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Department of Pathology and Laboratory Medicine, Lucille P. Markey Cancer Center,1 Graduate Center for Nutritional Sciences, University of Kentucky Medical Center, Lexington, Kentucky 40536,2 Department of Biochemistry and Molecular Biology, Wright State University, Dayton, Ohio 454353
Received 16 October 2001/ Returned for modification 4 December 2001/ Accepted 28 December 2001
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ABSTRACT |
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INTRODUCTION |
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The Escherichia coli MMR pathway is well characterized. Eleven activities are required to carry out MMR in E. coli, including MutS, MutL, MutH, UvrD, ExoI, ExoVII, ExoX, RecJ, single-stranded DNA binding protein (SSB), polymerase III holoenzyme, and DNA ligase (8, 29, 63). These enzymes are necessary and sufficient to perform MMR in vitro. For human cells, less is known about the biochemistry and the components of the repair process, and the reaction is more complex. The human MutS (hMutS) and MutL (hMutL) homologs have been identified by studying mutant cells that demonstrate microsatellite instability and are deficient in MMR. The most commonly studied MMR-deficient cell lines are from patients who have hereditary nonpolyposis colorectal cancer (for reviews see references 7, 21, 22, 28, and 39). Like the E. coli MutS and MutL proteins, hMutS and hMutL are involved in the initiation phase of the repair reaction. However, unlike E. coli MutS and MutL, hMutS and hMutL are heterodimers (reviewed in reference 41). hMSH2 interacts with hMSH6 or hMSH3 to form heterodimeric hMutS
(12, 43) or hMutSß (17, 44), respectively, and hMLH1 interacts with hPMS2, hPMS1, or hMLH3 to form three distinct hMutL heterodimers (16, 31, 33, 35, 50). Recently, DNA polymerase 
(37), proliferating cell nuclear antigen (PCNA) (3, 9, 10, 15, 18, 26, 61), human replication protein A (hRPA) (34), ExoI (2, 51, 54, 58, 59), and replication factor C (67) have been implicated in MMR. However, biochemical evidence for the involvement of many of these activities in human MMR is still lacking. In addition, in comparison with the E. coli pathway, many of the human components, e.g., a human MutH homolog(s) and a helicase(s), have not been identified.
Efforts have been made to identify novel components of MMR by characterizing human tumor cells that display microsatellite instability, but most of these tumor cell lines are defective in known hMSH2 or hMLH1. To identify novel proteins and to determine the involvement of known proteins in human MMR, it is necessary to establish a reconstituted in vitro assay system for human MMR by using fractionated extracts of wild-type cells. Similar approaches have been successful in studies of mammalian DNA replication (reviewed in reference 6), base excision repair (27), and nucleotide excision repair (1, 40). In this study, we have fractionated HeLa cell extracts and identified three essential fractions required for in vitro MMR. These three fractions identify two distinct stages in the human MMR reaction: nick-directed mismatch-provoked excision is the first stage, and repair DNA synthesis is the second stage. Purification of one fraction revealed the active component to be hRPA. hRPA is demonstrated to play multiple roles in the MMR pathway. The other two fractions comprise multiple activities required for MMR and require further fractionation.
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MATERIALS AND METHODS |
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TopAbstractIntroductionMaterials and MethodsResultsDiscussionReferences |
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(i) Ammonium sulfate precipitation. Nuclear extracts prepared from HeLa S3 cells (20) were fractionated by using a two-step ammonium sulfate precipitation procedure. First, the nuclear extract was adjusted to 35% ammonium sulfate (0.21 g/ml) and the precipitate was collected by centrifugation. The supernatant was removed and adjusted to a final concentration of 65% ammonium sulfate by addition of 0.19 g of solid ammonium sulfate/ml. The precipitate was collected by centrifugation, and the supernatant was removed. The precipitates from both treatments were resuspended in and dialyzed against buffer A (25 mM HEPES [pH 7.5], 0.1 mM EDTA, 2 mM dithiothreitol [DTT], 0.1% phenylmethylsulfonyl fluoride [PMSF], 1 µg of leupeptin/ml) containing 0.1 M KCl. Samples were frozen in liquid nitrogen and stored at -80°C. The protein fractions that were insoluble in 35 or 65% ammonium sulfate were designated FI and FII, respectively.
(ii) Preparation of fractions SS1 and SS2. FI was adjusted to a protein concentration of 5 mg/ml by using buffer B (25 mM Tris [pH 7.5], 10% glycerol, 0.01% NP-40, 0.1 mM EDTA, 2 mM DTT, 0.1% PMSF, 1 µg of leupeptin/ml) containing 0.5 M NaCl. The diluted sample was loaded onto a single-stranded DNA (ssDNA)-cellulose column (3 mg of DNA/g of cellulose; Sigma) as described elsewhere (25). The column was washed with buffer B containing 0.5 M NaCl until the flowthrough tested negative for protein by the Bradford assay (4). The bound proteins were eluted from the column with buffer B containing 2.0 M NaCl. The flowthrough and bound fractions, designated SS1 and SS2, respectively, were pooled, concentrated with 35% ammonium sulfate, dialyzed against buffer A containing 0.1 M KCl, and quickly frozen in liquid nitrogen. Samples were stored at -80°C.
(iii) Phosphocellulose chromatography of HeLa nuclear extracts. Phosphocellulose chromatography was performed as described previously (33). Briefly, HeLa nuclear extracts (300 mg) were adjusted to a protein concentration of 5 mg/ml by dilution with buffer A and were applied to a phosphocellulose column (Whatman P-11, 6 cm by 10 cm2) equilibrated with buffer A containing 0.05 M KCl. The column was washed with 200 ml of the equilibration buffer and developed with a 0.8-liter linear gradient from 0.05 to 1.3 M KCl in buffer A at a flow rate of 1/2 column volume per h. Fractions were collected, dialyzed against buffer A containing 0.1 M KCl, and stored in aliquots at -80°C.
(iv) MonoQ chromatography of SS2. Fraction SS2 (5 mg) was applied to a Pharmacia 5/5 MonoQ column equilibrated with buffer A containing 0.1 M KCl and was washed with 10 ml of the same buffer. The column was developed with a KCl gradient from 0.1 to 0.65 M. Fractions were collected and used in MMR assays.
Heteroduplex preparation and MMR assay. DNA heteroduplexes used in this study were 6.4-kb circular molecules (Fig. 1) containing either a G-T mismatch with a strand break 125 bp 5' to the mismatch (5' G-T substrate) or a TG dinucleotide insertion-deletion mispair with a strand break 181 bp 3' to the mispair (3' /TG\ substrate). The G-T substrate was constructed by hybridizing Sau96I-digested f1MR3 double-stranded DNA (dsDNA) with f1MR1 ssDNA as described previously (55). These two phages are identical in DNA sequence except at position 5632, so that a unique G-T mismatch forms when they hybridize to each other. The 3' /TG\ substrate was prepared as described previously (46) by first hybridizing Sau96I-digested f1MR23 dsDNA with f1MR24 ssDNA. The nicked heteroduplex was ligated in the presence of ethidium bromide to introduce supercoiling into the substrate. DNA substrates were purified by CsCl density gradient banding, and the supercoiled substrate was incubated with gpII protein, an endonuclease that specifically cleaves supercoiled filamentous phage DNA at the origin of replication in the viral strand (38). This procedure generates a strand break in the viral strand (V) 181 bp 3' to the heterology (see Fig. 1). A homoduplex (5' A-T) was also constructed as described for the 5' G-T heteroduplex, but using both single-stranded and double-stranded f1MR1 DNAs.
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Southern blot analyses. MMR reactions were carried out as described above or as indicated. Reaction products were linearized with Bsp106, electrophoresed in an alkaline agarose gel (1.5%), and transferred onto a nylon membrane. Membranes were blotted with 32P-labeled oligonucleotide probes (purchased from Gibco) complementary to sequences that flank the Bsp106 restriction site. Oligonucleotides were specific for DNA fragments C1 (5'-ATGGTTTCATTGGTGACGTT-3'), C2 (5'-GATTCTGTCGCTACTGATTAC-3'), V1 (5'-AACGTCACCAATGAAACCAT-3'), or V2 (5'-CAGCACCGTAATCAGTAGCG-3') (see Fig. 1 for details). Blots were exposed to X-ray film, and reaction products were visualized by autoradiography.
Antibodies and Western blot analyses. Antibodies against hMSH2, hMLH1, and PCNA were purchased from Oncogene Sciences (Boston, Mass.), and antibodies against the 70- and 34-kDa subunits of hRPA either were a generous gift from Zhengxiang Pan (Mount Sinai School of Medicine, New York, N.Y.) or were obtained from Santa Cruz Biotechnology, Inc. (Santa Cruz, Calif.). Protein samples were fractionated by sodium dodecyl sulfate-polyacrylamide gel electrophoresis (SDS-PAGE) and transferred to nitrocellulose membranes for Western blot analysis. Membranes were hybridized with antibodies against the 70- and 34-kDa subunits of hRPA. Bound antibody was detected by chemiluminescence using a secondary antibody conjugated with horseradish peroxidase (Amersham).
Expression and purification of recombinant hRPA. The RPA expression vector was kindly provided by Marc Wold, and hRPA was purified as described elsewhere (19). Briefly, 2 liters of culture was induced with isopropyl-ß-D-thiogalactopyranoside (IPTG) when the optical density at 600 nm reached 0.6 to 0.8. After 2 h of incubation at 37°C, the cells were collected and resuspended in buffer HI (30 mM HEPES [pH 7.8], 0.01% NP-40, 0.25 mM EDTA, 1 mM DTT, and 0.25% inositol) containing the protease inhibitors PMSF, pepstatin A, and leupeptin as described elsewhere (47, 48). The resulting supernatant was loaded onto a 20-ml blue-Sepharose column equilibrated in HI buffer containing 0.1 M KCl. After a wash with the same buffer, the column was sequentially washed with HI buffer containing 0.8 M KCl and 0.5 M NaSCN. The hRPA protein was eluted with HI buffer containing 1.5 M NaSCN. Fractions containing hRPA were further purified using a 5-ml hydroxylapatite column and a 2-ml Q-Sepharose column as described previously (47, 48). hRPA was identified by its DNA binding activity to the 5'-[32P]dT30 DNA substrate under conditions of DNA excess. This was accomplished by the addition of unlabeled dT30 DNA and enabled accurate determination of activity and exclusion of contaminating activities. This procedure resulted in >95% protein purity. hRPA was dialyzed in HI buffer and stored at -80°C.
DNA ligase and DNA polymerase assay. DNA ligase activity in FII was determined by its ability to convert a nicked circular substrate into supercoiled DNA. The 5' G-T substrate was incubated with 30 µg of FII at 20°C for 2 h in the presence of ethidium bromide (0.29 nM/µg of DNA), 30 mM Tris-HCl (pH 8.0), 4 mM MgCl2, 1 mM DTT, 26 µM NAD+, and 50 µg of bovine serum albumin/ml. As a positive control, the nicked DNA substrate was also incubated with E. coli DNA ligase (New England Biolabs) at a final concentration of 4 U/µg of DNA. DNA samples were recovered, fractionated in a 1% agarose gel, and visualized under UV illumination. DNA-dependent DNA polymerase activity was determined by measuring the incorporation of [32P]TMP using a poly(dA)/oligo(dT)16 substrate. Reactions were performed in 20 µl at 37°C as previously described (56). Reactions were terminated by addition of EDTA to a final concentration of 20 mM, and unincorporated nucleotides were removed by Sephadex G-50 spin column chromatography. Products were separated by electrophoresis on 8% polyacrylamide-7 M urea DNA sequencing gels. Products were detected by autoradiography.
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RESULTS |
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hRPA substitutes for SS2. Fractions SS1, SS2, and FII are complex protein samples, and one or more components in each fraction could be required for the MMR reaction. To determine if any of these fractions contains a single MMR activity, in vitro reconstitution was performed by supplementing a combination of two fractions with individual factors derived from HeLa nuclear extracts that were chromatographed as discrete species on a P-11 phosphocellulose column (see Materials and Methods for details). No phosphocellulose column fraction could substitute for SS1 or FII (data not shown), but the requirement for SS2 was eliminated by a broad range of phosphocellulose fractions, with peak fractions at 21 to 33 (Fig. 3A). This result was confirmed by fractionating SS2 by fast- performance liquid chromatography on a MonoQ column and assaying the fractions for the ability to restore MMR proficiency to SS1-FII. The SS1-FII-complementing activity was detected in a high-salt fraction of the MonoQ column (data not shown). These complementation experiments strongly suggest that SS2 contains a single activity that is required in order to reconstitute MMR in vitro.
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SS1 nicks ssDNA. A novel 3.2-kb species was observed in reactions with fraction SS1, but the level of this species was dramatically reduced when SS2 was added to the reaction mixtures (Fig. 2B, lane 5). The identity of this species is unknown; however, the size of the fragment generated suggests that the plasmid (6.4 kb) is digested into two DNA fragments of equal size, 3.2 kb each. As all reaction products were digested with Bsp106 prior to electrophoresis, a double strand break must be generated 180° from the Bsp106 site. This position corresponds with the Sau96I site that was used to generate the nick in the complementary strand; therefore, to generate a double strand break, SSI must nick the viral strand at a position close to the nick on the complementary strand.
If this is the case, digestion of the 6.4-kb G-T circular DNA substrate with Bsp106 or BseRI will produce two fragments; otherwise, a single species will be observed. The 5' G-T substrate was incubated with SS1 and digested with the restriction enzyme Bsp106. The product of this reaction was a 
3.2-kb DNA fragment (Fig. 4A, lane 2), with an electrophoretic mobility identical to that of the product of Bsp106-HindIII double digestion of the MMR reaction product (Fig. 2B). In contrast, digestion with BseRI created a 3.7- and a 2.7-kb fragment (Fig. 4A, lane 4). These results suggest that a strand break is made on the viral strand at or near the Sau96I site when the DNA substrate is incubated in the presence of SS1.
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Fraction SS1 carries out nick-directed and mismatch-dependent excision. A possible mechanism to create the nick of the viral strand is excision of the complementary strand to generate a nuclease-susceptible ssDNA region around the preexisting strand break. The excision activity must also then be present in SS1. To test this hypothesis, we performed experiments to determine if excision occurs in the SS1 reaction. In HeLa nuclear extracts, MMR excision intermediates contain a single-stranded region spanning the shorter patch between the nick and the mismatch in a circular substrate. The extent of the ssDNA region can be mapped relative to a restriction endonuclease cleavage site by Southern blot analysis (14, 18). Figure 5 shows such an analysis with the 5' G-T substrate. As expected, hybridization with the complementary fragment C1 (from the Bsp106 site to the mismatch to the strand break [Fig. 1]) placed the untreated substrates at the Sau96I site (Fig. 5, lane 3, 3.2 kb). After incubation with HeLa nuclear extracts in the presence of aphidicolin, a group of smeared molecules approximately 200 bp shorter than the untreated substrate were detected (Fig. 5; compare lanes 1 and 3). These molecules are excision intermediates that accumulate when DNA synthesis is blocked (14, 18). When the DNA substrate was incubated with SS1, similar reaction products were observed (Fig. 5, lane 2), suggesting that SS1 can carry out excision along the short path between the strand break and the mismatch, thereby leading to a ssDNA region in the viral strand. Southern hybridization was also carried out on the same blot with complementary fragment C2 (from Bsp106 to BseRI to the strand break [Fig. 1]). There was no evidence of excision in this region of the substrate, which is the longer path from the nick to the mismatch (Fig. 5, lanes 4, 5, and 6). These results suggest that SS1 may be capable of nick-directed mismatch-provoked excision.
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hRPA protects the template strand from incision by nucleases. While the excision reaction is required for MMR, the viral strand nicking activity is detrimental to the process, and it is likely that one component of the MMR pathway inhibits this reaction. As mentioned above, addition of SS2 to SS1 blocks the production of the 3.2-kb DNA fragment by SS1, suggesting that SS2 may possess this inhibition function. We therefore assessed hRPA for the ability to prevent SS1 from nicking DNA substrates. As shown in Fig. 6A, the amount of nicked viral strand decreased as the concentration of hRPA increased. One microgram of hRPA is sufficient to prevent SS1 (30 µg) from making strand breaks in the ssDNA region during the MMR reaction (Fig. 6A, lane 4). Interestingly, E. coli SSB binds ssDNA and is functionally similar to hRPA, but SSB does not substitute for hRPA in the reaction with human MMR proteins: as much as 8 µg of SSB failed to protect the continuous strand of the substrate from nicking in the presence of SS1 (Fig. 6A, lane 8). These results suggest that hRPA interacts specifically with human MMR proteins.
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FII carries out gap filling and ligation. The above results indicate that SS1 carries out mismatch-provoked excision on the nick-containing DNA strand of heteroduplex DNA and that fraction SS2 (or hRPA) protects the template DNA strand from degradation. When the MMR reaction is carried out in the presence of SS1 and SS2 and in the absence of FII, the reaction is blocked at the DNA synthesis step (Fig. 4). Therefore, it seems possible that FII might perform gap-filling DNA synthesis and/or DNA ligation. To test this hypothesis, repair intermediates were characterized in reactions with or without FII. As shown in Fig. 7A, the nicked complementary strand was a 6.4-kb species in reactions containing FII (lane 3), SS1-FII (lane 4), hRPA-FII (lane 6), and SS1-hRPA-FII (lane 7). However, reaction products in all reactions, except in that containing SS1, hRPA, and FII, still contained a mismatch, indicating that repair had not occurred (see Fig. 2B). Therefore, the 6.4-kb species is likely to result from sealing of the strand break by a DNA ligase in FII. This is consistent with the observation that SS1 is very active in repair excision (Fig. 5, lane 2, and Fig. 7A, lane 2), but FII inhibits this excision activity (Fig. 7A, lane 4), possibly because it removes the DNA substrate by ligating strand breaks that are required for in vitro MMR (20, 57). These results strongly suggest that fraction FII contains a ligase activity required for in vitro MMR. Our ligase activity assay confirmed that this was indeed the case. Like E. coli DNA ligase, FII could convert a nicked circular DNA substrate into a supercoiled molecule in the presence of ethidium bromide (Fig. 7B).
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-32P]TTP substrate. Increasing concentrations of FII were incubated with the DNA substrate, and incorporation of [-32P]TMP into high-molecular-weight products was determined. Reaction products were separated by denaturing PAGE and detected by autoradiography. Results are presented in Fig. 7C; the products observed were 50 to 100 bases in length and increased in intensity with increasing concentrations of FII. These results demonstrate that FII contains a DNA-dependent DNA polymerase activity. Preincubation of FII with the DNA polymerase -specific inhibitory monoclonal antibody (Fig. 7C, lanes 4 to 6) SJK 132-20 revealed minimal inhibition, suggesting that the polymerase responsible for the extension observed is either DNA polymerase or DNA polymerase 
. However, it should be noted that the conditions employed for the assay were optimized for DNA polymerase (56) and that the FII fraction also likely contains DNA polymerase . The gap-filling activity of FII is dependent on hRPA. It is not clear whether the gap-filling step of the in vitro MMR reaction is carried out by FII alone or by FII with another component(s) in SS1 and/or SS2 (hRPA). Previous studies indicate that ssDNA binding activity is essential for DNA repair synthesis during mammalian nucleotide excision repair (53). Thus, it seems possible that FII-mediated gap filling requires hRPA. To address this issue, the excision and repair synthesis steps of the human MMR reaction were carried out sequentially. The 5' G-T substrate was incubated with SS1-hRPA, and the repair intermediates from this reaction were purified and used as a substrate for a gap-filling reaction in the presence or absence of FII and SS1 or hRPA. The reaction products were analyzed by Southern blotting. As shown in Fig. 7D, reactions containing FII alone (lane 2) or FII with SS1 (lane 5) had about the same amount of full-length dsDNA (6.4 kb) as the control reaction (lane 1), suggesting that gapped intermediates recovered from the SS1-hRPA reaction are not converted into full-length dsDNA in these reactions. However, when the reaction was carried out in the presence of FII and hRPA (lane 3), more than 30% of the gapped intermediates were converted to full-length molecules, indicating that gap filling and ligation had occurred. In the presence of aphidicolin, no full-length ligated products were formed (Fig. 7D, lane 4), suggesting that DNA synthesis is required to form this product. Interestingly, when E. coli SSB was substituted for hRPA in the gap-filling reaction, approximately 30% of the gapped substrates were converted to the 6.4-kb product in the presence of FII and E. coli SSB (data not shown). This result suggests that hRPA may bind and protect the ssDNA region during repair synthesis associated with MMR. To determine if the removal of the mispaired base is associated with hRPA-FII-mediated gap filling, DNA products were subjected to digestion by restriction enzymes HindIII (scoring enzyme) and Bsp106 (see Fig. 1 for assay details). As shown in Fig. 7D, the expected repair products (3.1- and 3.3-kb fragments) were observed in reactions containing FII and hRPA (lane 8), but minimal levels (if any) were observed in reactions containing FII only (lane 7). It was noted that the repair rate (16%) in the partial reaction (gapped substrate, FII, and hRPA) was lower than that (39%) in a normal reaction (nicked substrate, SS1, SS2, and FII [see Fig. 2B, lane 8]). On the other hand, a similar lower rate (22%) was also observed when whole HeLa cell nuclear extracts were tested for processing of the gapped DNA substrate (data not shown) (compare the repair rate of 22% in this gap-filling reaction with that of 72% in a normal reaction [Fig. 2B, lane 1]). Therefore, the DNA substrate used in the gap-filling reaction seems to be a limiting factor. Nevertheless, these observations clearly indicate that the hRPA-dependent gap filling by FII employed the continuous strand as a template for repair resynthesis and that the mispaired base in the nicked strand was removed during the process.
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DISCUSSION |
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TopAbstractIntroductionMaterials and MethodsResultsDiscussionReferences |
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SS1 is capable of initiating strand-specific MMR in a manner dependent on a mismatch and a strand break, as evidenced by the fact that the repair excision intermediates generated by SS1 are almost identical to those produced in HeLa nuclear extracts containing aphidicolin (Fig. 6A, lanes 1 and 2). In addition, SS1-mediated excision was not detected when a homoduplex was used in the reaction (Fig. 5, lanes 7 and 9). Previous studies have shown that defects in human MutS and MutL homologs and PCNA abolish mismatch-provoked excision (9, 18, 23, 46, 61). In E. coli, a helicase and at least four exonucleases are involved in MMR-associated excision (8, 29, 63), and human MMR may be mechanistically similar. Therefore, it is conceivable that SS1 from HeLa cells includes hMutS, hMutL, PCNA, helicase, and nuclease activities. Western blot analysis indeed revealed that MSH2, MLH1, and PCNA are present in significant amounts in SS1. Although a helicase(s) and an exonucleases(s) that participate in human MMR have not yet been identified or characterized, ExoI, which possesses a 5'-to-3' exonuclease activity, has been implicated in MMR (2, 51, 54, 58, 59). It may be possible to purify an MMR-associated helicase(s) and exonucleases, including ExoI if it is required for MMR, by additional fractionation of SS1. Biochemical analyses of these protein fractions will improve understanding of the mechanism of MMR in human cells.
Although SS1 carries out nick-directed mismatch-provoked excision along the shorter path between the strand break and the mismatch with the 5' G-T substrate, SS1 does not carry out this reaction with the 3' /TG\ substrate (data not shown). This is presumably because SS1 cannot carry out excision in the 3'-to-5' direction from the nick to the mismatch. Previous studies indicate that HeLa cells possess a bidirectional mechanism to remove a mismatch (14). Depending on the location of a strand break relative to the mismatch, MMR-associated excision occurs in a 5'-to-3' or a 3'-to-5' direction. Because MMR reconstituted in vitro in the presence of SS1-hRPA-FII corrects the 3'/TG substrate in a strand-specific manner (data not shown), it is likely that 3'-to-5' excision activity is present in SS2 and/or FII. Further studies are required in order to determine which of these two fractions contains 3'-to-5' excision activity.
The second stage of human MMR in this reconstituted assay system is DNA repair synthesis. During this stage of the reaction, SS2 and FII convert gapped intermediates into closed dsDNA molecules. We have shown that hRPA can substitute for SS2. The components of FII that play a role in MMR are not yet clear, but they apparently include DNA polymerase and ligase activities required for MMR. FII does not carry out strand-specific MMR (Fig. 2), but it does generate a 6.4-kb full-length product that is resistant to restriction enzyme cleavage. This product is probably generated by a very active ligase in FII that ligates the nick in the DNA substrate. This possibility is consistent with the fact that FII inhibits SS1-mediated nick-directed excision on heteroduplex DNA, presumably by ligating the nick before excision takes place. Indeed, our in vitro ligase assay shows that FII is capable of sealing single-stranded breaks and converting a nicked circular DNA substrate into supercoiled DNA (Fig. 7B). We also show that FII contains a DNA polymerase activity. For example, FII and hRPA convert gapped MMR reaction intermediates generated by SS1-hRPA into full-length dsDNA molecules (Fig. 7D) (see discussion below), and this conversion is inhibited by aphidicolin, indicating involvement of DNA polymerase , , or in the gap-filling reaction. DNA polymerase activity is indeed identified in FII by using a traditional in vitro DNA replication assay system (Fig. 7C). Even though our data cannot rule out the involvement of polymerase in MMR, the gap-filling activity detected in FII is not conducted by polymerase , as evidenced by the fact that an antibody specific for DNA polymerase has essentially no effect on the DNA polymerization reaction in FII (Fig. 7C). Thus, it is highly likely that DNA polymerase (37) and/or is responsible for the gap-filling activity in FII. Western blot analyses revealed that FII also contains abundant MSH2, MLH1, and PCNA. However, unlike SS1, FII is unable to conduct repair excision, suggesting that components required for excision, e.g., exonucleases, are not present in FII.
Role of hRPA in MMR. hRPA is a human ssDNA binding protein that is essential for cellular DNA metabolism (62) involving ssDNA intermediates including DNA replication (13, 64, 65), homologous recombination (36), base excision repair (45), and nucleotide excision repair (11). Recently, Lin et al. have demonstrated that incubation of an anti-hRPA antibody with HeLa extracts inhibits strand-specific MMR in vitro, suggesting that hRPA is also involved in MMR (34). However, the actual role of hRPA in MMR is not known. Using an in vitro reconstitution system, we demonstrate here that recombinant hRPA can substitute for one of the required HeLa nuclear fractions in MMR. Analysis of critical intermediates reveals that hRPA plays multiple roles in human MMR in vitro.
First, hRPA protects single-stranded regions of the template DNA strand from nuclease degradation. While SS1 is capable of mismatch-provoked excision in the nicked strand, it also makes a single-stranded break in the continuous strand that serves as a template for repair synthesis. Since such a strand break in the template strand has never been observed in the whole-cell nuclear extract, a DNA binding activity required for MMR must be responsible for protecting the single-stranded region in the template strand. We found that this activity is hRPA, as evidenced by the fact that addition of hRPA to the SS1 reaction mixture blocks the single-stranded nicking in the continuous DNA strand, suggesting that hRPA may bind to the single-stranded region, protecting it from attack by nucleases and ensuring that the template DNA strand is suitable for repair DNA synthesis.
Second, hRPA may also directly contribute to mismatch-provoked excision, because hRPA enhances repair excision by SS1 (Fig. 6B). How might hRPA participate in repair excision? It is known that in E. coli, MMR-associated excision requires DNA helicase II to unwind the DNA helix (29), and a similar activity should also be required for the human reaction. Possibly, hRPA facilitates DNA unwinding by a DNA helicase activity that participates in MMR. Recently, it was shown that yeast RPA stimulates MER3 helicase during meiotic crossing over (42). hRPA plays a similar role in simian virus 40 (SV40) DNA replication, during which hRPA and T antigen interact physically and unwind the SV40 origin of replication (5, 24, 66). A DNA helicase activity that is stimulated by hRPA has been purified from human cells (52), and it is possible that this helicase could play a role in human MMR.
Finally, hRPA plays a crucial role in repair DNA synthesis during human MMR. FII is required to convert gapped intermediates into complete circular DNA, and this conversion also requires hRPA (Fig. 7D). However, the mechanism by which hRPA stimulates repair synthesis during human MMR is not exactly clear. Previous studies have demonstrated that hRPA stimulates the activity of DNA polymerases , , and (24, 25, 30, 60), all of which are sensitive to aphidicolin and may participate in MMR-associated DNA repair synthesis. In fact, evidence suggests that DNA polymerase is involved in human MMR (37). Therefore, it is possible that hRPA may stimulate repair synthesis during MMR in addition to protecting the DNA template from degradation by nucleases. Recently, Ranalli et al. (49) have demonstrated that hRPA stimulates a ligase activity of DNA ligase I, which is probably required for MMR.
In summary, we have established an in vitro system that enables one to dissect the complex human MMR reaction into multiple stages. Analysis of individual stages of the reaction has revealed crucial repair intermediates, which help to identify the requirement for hRPA in MMR and define the roles of hRPA in the pathway. We believe that further analysis of the three fractions described here, especially fractions SS1 and FII, will identify additional components required for human MMR and will eventually elucidate the molecular mechanisms of the human pathway.
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ACKNOWLEDGMENTS |
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This work was supported in part by grants CA82604 and CA85377 (to G.-M.L.) and CA82741 (to J.J.T.) from the National Cancer Institute.
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FOOTNOTES |
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