, since we wanted to understand the role of Mst2p on native telomeres and to avoid confusion with different partial telomeric constructs that change the wild-type context. We generated a telomeric map for the distribution of Taz1p, Sir2p, Swi6p, and Rad21p and defined histone acetylation and H3 K9 methylation patterns using ChIP and real-time PCR (Fig. (Fig.55).

As shown previously, Taz1p and Sir2p are highly enriched close to the distal end of the telomere end and decrease in abundance towards the centromere-proximal side (29). We found that Swi6p abundance at specific telomeric regions changes with the mating type; our results suggest that h cells have a surplus of Swi6p that localizes to a specific region within the telomere. Interestingly, no differences in telomeric silencing are observed between h+ and h cells, although these could occur dynamically and not be apparent in our assay.

Fission yeast centromeres and mating type regions have hypermethylated histone H3 K9, and this modification is needed for Swi6p localization (65). In contrast to what is seen at the centromere, the distribution patterns of H3 K9-Me and Swi6p at the telomeres differ from one another. Significantly, in the 6.2-kb region of h strains, high levels of Swi6p do not correlate with hypermethylated histone H3. These results suggest that at the telomere either low levels of methylated histone H3 K9 are sufficient for Swi6p localization or that the mechanism for Swi6p binding to chromatin is different compared to that of the centromere and mating type regions. Telomeric distribution of Taz1p, Sir2p, Swi6p, and Rad21p as well as histone H3 K9 methylation were all independent of Mst2p, although histone H4 and histone H3 K9 acetylation were reduced in the region 16.9 kb from the telomere end (Fig. (Fig.5A5A).

The increased telomeric silencing we observe in Δmst2 may reflect the reduction in histone acetylation or the increased ratio of methylated versus acetylated histones. These data also show that in Δmst2 cells the increase in telomeric silencing is independent of Swi6p, suggesting that other mechanisms must be contributing to silencing at telomeres. A recent study characterizing SpArp6p showed that this protein is involved in telomeric silencing and binds telomeres in an Swi6p-independent manner; moreover, Swi6p localization was not affected in Δarp6 cells. The authors suggest that there is an Arp6p-mediated repression mechanism that works side by side with the Swi6p silencing machinery at telomeres (87). It will be interesting to test if Mst2p affects Arp6p localization and activity at telomeres.

Most intriguing, our work suggests that there may be specific telomere boundary elements in S. pombe. Mst2p affects the histone acetylation of a localized area, starting 16.9 kb from the telomeric repeat and extending at least 2 kb towards the centromere. This increase in histone acetylation could be acting as a barrier for the spreading of telomeric heterochromatin. A study analyzing the Gallus gallus β-globin locus demonstrated that the region immediately surrounding a 16-kb block of heterochromatin had constitutively high levels of histone H3 K9 acetylation, revealing that heterochromatin boundaries can be marked by peaks of acetylated histones (52). ScSas2p and acetylation on histone H4 K16 are proposed to generate a boundary for the spreading of telomeric heterochromatin (49, 78). However, we were unable to immunoprecipitate acetylated histone H4 lysine 16 or ChIP Mst2-HA to the native or the minichromosome Ch16 telomere to test this model (data not shown). Similarly, S. cerevisiae Sas2p was never localized to telomeres, but the evidence highly suggests that Sas2p is the responsible HAT for the H4 K16 acetylation.

Interestingly, the subtelomeric region analyzed in this work is present in two different cosmids, c212 and pT2R1, that have been anchored to chromosomes I and II, respectively, indicating that the high identity between TAS elements of chromosomes I and II goes far beyond 20 kb from the telomeric ends.

Although the changes we saw in wild-type telomeres in Δmst2 were modest, the hypoacetylation of the telomeres and the synthetic growth defect with Δtaz1 implicate Mst2p in normal telomere function. Further, we observed that homozygous Δmst2 diploids have an aberrant meiosis (Fig. (Fig.6).6). Δtaz1 mutants also have severely disrupted meiosis (18, 63), while Δswi6 mutants suffer only very modest defects (86). These data suggest that telomeric acetylation is important for some aspect of fission yeast meiosis. We tested if recombination was affected in this mutant and found that wild-type and Δmst2/Δmst2 diploids have the same recombination frequency in the his4-lys4 interval (data not shown). Because normal telomeres are required for pairing, this function may be disrupted in Δmst2 cells. A second alternative is that meiotic chromosome segregation is abnormal, and a third possibility is that this reflects changes in gene expression. It has been shown that during nitrogen starvation (which induces meiosis), clusters of genes located close to telomeres are up-regulated (55), raising the possibility that disruption of these silent regions may affect a meiotic transcriptional program. Thus, the aberrant meiosis in Δmst2mst2 diploids could be a consequence of downregulation of important subtelomeric meiosis-induced genes in addition to or instead of effects on telomere structure per se. Further examination of telomere structure and expression will be required to determine how this conserved protein affects chromosome function.

Supplementary Material

[Supplemental material]


We thank Karl Ekwall, Robin Allshire, and Junko Kanoh for strains, Sally Pasion for discussion of unpublished results, and Lorraine Pillus, Angel Tabancay, and Will Dolan for helpful comments on the manuscript. We are grateful to Melissa Baker for assistance with the Q-PCR. We thank Ji-Ping Yuan for assistance with meiotic recombination assays. We thank Lorraine Pillus, Beverly Emerson, Dick McIntosh, and Paula Grissom for their hospitality and help to E.B.G. during the course of this work.

This study was supported by NIH grant R01 GM59321 to S.L.F.


Supplemental material for this article may be found at http://mcb.asm.org/.


1. Alexiadis, V., L. Halmer, and C. Gruss. 1997. Influence of core histone acetylation on SV40 minichromosome replication in vitro. Chromosoma 105:324-331. [PubMed]
2. Allard, S., R. T. Utley, J. Savard, A. Clarke, P. Grant, C. J. Brandl, L. Pillus, J. L. Workman, and J. Cote. 1999. NuA4, an essential transcription adaptor/histone H4 acetyltransferase complex containing Esa1p and the ATM-related cofactor Tra1p. EMBO J. 18:5108-5119. [PMC free article] [PubMed]
3. Allshire, R. C., J. P. Javerzat, N. J. Redhead, and G. Cranston. 1994. Position effect variegation at fission yeast centromeres. Cell 76:157-169. [PubMed]
4. Allshire, R. C., E. R. Nimmo, K. Ekwall, J. P. Javerzat, and G. Cranston. 1995. Mutations derepressing silent centromeric domains in fission yeast disrupt chromosome segregation. Genes Dev. 9:218-233. [PubMed]
5. Bailis, J. M., P. Bernard, R. Antonelli, R. C. Allshire, and S. L. Forsburg. 2003. Hsk1-Dfp1 is required for heterochromatin-mediated cohesion at centromeres. Nat. Cell Biol. 5:1111-1116. [PubMed]
6. Bannister, A. J., P. Zegerman, J. F. Partridge, E. A. Miska, J. O. Thomas, R. C. Allshire, and T. Kouzarides. 2001. Selective recognition of methylated lysine 9 on histone H3 by the HP1 chromo domain. Nature 410:120-124. [PubMed]
7. Bernard, P., J. F. Maure, J. F. Partridge, S. Genier, J. P. Javerzat, and R. C. Allshire. 2001. Requirement of heterochromatin for cohesion at centromeres. Science 294:2539-2542. [PubMed]
8. Bird, A. W., D. Y. Yu, M. G. Pray-Grant, Q. Qiu, K. E. Harmon, P. C. Megee, P. A. Grant, M. M. Smith, and M. F. Christman. 2002. Acetylation of histone H4 by Esa1 is required for DNA double-strand break repair. Nature 419:411-415. [PubMed]
9. Birkenbihl, R. P., and S. Subramani. 1992. Cloning and characterization of rad21 an essential gene of Schizosaccharomyces pombe involved in DNA double-strand-break repair. Nucleic Acids Res. 20:6605-6611. [PMC free article] [PubMed]
10. Boeke, J. D., F. LaCroute, and G. R. Fink. 1984. A positive selection for mutants lacking orotidine-5′-phosphate decarboxylase activity in yeast: 5-fluoro-orotic acid resistance. Mol. Gen. Genet. 197:345-346. [PubMed]
11. Boudreault, A. A., D. Cronier, W. Selleck, N. Lacoste, R. T. Utley, S. Allard, J. Savard, W. S. Lane, S. Tan, and J. Cote. 2003. Yeast enhancer of polycomb defines global Esa1-dependent acetylation of chromatin. Genes Dev. 17:1415-1428. [PMC free article] [PubMed]
12. Brehm, A., K. R. Tufteland, R. Aasland, and P. B. Becker. 2004. The many colours of chromodomains. Bioessays 26:133-140. [PubMed]
13. Burke, T. W., J. G. Cook, M. Asano, and J. R. Nevins. 2001. Replication factors MCM2 and ORC1 interact with the histone acetyltransferase HBO1. J. Biol. Chem. 276:15397-15408. [PubMed]
14. Chen, H., M. Tini, and R. M. Evans. 2001. HATs on and beyond chromatin. Curr. Opin. Cell Biol. 13:218-224. [PubMed]
15. Chikashige, Y., and Y. Hiraoka. 2001. Telomere binding of the Rap1 protein is required for meiosis in fission yeast. Curr. Biol. 11:1618-1623. [PubMed]
16. Clarke, A. S., J. E. Lowell, S. J. Jacobson, and L. Pillus. 1999. Esa1p is an essential histone acetyltransferase required for cell cycle progression. Mol. Cell. Biol. 19:2515-2526. [PMC free article] [PubMed]
17. Cooper, J. P., E. R. Nimmo, R. C. Allshire, and T. R. Cech. 1997. Regulation of telomere length and function by a Myb-domain protein in fission yeast. Nature 385:744-747. [PubMed]
18. Cooper, J. P., Y. Watanabe, and P. Nurse. 1998. Fission yeast Taz1 protein is required for meiotic telomere clustering and recombination. Nature 392:828-831. [PubMed]
19. Downs, J. A., S. Allard, O. Jobin-Robitaille, A. Javaheri, A. Auger, N. Bouchard, S. J. Kron, S. P. Jackson, and J. Cote. 2004. Binding of chromatin-modifying activities to phosphorylated histone H2A at DNA damage sites. Mol. Cell 16:979-990. [PubMed]
20. Dziak, R., D. Leishman, M. Radovic, B. K. Tye, and K. Yankulov. 2003. Evidence for a role of MCM (mini-chromosome maintenance)5 in transcriptional repression of sub-telomeric and Ty-proximal genes in Saccharomyces cerevisiae. J. Biol. Chem. 278:27372-27381. [PubMed]
21. Ehrenhofer-Murray, A. E., D. H. Rivier, and J. Rine. 1997. The role of Sas2, an acetyltransferase homologue of Saccharomyces cerevisiae, in silencing and ORC function. Genetics 145:923-934. [PMC free article] [PubMed]
22. Ekwall, K., J. P. Javerzat, A. Lorentz, H. Schmidt, G. Cranston, and R. Allshire. 1995. The chromodomain protein Swi6: a key component at fission yeast centromeres. Science 269:1429-1431. [PubMed]
23. Ekwall, K., E. R. Nimmo, J. P. Javerzat, B. Borgstrom, R. Egel, G. Cranston, and R. Allshire. 1996. Mutations in the fission yeast silencing factors clr4+ and rik1+ disrupt the localisation of the chromo domain protein Swi6p and impair centromere function. J. Cell Sci. 109:2637-2648. [PubMed]
24. Ewen, M. E. 2000. Where the cell cycle and histones meet. Genes Dev. 14:2265-2270. [PubMed]
25. Formosa, T. 2003. Changing the DNA landscape: putting a SPN on chromatin. Curr. Top. Microbiol. Immunol. 274:171-201. [PubMed]
26. Formosa, T., S. Ruone, M. D. Adams, A. E. Olsen, P. Eriksson, Y. Yu, A. R. Rhoades, P. D. Kaufman, and D. J. Stillman. 2002. Defects in SPT16 or POB3 (yFACT) in Saccharomyces cerevisiae cause dependence on the Hir/Hpc pathway: polymerase passage may degrade chromatin structure. Genetics 162:1557-1571. [PMC free article] [PubMed]
27. Forsberg, E. C., and E. H. Bresnick. 2001. Histone acetylation beyond promoters: long-range acetylation patterns in the chromatin world. Bioessays 23:820-830. [PubMed]
28. Forsburg, S. L., and D. A. Sherman. 1997. General purpose tagging vectors for fission yeast. Gene 191:191-195. [PubMed]
29. Freeman-Cook, L., E. B. Gomez, E. J. Spedale, J. Marlett, S. L. Forsburg, L. Pillus, and P. Laurenson. 2004. Conserved locus-specific silencing functions of S. pombe sir2+. Genetics 169:1243-1260. [PMC free article] [PubMed]
30. Fung, A. D., J. Ou, S. Bueler, and G. W. Brown. 2002. A conserved domain of Schizosaccharomyces pombe dfp1(+) is uniquely required for chromosome stability following alkylation damage during S phase. Mol. Cell. Biol. 22:4477-4490. [PMC free article] [PubMed]
31. Gómez, E. B., M. G. Catlett, and S. L. Forsburg. 2002. Different phenotypes in vivo are associated with ATPase motif mutations in Schizosaccharomyces pombe minichromosome maintenance proteins. Genetics 160:1305-1318. [PMC free article] [PubMed]
32. Grant, P. A. 2001. A tale of histone modifications. Genome Biol. 2:1-6. [PMC free article] [PubMed]
33. Grant, P. A., L. Duggan, J. Cote, S. M. Roberts, J. E. Brownell, R. Candau, R. Ohba, T. Owen-Hughes, C. D. Allis, F. Winston, S. L. Berger, and J. L. Workman. 1997. Yeast Gcn5 functions in two multisubunit complexes to acetylate nucleosomal histones: characterization of an Ada complex and the SAGA (Spt/Ada) complex. Genes Dev. 11:1640-1650. [PubMed]
34. Grewal, S. I. 2000. Transcriptional silencing in fission yeast. J. Cell Physiol. 184:311-318. [PubMed]
35. Gutz, H., H. Heslot, U. Leupold, and N. Lopreno. 1974. Schizosaccharomyces pombe. Plenum Press, New York, N.Y.
36. Hirota, K., C. S. Hoffman, T. Shibata, and K. Ohta. 2003. Fission yeast Tup1-like repressors repress chromatin remodeling at the fbp1+ promoter and the ade6-M26 recombination hotspot. Genetics 165:505-515. [PMC free article] [PubMed]
37. Hoffman, C. S., and F. Winston. 1991. Glucose repression of transcription of the Schizosaccharomyces pombe fbp1 gene occurs by a cAMP signaling pathway. Genes Dev. 5:561-571. [PubMed]
38. Howe, L., D. Auston, P. Grant, S. John, R. G. Cook, J. L. Workman, and L. Pillus. 2001. Histone H3 specific acetyltransferases are essential for cell cycle progression. Genes Dev. 15:3144-3154. [PMC free article] [PubMed]
39. Huang, Y. 2002. Transcriptional silencing in Saccharomyces cerevisiae and Schizosaccharomyces pombe. Nucleic Acids Res. 30:1465-1482. [PMC free article] [PubMed]
40. Iizuka, M., and B. Stillman. 1999. Histone acetyltransferase HBO1 interacts with the ORC1 subunit of the human initiator protein. J. Biol. Chem. 274:23027-23034. [PubMed]
41. Jenuwein, T., and C. D. Allis. 2001. Translating the histone code. Science 293:1074-1080. [PubMed]
42. Jin, Y., S. Uzawa, and W. Z. Cande. 2002. Fission yeast mutants affecting telomere clustering and meiosis-specific spindle pole body integrity. Genetics 160:861-876. [PMC free article] [PubMed]
43. John, S., L. Howe, S. T. Tafrov, P. A. Grant, R. Sternglanz, and J. L. Workman. 2000. The something about silencing protein, Sas3, is the catalytic subunit of NuA3, a yTAF(II)30-containing HAT complex that interacts with the Spt16 subunit of the yeast CP (Cdc68/Pob3)-FACT complex. Genes Dev. 14:1196-1208. [PMC free article] [PubMed]
44. Jones, D. O., I. G. Cowell, and P. B. Singh. 2000. Mammalian chromodomain proteins: their role in genome organisation and expression. Bioessays 22:124-137. [PubMed]
45. Kadam, S., and B. M. Emerson. 2002. Mechanisms of chromatin assembly and transcription. Curr. Opin. Cell Biol. 14:262-268. [PubMed]
46. Kearsey, S. E., S. Montgomery, K. Labib, and K. Lindner. 2000. Chromatin binding of the fission yeast replication factor mcm4 occurs during anaphase and requires ORC and cdc18. EMBO J. 19:1681-1690. [PMC free article] [PubMed]
47. Keeney, J. B., and J. D. Boeke. 1994. Efficient targeted integration at leu1-32 and ura4-294 in Schizosaccharomyces pombe. Genetics 136:849-856. [PMC free article] [PubMed]
48. Kelly, T. J., G. S. Martin, S. L. Forsburg, R. J. Stephen, A. Russo, and P. Nurse. 1993. The fission yeast cdc18+ gene product couples S phase to START and mitosis. Cell 74:371-382. [PubMed]
49. Kimura, A., T. Umehara, and M. Horikoshi. 2002. Chromosomal gradient of histone acetylation established by Sas2p and Sir2p functions as a shield against gene silencing. Nat. Genet. 32:370-377. [PubMed]
50. Krude, T. 1995. Chromatin. Nucleosome assembly during DNA replication. Curr. Biol. 5:1232-1234. [PubMed]
51. Kuo, M. H., J. E. Brownell, R. E. Sobel, T. A. Ranalli, R. G. Cook, D. G. Edmondson, S. Y. Roth, and C. D. Allis. 1996. Transcription-linked acetylation by Gcn5p of histones H3 and H4 at specific lysines. Nature 383:269-272. [PubMed]
52. Litt, M. D., M. Simpson, F. Recillas-Targa, M. N. Prioleau, and G. Felsenfeld. 2001. Transitions in histone acetylation reveal boundaries of three separately regulated neighboring loci. EMBO J. 20:2224-2235. [PMC free article] [PubMed]
53. Marmorstein, R. 2001. Structure of histone acetyltransferases. J. Mol. Biol. 311:433-444. [PubMed]
54. Masai, H., T. Miyake, and K. Arai. 1995. hsk1+, a Schizosaccharomyces pombe gene related to Saccharomyces cerevisiae CDC7, is required for chromosomal replication. EMBO J. 14:3094-3104. [PMC free article] [PubMed]
55. Mata, J., R. Lyne, G. Burns, and J. Bahler. 2002. The transcriptional program of meiosis and sporulation in fission yeast. Nat. Genet. 32:143-147. [PubMed]
56. Meijsing, S. H., and A. E. Ehrenhofer-Murray. 2001. The silencing complex SAS-I links histone acetylation to the assembly of repressed chromatin by CAF-I and Asf1 in Saccharomyces cerevisiae. Genes Dev. 15:3169-3182. [PMC free article] [PubMed]
57. Mellone, B. G., L. Ball, N. Suka, M. R. Grunstein, J. F. Partridge, and R. C. Allshire. 2003. Centromere silencing and function in fission yeast is governed by the amino terminus of histone H3. Curr. Biol. 13:1748-1757. [PubMed]
58. Minoda, A., S. Saitoh, K. Takahashi, and T. Toda. 2005. BAF53/Arp4 homolog Alp5 in fission yeast is required for histone H4 acetylation, kinetochore-spindle attachment, and gene silencing at centromere. Mol. Biol. Cell 16:316-327. [PMC free article] [PubMed]
59. Moazed, D. 2001. Common themes in mechanisms of gene silencing. Mol. Cell 8:489-498. [PubMed]
60. Moreno, S., A. Klar, and P. Nurse. 1991. Molecular genetic analysis of the fission yeast Schizosaccharomyces pombe. Methods Enzymol. 194:795-823. [PubMed]
61. Nakayama, J., J. C. Rice, B. D. Strahl, C. D. Allis, and S. I. Grewal. 2001. Role of histone H3 lysine 9 methylation in epigenetic control of heterochromatin assembly. Science 292:110-113. [PubMed]
62. Nimmo, E. R., G. Cranston, and R. C. Allshire. 1994. Telomere-associated chromosome breakage in fission yeast results in variegated expression of adjacent genes. EMBO J. 13:3801-3811. [PMC free article] [PubMed]
63. Nimmo, E. R., A. L. Pidoux, P. E. Perry, and R. C. Allshire. 1998. Defective meiosis in telomere-silencing mutants of Schizosaccharomyces pombe. Nature 392:825-828. [PubMed]
64. Niwa, O., T. Matsumoto, Y. Chikashige, and M. Yanagida. 1989. Characterization of Schizosaccharomyces pombe minichromosome deletion derivatives and a functional allocation of their centromere. EMBO J. 8:3045-3052. [PMC free article] [PubMed]
65. Noma, K., C. D. Allis, and S. I. Grewal. 2001. Transitions in distinct histone H3 methylation patterns at the heterochromatin domain boundaries. Science 293:1150-1155. [PubMed]
66. Nonaka, N., T. Kitajima, S. Yokobayashi, G. Xiao, M. Yamamoto, S. I. Grewal, and Y. Watanabe. 2002. Recruitment of cohesin to heterochromatic regions by Swi6/HP1 in fission yeast. Nat. Cell Biol. 4:89-93. [PubMed]
67. Orphanides, G., W. H. Wu, W. S. Lane, M. Hampsey, and D. Reinberg. 1999. The chromatin-specific transcription elongation factor FACT comprises human SPT16 and SSRP1 proteins. Nature 400:284-288. [PubMed]
68. Osada, S., A. Sutton, N. Muster, C. E. Brown, J. R. Yates III, R. Sternglanz, and J. L. Workman. 2001. The yeast SAS (something about silencing) protein complex contains a MYST-type putative acetyltransferase and functions with chromatin assembly factor ASF1. Genes Dev. 15:3155-3168. [PMC free article] [PubMed]
69. Partridge, J. F., B. Borgstrom, and R. C. Allshire. 2000. Distinct protein interaction domains and protein spreading in a complex centromere. Genes Dev. 14:783-791. [PMC free article] [PubMed]
70. Reifsnyder, C., J. Lowell, A. Clarke, and L. Pillus. 1996. Yeast SAS silencing genes and human genes associated with AML and HIV-1 Tat interactions are homologous with acetyltransferases. Nat. Genet. 14:42-49. [PubMed]
71. Sadaie, M., T. Naito, and F. Ishikawa. 2003. Stable inheritance of telomere chromatin structure and function in the absence of telomeric repeats. Genes Dev. 17:2271-2282. [PMC free article] [PubMed]
72. Shankaranarayana, G. D., M. R. Motamedi, D. Moazed, and S. I. Grewal. 2003. Sir2 regulates histone H3 lysine 9 methylation and heterochromatin assembly in fission yeast. Curr. Biol. 13:1240-1246. [PubMed]
73. Shia, W. J., S. Osada, L. Florens, S. K. Swanson, M. P. Washburn, and J. L. Workman. 2005. Characterization of the yeast trimeric-SAS acetyltransferase complex. J. Biol. Chem. 280:11987-11994 [PubMed]
74. Smith, E. R., A. Eisen, W. Gu, M. Sattah, A. Pannuti, J. Zhou, R. G. Cook, J. C. Lucchesi, and C. D. Allis. 1998. ESA1 is a histone acetyltransferase that is essential for growth in yeast. Proc. Natl. Acad. Sci. USA 95:3561-3565. [PMC free article] [PubMed]
75. Sterner, D. E., and S. L. Berger. 2000. Acetylation of histones and transcription-related factors. Microbiol. Mol. Biol. Rev. 64:435-459. [PMC free article] [PubMed]
76. Strahl, B. D., and C. D. Allis. 2000. The language of covalent histone modifications. Nature 403:41-45. [PubMed]
77. Strahl, B. D., R. Ohba, R. G. Cook, and C. D. Allis. 1999. Methylation of histone H3 at lysine 4 is highly conserved and correlates with transcriptionally active nuclei in Tetrahymena. Proc. Natl. Acad. Sci. USA 96:14967-14972. [PMC free article] [PubMed]
78. Suka, N., K. Luo, and M. Grunstein. 2002. Sir2p and Sas2p opposingly regulate acetylation of yeast histone H4 lysine16 and spreading of heterochromatin. Nat. Genet. 32:378-383. [PubMed]
79. Sutton, A., W. J. Shia, D. Band, P. D. Kaufman, S. Osada, J. L. Workman, and R. Sternglanz. 2003. Sas4 and Sas5 are required for the histone acetyltransferase activity of Sas2 in the SAS complex. J. Biol. Chem. 278:16887-16892. [PubMed]
80. Takahashi, K., H. Yamada, and M. Yanagida. 1994. Fission yeast minichromosome loss mutants mis cause lethal aneuploidy and replication abnormality. Mol. Biol. Cell 5:1145-1158. [PMC free article] [PubMed]
81. Takechi, S., and T. Nakayama. 1999. Sas3 is a histone acetyltransferase and requires a zinc finger motif. Biochem. Biophys. Res. Commun. 266:405-410. [PubMed]
82. Takeda, T., K. Ogino, E. Matsui, M. K. Cho, H. Kumagai, T. Miyake, K. Arai, and H. Masai. 1999. A fission yeast gene, him1(+)/dfp1(+), encoding a regulatory subunit for Hsk1 kinase, plays essential roles in S-phase initiation as well as in S-phase checkpoint control and recovery from DNA damage. Mol. Cell. Biol. 19:5535-5547. [PMC free article] [PubMed]
83. Tanaka, K., T. Yonekawa, Y. Kawasaki, M. Kai, K. Furuya, M. Iwasaki, H. Murakami, M. Yanagida, and H. Okayama. 2000. Fission yeast Eso1p is required for establishing sister chromatid cohesion during S phase. Mol. Cell. Biol. 20:3459-3469. [PMC free article] [PubMed]
84. Tatusova, T. A., and T. L. Madden. 1999. BLAST 2 Sequences, a new tool for comparing protein and nucleotide sequences. FEMS Microbiol. Lett. 174:247-250. [PubMed]
85. Timmermann, S., H. Lehrmann, A. Polesskaya, and A. Harel-Bellan. 2001. Histone acetylation and disease. Cell Mol. Life Sci. 58:728-736. [PubMed]
86. Tuzon, C. T., B. Borgstrom, D. Weilguny, R. Egel, J. P. Cooper, and O. Nielsen. 2004. The fission yeast heterochromatin protein Rik1 is required for telomere clustering during meiosis. J. Cell Biol. 165:759-765. [PMC free article] [PubMed]
87. Ueno, M., T. Murase, T. Kibe, N. Ohashi, K. Tomita, Y. Murakami, M. Uritani, T. Ushimaru, and M. Harata. 2004. Fission yeast Arp6 is required for telomere silencing, but functions independently of Swi6. Nucleic Acids Res. 32:736-741. [PMC free article] [PubMed]
88. van Leeuwen, F., and D. E. Gottschling. 2002. Genome-wide histone modifications: gaining specificity by preventing promiscuity. Curr. Opin. Cell Biol. 14:756-762. [PubMed]
89. Weiss, G., and B. Puschendorf. 1988. The maximum of the histone acetyltransferase activity precedes DNA-synthesis in regenerating rat liver. FEBS Lett. 238:205-210. [PubMed]
90. Wilson, S., N. Warr, D. L. Taylor, and F. Z. Watts. 1999. The role of Schizosaccharomyces pombe Rad32, the Mre11 homologue, and other DNA damage response proteins in non-homologous end joining and telomere length maintenance. Nucleic Acids Res. 27:2655-2661. [PMC free article] [PubMed]
91. Wittmeyer, J., and T. Formosa. 1997. The Saccharomyces cerevisiae DNA polymerase alpha catalytic subunit interacts with Cdc68/Spt16 and with Pob3, a protein similar to an HMG1-like protein. Mol. Cell. Biol. 17:4178-4190. [PMC free article] [PubMed]
92. Wittmeyer, J., L. Joss, and T. Formosa. 1999. Spt16 and Pob3 of Saccharomyces cerevisiae form an essential, abundant heterodimer that is nuclear, chromatin-associated, and copurifies with DNA polymerase alpha. Biochemistry 38:8961-8971. [PubMed]
93. Wood, V., R. Gwilliam, M. A. Rajandream, M. Lyne, R. Lyne, A. Stewart, J. Sgouros, N. Peat, J. Hayles, S. Baker, D. Basham, S. Bowman, K. Brooks, D. Brown, S. Brown, T. Chillingworth, C. Churcher, M. Collins, R. Connor, A. Cronin, P. Davis, T. Feltwell, A. Fraser, S. Gentles, A. Goble, N. Hamlin, D. Harris, J. Hidalgo, G. Hodgson, S. Holroyd, T. Hornsby, S. Howarth, E. J. Huckle, S. Hunt, K. Jagels, K. James, L. Jones, M. Jones, S. Leather, S. McDonald, J. McLean, P. Mooney, S. Moule, K. Mungall, L. Murphy, D. Niblett, C. Odell, K. Oliver, S. O'Neil, D. Pearson, M. A. Quail, E. Rabbinowitsch, K. Rutherford, S. Rutter, D. Saunders, K. Seeger, S. Sharp, J. Skelton, M. Simmonds, R. Squares, S. Squares, K. Stevens, K. Taylor, R. G. Taylor, A. Tivey, S. Walsh, T. Warren, S. Whitehead, J. Woodward, G. Volckaert, R. Aert, J. Robben, B. Grymonprez, I. Weltjens, E. Vanstreels, M. Rieger, M. Schafer, S. Muller-Auer, C. Gabel, M. Fuchs, A. Dusterhoft, C. Fritzc, E. Holzer, D. Moestl, H. Hilbert, K. Borzym, I. Langer, A. Beck, H. Lehrach, R. Reinhardt, T. M. Pohl, P. Eger, W. Zimmermann, H. Wedler, R. Wambutt, B. Purnelle, A. Goffeau, E. Cadieu, S. Dreano, S. Gloux, et al. 2002. The genome sequence of Schizosaccharomyces pombe. Nature 415:871-880. [PubMed]
94. Yamamoto, A., and Y. Hiraoka. 2001. How do meiotic chromosomes meet their homologous partners? Lessons from fission yeast. Bioessays 23:526-533. [PubMed]

Articles from Molecular and Cellular Biology are provided here courtesy of American Society for Microbiology (ASM)
PubReader format: click here to try


Related citations in PubMed

See reviews...See all...

Cited by other articles in PMC

See all...


  • Gene
    Gene links
  • GEO Profiles
    GEO Profiles
    Related GEO records
  • HomoloGene
    HomoloGene links
  • MedGen
    Related information in MedGen
  • Pathways + GO
    Pathways + GO
    Pathways, annotations and biological systems (BioSystems) that cite the current article.
  • Protein
    Published protein sequences
  • PubMed
    PubMed citations for these articles
  • Substance
    PubChem Substance links
  • Taxonomy
    Related taxonomy entry
  • Taxonomy Tree
    Taxonomy Tree

Recent Activity

Your browsing activity is empty.

Activity recording is turned off.

Turn recording back on

See more...