Correspondence: Piotr Jonczyk, Institute of Biochemistry and Biophysics, Polish Academy of Sciences, Pawinskiego 5A, 02-106 Warsaw, Poland. Tel.: +48 22 592 1113; fax: +48 22 592 2190; e-mail: email@example.com
High accuracy (fidelity) of DNA replication is important for cells to preserve the genetic identity and to prevent the accumulation of deleterious mutations. The error rate during DNA replication is as low as 10−9 to 10−11 errors per base pair. How this low level is achieved is an issue of major interest. This review is concerned with the mechanisms underlying the fidelity of the chromosomal replication in the model system Escherichia coli by DNA polymerase III holoenzyme, with further emphasis on participation of the other, accessory DNA polymerases, of which E. coli contains four (Pols I, II, IV, and V). Detailed genetic analysis of mutation rates revealed that (1) Pol II has an important role as a back-up proofreader for Pol III, (2) Pols IV and V do not normally contribute significantly to replication fidelity, but can readily do so under conditions of elevated expression, (3) participation of Pols IV and V, in contrast to that of Pol II, is specific to the lagging strand, and (4) Pol I also makes a lagging-strand-specific fidelity contribution, limited, however, to the faithful filling of the Okazaki fragment gaps. The fidelity role of the Pol III τ subunit is also reviewed.
The mechanisms by which organisms are able to efficiently and faithfully replicate their DNA are of critical importance in genetics, biology, and medical science, and research into these mechanisms has received significant attention. Overall, DNA replication is a high-accuracy process that enables cells and organisms to maintain their genetic identity. On the other hand, the replication process is not without error and mutations will occur with defined frequencies. While mutations are essential factors in mediating long-term processes of adaptation and evolution or in generating antibody diversity, in the short run mutations are generally deleterious and may be a cause of human disease, like birth defects or cancer (Loeb, 1991; Jackson & Loeb, 1998; Preston et al., 2010; Tuppen et al., 2010). Studies of spontaneous mutation rates in various systems have provided a baseline value for the in vivo replication error rate. When expressed per base pair (per round of replication), the rates can be 5 × 10−10 for bacterial systems (Escherichia coli) or 5 × 10−11 for mammalian systems (Drake, 1991; Drake et al., 1998). It is clear that such low error rates must be the outcome of multiple fidelity pathways acting in parallel and/or consecutively.
In broad outline, high fidelity must be based on two major components. First, the DNA must be kept intact and, to the extent possible, free of any damage before DNA replication is to proceed. Obviously, damaged DNA is unlikely to be copied accurately. The multitude of DNA surveying and repair systems used by cells to monitor their DNA attest to the critical importance of this issue (Friedberg et al., 2006). Second, the intrinsic accuracy of DNA replication, when performed on essentially damage-free DNA, has its limits. Therefore, unavoidably, DNA polymerases will commit errors, leading to mutations. The present review focuses on this particular aspect of DNA replication fidelity and will cover insights obtained regarding this process from the model system E. coli. The data used are derived from mutation frequencies in actively growing E. coli cultures under aerobic conditions in the absence of external stresses. Nevertheless, spontaneous DNA damage (e.g. hydrolytic DNA damage leading to deaminated bases or abasic sites) does occur under these conditions, which, if unrepaired, may contribute to observed mutations. Thus, an absolute distinction between the two types of mutation production may not be possible. In our studies, we have minimized the possible contribution of spontaneous DNA damage by performing most experiments in DNA mismatch-repair-defective strains, in which uncorrected replication errors are assumed to predominate (see below).
As a general outline, we present in Fig. 1 a cartoon showing how in most organisms the overall accuracy of DNA replication can be considered as the outcome of three (highly conserved) components acting sequentially: (1) selection of the correct DNA nucleotide by the replicative DNA polymerase, (2) removal of any misinserted nucleotides by the 3′→5′ exonuclease proofreading activity associated with the polymerase, and (3) postreplicative correction of polymerase errors that have escaped proofreading by the DNA mismatch repair system (MMR) (Schaaper, 1993a; Kunkel & Bebenek, 2000; Kunkel, 2004; Kunkel & Bebenek, 2004). In E. coli, the mismatch repair step is performed by the mutHLS system, which is capable of distinguishing the (incorrect) newly synthesized strand from the (correct) parental strand based on the transient undermethylation (at 5′-GATC-3′ sequences) of the newly made strand (reviewed in Modrich, 1987; Kunkel & Erie, 2005). Roughly, the contribution of each of these components to the error rate can be estimated at 10−5 (insertion), 10−2 (proofreading), and 10−3 (mismatch repair), accounting for the 10−10 overall rate, although each contribution is highly dependent on the precise type of error under question (Schaaper, 1993a; Kunkel & Bebenek, 2000; Kunkel, 2004).
Chromosomes are replicated generally by large, multisubunit, dimeric complexes – termed replicases, which are capable of copying the two strands, leading and lagging, at a replication fork in a coordinated fashion. In E. coli, the replicase is DNA polymerase III holoenzyme (Pol III HE), a dimeric enzyme that contains two copies of DNA polymerase III, one for each strand. A schematic depiction of HE containing its various associated subunits at a replication fork (replisome) is shown in Fig. 2. Replicases and their functioning at the replication fork are subjects of intense current interest (e.g. McHenry, 2011).
Specific questions regarding the functioning and fidelity of chromosomal replisomes center around: (1) what is the precise composition of the complex, (2) which DNA polymerase copies which strand, (3) is there differential fidelity between leading and lagging strands, (4) what is the contribution to fidelity of the noncatalytic subunits within the replicase, and (5) what is the fidelity contribution, if any, of the additional DNA polymerases that cells possess? The present review will focus, in part, on the latter aspect, namely the possible role of the additional polymerases, often referred to as ‘polymerase switching’.
Multiple DNA polymerases in the cell
Escherichia coli encodes five distinct DNA polymerases: Pol I, Pol II, Pol III, Pol IV, and Pol V. These polymerases, along with some of their relevant properties, are listed in Fig. 3. The presence of multiple DNA polymerases in the cell is a general phenomenon: for example, the yeast Saccharomyces cerevisiae has eight, while human cells possess at least 16 DNA-template-dependent DNA polymerases (Friedberg et al., 2006; Shcherbakova & Fijalkowska, 2006; Kunkel, 2009). Some of these, functioning usually as replicative DNA polymerases, are high-fidelity enzymes possessing a 3′→5′ exonuclease proofreading activity. But other polymerases are error-prone enzymes, lacking a proofreading activity and having an adjusted (or enlarged) active site permitting higher frequencies of base misinsertions (reviewed in Friedberg et al., 2002; Goodman, 2002; Nohmi, 2006; Shcherbakova & Fijalkowska, 2006; Jarosz et al., 2007; Lehmann et al., 2007; McCulloch & Kunkel, 2008). Most of the error-prone polymerases, referred to as translesion synthesis polymerases (TLS polymerases), may have evolved to bypass replication-blocking template lesions. TLS allows strand extension when the replicative DNA polymerase is stalled at a DNA lesion, a subject that has been extensively covered (reviewed in Friedberg et al., 2002; Goodman, 2002; Nohmi, 2006; Shcherbakova & Fijalkowska, 2006; Jarosz et al., 2007; Fuchs & Fujii, 2007; Lehmann et al., 2007; Guo et al., 2009; Takata & Wood, 2009; Sutton, 2010; Andersson et al., 2010; Livneh et al., 2010; Ho & Scharer, 2010).
In addition to lesion bypass performed by specialized TLS polymerases, evidence has accumulated, from both in vitro and in vivo experiments, that the replicase is a dynamic entity, in which DNA polymerase exchanges can occur, thus providing access of accessory polymerases to the replication fork also during the synthesis of undamaged DNA (Banach-Orlowska et al., 2005; Furukohri et al., 2008; Gawel et al., 2008; Uchida et al., 2008; Curti et al., 2009; Heltzel et al., 2009a; Makiela-Dzbenska et al., 2009). These observations raise important fidelity questions. In some cases, this participation of accessory polymerases may lead to improved fidelity, when the accessory DNA polymerase is accurate (e.g. a proofreading-proficient polymerase), while in other cases this may lead to lower fidelity when the polymerase is error-prone.
In this review, we will summarize the results from work conducted in the bacterium E. coli, showing that during normal DNA replication, both replicative and accessory DNA polymerases contribute to the overall fidelity of DNA replication. Furthermore, we will describe studies suggesting that certain noncatalytic subunits of HE, like the τ subunit, have a role in controlling the access of these polymerases to the fork, affecting, in this manner, the fidelity of replication. We will first discuss the major replicase, DNA Pol III HE, then accessory polymerases II, IV, and V, which may have occasional access to the replication fork, and finally Pol I, whose fidelity role may be limited to the processing of Okazaki fragments.
DNA Pol III HE
The major replicative DNA polymerase in E. coli cells is DNA Pol III HE that can synthesize DNA with high processivity (over 50 kb per binding event) (Yao et al., 2009) and with high speed (up to 1000 nucleotides per second). As shown in Fig. 2, Pol III HE in E. coli is an asymmetric, dimeric enzyme and can perform coupled, high-speed replication of the two, leading and lagging, DNA strands at the replication fork (for reviews, see: McHenry, 2003; O'Donnell, 2006; Pomerantz & O'Donnell, 2007; Yao & O'Donnell, 2008; Langston et al., 2009; McHenry, 2011). Pol III HE is a complex of 17 subunits (10 distinct proteins) with an overall composition (αεθ)2(β2)2τ2γδδ′χψ. It contains two Pol III core subassemblies, one for each strand, each consisting of three tightly bound subunits: α (dnaE gene product, the DNA polymerase), ε (dnaQ gene product, the 3′→5′ proofreading exonuclease), and θ (holE gene product, stabilizer for ε subunit) (Gefter et al., 1971; Takano et al., 1986; Taft-Benz & Schaaper, 2004). Each core is tethered to the DNA by a ring-shaped sliding-clamp processivity factor (β2 homodimer) (Kong et al., 1992). Additionally, Pol III HE contains the seven-subunit (τ2γδδ′χψ) DnaX complex (Pritchard et al., 2000). This complex contains the τ2 dimer, which connects the two Pol III α subunits, creating the dimeric polymerase unit capable of coupled synthesis of leading and lagging strands. The DnaX complex is also responsible, because of the activity of the δ and δ′ subunits, for the loading and unloading of the β2 sliding-clamp (Jeruzalmi et al., 2001). This important activity is especially critical for the lagging-strand polymerase, which needs to cycle on and off during Okazaki fragment synthesis (McHenry, 2011).
The form of Pol III HE depicted here, with the DnaX complex containing two τ subunits and one γ subunit, is the form of HE historically found when isolated from cells (McHenry, 2011). More recently, a form of Pol III has been described, upon reconstitution of HE in vitro, in which the DnaX complex contains three τ subunits and no γ subunit (τ3δδ′χψ) leading to incorporation of three pol III core units (McInerney et al., 2007; Reyes-Lamothe et al., 2010; Georgescu et al., 2012). As τ and γ are products of the same (dnaX) gene and are identical for the first 430 amino acids, they share several functions and can partially substitute for each other (Flower & McHenry, 1986; Blinkowa & Walker, 1990; McHenry, 2011). However, τ as the longer, full-length dnaX gene product (643 residues) has additional capabilities not present in γ, including its interaction with the α subunit, which is responsible for the dimerization of the polymerase. The alternative τ3δδ′χψ DnaX complex is, however, capable of binding three pol III cores, and this trimeric form of HE has been demonstrated to operate efficiently in vitro (McInerney et al., 2007; Reyes-Lamothe et al., 2010; Georgescu et al., 2012). While a trimeric form of HE may have certain advantages over the dimeric form (Georgescu et al., 2012), including possibly its fidelity, the significance of the trimeric form for HE operating in vivo remains to be established (McHenry, 2011).
The fidelity properties of Pol III have been investigated in vivo and in vitro. The in vivo experiments have suggested that indeed HE is highly accurate, as expected for the major replicating enzyme (Schaaper, 1993a). The importance of Pol III for controlling the mutation rate is also evidenced by the properties of several E. coli mutator mutants (which have enhanced mutation rates) carrying a defect in the dnaE gene encoding the Pol III α subunit (Sevastopoulos & Glaser, 1977; Fijalkowska et al., 1993; Oller et al., 1993; Vandewiele et al., 2002). Strong mutators have also been found residing in the dnaQ gene, encoding the ε proofreading subunit (Fijalkowska & Schaaper, 1996; Taft-Benz & Schaaper, 1998), establishing the importance of the proofreading process for the chromosomal replication process. A modest mutator effect was also detected for strain lacking the holE gene, encoding the θ subunit (Taft-Benz & Schaaper, 2004). This mutator effect likely reflects the stabilizing role that θ subunit plays for ε subunit (the three subunits are arranged in the linear order α-ε-θ) (Taft-Benz & Schaaper, 2004; Chikova & Schaaper, 2005).
While the studies on E. coli mutator mutants described above bear evidence to the important role that (wild-type) Pol III HE plays in preventing replication errors, they do not necessarily prove that errors made by the wild-type enzyme contribute to the observed replication error rate or bacterial mutation rate. That this is indeed the case was evidenced by the isolation of a series of dnaE antimutator mutants (Fijalkowska & Schaaper, 1993; Fijalkowska et al., 1993; Oller & Schaaper, 1994; Schaaper, 1993, 1996, 1998). In these strains, replication has become more accurate because of the altered α subunit of HE, resulting in a detectably lower mutation rate. The mechanism underlying the antimutator effects could be enhanced fidelity at the insertion step or, more likely, an effect on the interplay between polymerase and associated proofreading exonuclease. Following a nucleotide misinsertion, competition arises between (1) the forward polymerization rate, extending the mismatch and hence fixing the error as a potential mutation, and (2) the reverse reaction by the movement of the incorrect base from the polymerase active site to the exonuclease site leading to the removal of the base (proofreading). Obviously, impairment in the polymerase forward rate will lead to a different partitioning between the two reactions, leading to enhanced proofreading and a reduction in the error rate. This enhanced-proofreading mechanism for antimutators was first demonstrated in studies with the bacteriophage T4 DNA polymerase (Drake & Allen, 1968; Gillin & Nossal, 1976; Drake, 1993; Reha-Krantz & Nonay, 1993; Reha-Krantz, 1995).
Differential fidelity of Pol III HE in leading and lagging strands
Based on the differential enzymology of leading- and lagging-strand polymerization (continuous synthesis in the leading strand and discontinuous in the lagging strand), it is a relevant question to ask whether replication fidelity is identical in the two strands or whether they might differ. In the latter case, most of the replication errors may result predominantly from one of the two strands. This question has been addressed in E. coli by investigating the reversion of certain lacZ alleles when placed in the two possible orientations on the E. coli chromosome. The logic for this type of experiment is that when a given base substitution is mediated by a known mispair (e.g. Ttemplate·G errors causing A·T→G·C base substitutions), inversion of the gene orientation will place the causative error from, for example, the leading strand to lagging strand or vice versa. Thus, any difference observed in the mutation rate between the two orientations may be indicative of strand-dependent replication fidelity. These experiments have been performed with several lacZ alleles under a large series of circumstances (Fijalkowska et al., 1998; Maliszewska-Tkaczyk et al., 2000; Gawel et al., 2002a, b; Banach-Orlowska et al., 2005; Kuban et al., 2005; Makiela-Dzbenska et al., 2009; Gawel et al., 2011). The conclusion reached from these experiments is that indeed there is a significant difference in the error rate depending on the gene orientation. This difference is generally 2- to 6-fold, with the lagging-strand replication being more accurate. Therefore, the majority of replication errors result from leading-strand replication (Fijalkowska et al., 1998). It should be noted that the critical experiments were all performed in a mismatch-repair-defective (mutL) background (see Fig. 1), so that the outcomes reflect the direct production of the errors without interference of the subsequent mismatch repair step, which may have its own specificity.
Differential leading- and lagging-strand replications have also been described in eukaryotic systems, like S. cerevisiae (Pavlov et al., 2002; Pursell et al., 2007; Nick McElhinny et al., 2008). In this case, the fidelity differences are ascribed to replication being performed by different enzymes in the two strands (e.g. Pol ε and Pol δ in leading and lagging strands, respectively). However, in the E. coli case, both strands are copied by the same polymerase (Pol III) and the differential outcome must reflect a different behavior of the same enzyme in its two configurations. The reason why in E. coli leading and lagging strands are copied with differential fidelity is still open at this time, but some clues may be found in the experiments focusing on the role of the accessory DNA polymerases, as described in the following sections.
DNA polymerase switching
The question whether the E. coli accessory DNA polymerases have access to the DNA replication process and hence may contribute to the observed error rate may be raised for several reasons, but most directly based on the relatively high intracellular concentrations of Pol I (400 molecules per cell), Pol II (50 molecules per cell), or Pol IV (200–250 molecules per cell), compared to those estimated for Pol III HE (10–20 molecules per cell) (Kornberg & Baker, 1992; Qui & Goodman, 1997; Kim et al., 2001; McHenry, 2003). The term ‘DNA polymerase switching’ is used to describe a process by which one DNA polymerase (e.g. the major replicative DNA polymerase) is replaced, temporarily, by another DNA polymerase at the 3′-OH end of growing chain, possibly in a coordinated manner. This type of DNA polymerase exchange occurs normally during DNA replication of lagging-strand DNA synthesis. Lagging-strand replication starts with the synthesis of a short RNA primer by DNA primase (DnaG in E. coli) followed by a switch replacing the primase by the main replicating polymerase for the elongation of the strand. When the polymerase reaches the end of the Okazaki fragment, a second switch occurs, replacing the polymerase by an enzyme (Pol I in E. coli) capable of removing the RNA primer and filling the remaining gap.
Do other, similar types of DNA polymerase exchanges occur at the replication fork during ongoing DNA replication, allowing alternative polymerases to synthesize parts of the chromosome and contribute to the overall replication fidelity? The possible mechanisms that promote or enable polymerase switches have been the subject of several investigations. In vivo data clearly indicate that in prokaryotic cells the β sliding-clamp, like PCNA (Proliferating Cell Nuclear Antigen) in eukaryotes, is the important platform that coordinates the participation of different polymerases (Becherel et al., 2002; Lenne-Samuel et al., 2002; Heltzel et al., 2009a; reviewed in Sutton, 2010). In vitro data also demonstrate the possibility of polymerase exchanges during ongoing DNA synthesis, showing that DNA polymerases compete depending on polymerase concentrations and their affinity to the β-clamp (Indiani et al., 2005, 2009; Furukohri et al., 2008; Heltzel et al., 2009b).
Role of DNA polymerase II (Pol II)
DNA polymerase II, encoded by the polB (dinA) gene, was discovered in 1970 (Knippers, 1970). Some of its properties are presented in Fig. 3. Pol II is a prototype for the B-family polymerases, which mostly contain replicative DNA polymerases, including the major eukaryotic DNA polymerases α, δ, ε, as well as DNA polymerase ζ (Bonner et al., 1990). Purified Pol II protein is a single 90-kDa polypeptide possessing both a DNA polymerase and a 3′→5′ exonuclease (Cai et al., 1995). There are 30–50 molecules of Pol II per cell, which is several times more than the number of Pol III HE molecules (Qui & Goodman, 1997). The level of Pol II increases about sevenfold following SOS induction (global response to DNA damage) (Bonner et al., 1990; Iwasaki et al., 1990). Genetic studies indicate that Pol II may be involved in a variety of cellular activities including repair of intrastrand cross-links (Berardini et al., 1999), repair of DNA damaged by UV irradiation and replication restart after UV irradiation (Masker et al., 1973; Rangarajan et al., 1999), repair of DNA damaged by oxidation (Escarceller et al., 1994), stress-induced mutagenesis (Foster et al., 1995; Hastings et al., 2010), and long-term survival (Yeiser et al., 2002). It has been also shown that although Pol II is a proofreading-proficient enzyme, it can carry out error-prone TLS at certain lesions (Becherel & Fuchs, 2001; Wang & Yang, 2009). In vitro studies have shown that Pol II interacts with the β-clamp (β2) and the clamp-loading complex (γδδ′χψ), both major Pol III accessory proteins, to become competent for synthesizing DNA with high fidelity and processivity (Wickner & Hurwitz, 1974; Hughes et al., 1991; Bonner et al., 1992; Heltzel et al., 2009a). Thus, E. coli, besides Pol III, possesses another DNA polymerase capable of participating, at least in principle, in chromosomal DNA synthesis.
The above properties of Pol II have given rise to the concept that this enzyme may function as a back-up polymerase for Pol III HE (Banach-Orlowska et al., 2005). In this model, Pol II may occasionally take the place of Pol III through polymerase switching. Initially, this concept was rather difficult to accept, as experiments with E. coli strains deleted for Pol II did not show significant effects on the chromosomal error rate (Rangarajan et al., 1997; Banach-Orlowska et al., 2005). However, a role of Pol II in chromosomal DNA synthesis was revealed through experiments using mutants carrying a proofreading-deficient form of Pol II (PolBex1). The underlying rationale for the experiments replacing the accurate, proofreading-proficient form of Pol II by its proofreading-deficient and error-prone form (PolBex1) is that in a background of high-fidelity DNA synthesis (by Pol III HE), even a small amount of Pol II-mediated synthesis may be detectable through an increase in the mutation frequency (mutator phenotype). Initially, this strategy was used to demonstrate a polBex1-mediated increase in chromosomal rpoB mutations in the dnaE915 antimutator background (Rangarajan et al., 1997). The dnaE915 allele encodes a mutant Pol III α-subunit that promotes higher accuracy of chromosomal replication (Fijalkowska & Schaaper, 1993; Fijalkowska et al., 1993), and it has been assumed that the more prominent apparent role of the polBex allele in the dnaE915 background is a consequence of either the reduced background of HE-mediated mutations, making it easier to see the Pol II effect, or a possibly enhanced tendency of the DnaE915-encoded polymerase to dissociate from the template and hence to exchange places with Pol II (Fijalkowska et al., 1993; Fijalkowska & Schaaper, 1995; Rangarajan et al., 1997). Regardless of the precise mechanisms, these experiments highlight the potential of Pol II to participate in chromosomal DNA synthesis.
Using the lacZ leading/lagging system described earlier, Banach-Orlowska et al. (2005) also demonstrated that the presence of the proofreading-deficient Pol II (PolBex1) in the cell significantly increased the mutant frequencies, however, not only in cells carrying dnaE915 but also in dnaE+ cells. Even more interestingly, the polBex1 mutator effect was more pronounced for the lagging strand. These results suggested that Pol II has access to the chromosomal replication fork and participates in the replication process, possibly in a strand-preferential way. Interestingly, no significant changes in mutability were observed in cells lacking Pol II (ΔpolB strains), suggesting that any DNA synthesis performed by wild-type (proofreading-proficient) Pol II is generally error-free.
We have proposed that the role of Pol II in DNA replication is that of a back-up polymerase to Pol III HE. There are likely to be situations where HE may temporarily dissociate from the primer terminus, possibly randomly, but more plausibly only in special situations where HE could temporarily stall, such as at DNA lesions or secondary structures. We have proposed that the fidelity role of Pol II is most easily explained by a switch-over from HE to Pol II at terminal mismatches created by a HE misinsertion error. Extension of terminal mismatches is generally difficult for DNA polymerases (Perrino & Loeb, 1989; Mendelman et al., 1990; Joyce et al., 1992), and in vitro data on α subunit and HE have confirmed this to be the case also for Pol III (Kim & McHenry, 1996; Mo & Schaaper, 1996; Pham et al., 1998, 1999). While a majority of terminal mismatches are expected to be removed by the proofreading activity of Pol III (ε subunit), a certain fraction of errors will escape the exonuclease, presenting a critical decision point for the polymerase. Extension of the mismatch would fix the error into a potential mutation, while Pol III dissociation from the mismatch would allow for additional scenarios. Take-over of the terminal mismatch by Pol II is expected to lead to the removal of the mismatch by the Pol II 3′-exonuclease, a clear fidelity function. On the other hand, a take-over by the exonuclease-deficient Pol II would likely lead to the extension of the mismatch – fixing the error – consistent with the observed polBex mutator effect. This model has the added advantage that extensive chromosomal synthesis by Pol II need not be invoked to explain the polBex mutator effect (Banach-Orlowska et al., 2005). The possibility that the proofreading activity of one polymerase can correct errors made by another polymerase has been shown in S. cerevisiae cells (Pavlov et al., 2004).
Further support for the involvement of Pol II in DNA replication and the proposed sequential action of Pol III and Pol II came from experiments showing that the polBex allele synergistically enhanced a Pol III proofreading defect (dnaQ mutant) or Pol III mutator effect (dnaE486 or dnaE511 mutants) (Banach-Orlowska et al., 2005). Again, the simplest interpretation of these results is that when Pol III HE has problems (e.g. stalling owing to increased mismatch production and/or defective polymerase) and the frequency of its dissociation increases, the access of Pol II to the terminal mismatch also increases. This model for the participation of Pol II is presented in Fig. 4.
Role of Pol IV at the replication fork
DNA Polymerase IV (Pol IV) is one of the two main TLS polymerases of E. coli, the other being Pol V (see section below), both members of Y family of polymerases (Reuven et al., 1999; Tang et al., 1999; Wagner et al., 1999). Pol IV, encoded by the damage-inducible dinB gene, is a single-polypeptide enzyme lacking intrinsic proofreading activity, and its fidelity is considered to be relatively low (Tang et al., 2000; Goodman, 2002). The constitutive intracellular concentration of Pol IV is fairly high (250 molecules per cell) and increases by about 10-fold upon SOS induction (Kim et al., 2001). The high constitutive presence of this polymerase in the cell raises the question what its role might be and whether it might have occasional access to the replication fork and affect the overall chromosomal fidelity. Owing to the lack of exonucleolytic proofreading activity, its involvement in replication, if any, is expected to be error-prone.
Goodman (2002) proposed that in certain situations, for example at blocked replication forks, Pol IV might gain access to the nascent 3′-end and perform remedial DNA synthesis. This possibility again raised the question of any possible Pol IV contribution to spontaneous mutagenesis. However, three independent studies demonstrated that in growing cells the lack of Pol IV did not significantly reduce the level or types of spontaneous chromosomal mutations (McKenzie et al., 2003; Kuban et al., 2004; Wolff et al., 2004). This indicated that access of Pol IV to the replication fork must be limited under normal growth conditions, at least as far as any error-prone role is involved (an error-free role would not be readily detectable in these assays). On the other hand, overproduction of Pol IV, from low- or medium-copy number plasmids, clearly resulted in a mutator phenotype (Kim et al., 1997; Wagner & Nohmi, 2000; Kuban et al., 2005). Interestingly, our group also showed that this Pol IV mutator effect occurs preferentially during lagging-strand synthesis, similar to the mutator effect of polBex1 strains (Banach-Orlowska et al., 2005; Kuban et al., 2005). Furthermore, the expression of dinB from a medium-copy plasmid led to a threefold decrease in viability, indicative of some deleterious effects of Pol IV overproduction (Kuban et al., 2005), consistent with experiments in which Pol IV was overexpressed from an arabinose-inducible promoter (Uchida et al., 2008), which showed the inhibition of DNA synthesis and a dramatic loss of viability when Pol IV levels were increased up to 15-fold higher than observed in SOS-induced cells (Uchida et al., 2008). Clearly, Pol IV can compete with HE when its concentration is sufficiently elevated.
To account for the mutator effect resulting from Pol IV overproduction, two simple models can be proposed. In the first model, the increased number of mutations results from errors made by Pol IV during ongoing synthesis. However, this would require extensive synthesis by Pol IV, especially in view of the low processivity of Pol IV (even when supported by the β-clamp) (Wagner et al., 2000; Kobayashi et al., 2002). For example, assuming that Pol IV is 100-fold less accurate than Pol III, the 10-fold mutator effect would require 10% of the chromosome to be replicated by Pol IV. In the second, probably more plausible model, the Pol IV mutator activity results from the error-prone extension of mismatches made by Pol III HE, similar to the proposed model for the PolBex mutator effect (see above). Again, terminal mismatches present a logical step-up point for accessory polymerases, and their effect could be either mutagenic or antimutagenic depending on the nature of the accessory polymerase. Support for this view of Pol IV-mediated mismatch extension is found in experiments where greater than additive effects were observed when Pol IV overproduction is performed in dnaQ928, dnaE486, or dnaE511 mutator strains, which contain functionally impaired ε (dnaQ) or α (dnaE) subunits (Kuban et al., 2005). As the dnaQ or dnaE mutator alleles are expected to increase the number of replication errors (i.e. terminal mismatches), a multiplicative or at least a greater than additive effect is expected.
The experiments with the dnaQ or dnaE mutator alleles, where replication produces increased number of terminal mismatches, provide a useful testing ground for probing the competition between various polymerases, in particular competition between accessory polymerases Pol II and Pol IV. These experiments were performed in dnaE or dnaQ mutator strains lacking Pol II, Pol IV, or both (Banach-Orlowska et al., 2005; Makiela-Dzbenska et al., 2009). In contrast to what is observed in dnaE+ strains, the lack of Pol II (ΔpolB) in dnaE486 or dnaE511 strains led to a 10- or 7-fold increase in the mutator effect, respectively. The lack of Pol IV (ΔdinB) reduced the mutator activity of dnaE486 or dnaE511 by twofold. Both results are consistent with an important role of the two accessory polymerases in establishing the replication error rate: Pol II in a mutation-preventive mode and Pol IV in a mutation-enhancing mode. When both accessory polymerases were deleted, the mutability of dnaE strains was similar to that observed when only Pol IV was lacking. The results are fully consistent with a model in which access of Pol IV leads to mutagenesis, and this is a major component of the dnaE or dnaQ mutator effects, whereas Pol II is strongly antimutagenic, most simply envisaged by competing out Pol IV for access to the mismatch.
Interestingly, the (dinB-dependent) 10- or 7-fold increase in mutagenesis of dnaE486 ΔpolB or dnaE511 ΔpolB strains is much lower than the increase caused by the presence of polBex1 allele (55- to 280-fold) (polBex dnaE486 or polBex dnaE511). This large 55- to 280-fold effect indicates that Pol II's role in editing mismatches in dnaE486 or dnaE511 cells is much larger than anticipated from the ΔpolB or ΔpolB ΔdinB experiments. Presumably, in the absence of Pol II, Pol IV still has limited access and will need to compete with other factors, most likely Pol III HE. Taken together, these in vivo experiments indicate that Pol II along with its proofreading activity serves as an important back-up system for error removal and at the same time protects primer termini against the activity of error-prone Pol IV. These functions become particularly important under conditions of a malfunctioning of Pol III HE. The role of Pol IV in lagging-strand replication and its competition with Pol II is schematically presented in Fig. 4.
Role of DNA polymerase V (Pol V)
Pol V, encoded by the umuDC operon, is, like Pol IV, a member of the Y family of polymerases (Reuven et al., 1999; Tang et al., 1999; Wagner et al., 1999). See Fig. 2 for some of its properties. Pol V is a heterotrimeric complex (), containing the umuC gene product representing the catalytic subunit, and two copies of UmuD′, a product of RecA-facilitated autodigestion of UmuD protein (Nohmi et al., 1988; Shinagawa et al., 1988; McDonald et al., 1998). Pol V is clearly an error-prone enzyme, as it lacks proofreading activity and has a promiscuous base insertion fidelity that allows it to copy across a variety of DNA lesions (TLS polymerase) at the expense of high levels of mutagenesis (Reuven et al., 1999; Tang et al., 1999, 2000). The level of Pol V in normal (noninduced) cells is low and largely undetectable (Woodgate & Ennis, 1991), although certain genetic experiments have suggested that it is not entirely absent (e.g. Bhamre et al., 2001). However, importantly, upon SOS induction, the level of Pol V increases dramatically, producing 2400 molecules of UmuD and 200 molecules of UmuC (Woodgate & Ennis, 1991; Kim et al., 2001).
As normally Pol V is rarely expressed in the cell, it does not play a significant role in determining the chromosomal replication fidelity under normal (non-SOS-induced) growth conditions (Nowosielska et al., 2004). On the other hand, its potential of interfering with ongoing chromosomal replication can be seen in strains in which the SOS system (and hence Pol V) is induced constitutively in the absence of exogenous DNA damage. This condition of ‘spontaneous SOS induction’ is achieved in certain recA strains (recA441, recA730) in which the RecA regulatory protein is constitutively active, leading to constitutive expression of the SOS system, including the overproduction of Pol V as well as Pol IV (Witkin, 1974; Witkin et al., 1982; Tessman & Peterson, 1985). In these strains, increased mutagenesis is observed in the absence of any DNA-damaging treatment (Castellazzi et al., 1972; Ciesla, 1982; Witkin & Kogoma, 1984; Sweasy et al., 1990). This phenomenon of increased spontaneous mutagenesis is named the ‘SOS mutator phenotype’ or ‘untargeted SOS mutagenesis’ (Caillet-Fauquet & Meanhaut-Michel, 1988). Genetic studies on the recA730-induced SOS mutator phenotype led to a postulated model in which the Pol V-mediated increase in mutagenesis results from Pol V displacing HE at HE-generated terminal mismatches (insertion errors) leading to error-prone extension of these mispairs (Fijalkowska et al., 1997). This type of mispair extension is likely further aided by the observed increases in cellular dNTP levels in SOS-induced cells (Gon et al., 2011). As noted above for Pol II and Pol IV, error-prone extension of pre-existing mispairs is an economical way of accounting for the increased mutation rates, as opposed to postulating extensive synthesis by Pol V and accounting for the high error rate by Pol V-mediated synthesis errors (Maliszewska-Tkaczyk et al., 2000).
Among the base substitution mutations that are enhanced in recA730 strains, transversions predominate (Fijalkowska et al., 1997; Maliszewska-Tkaczyk et al., 2000; Kuban et al., 2006). This finding is consistent with in vitro data showing that transversion mismatches are most difficult to extend by HE (and more difficult to proofread) and result in DNA polymerase stalling (Kim & McHenry, 1996). It was suggested that the transient stalling of Pol III HE at terminal mismatches may stimulate the dissociation of HE, allowing extension of mismatches by Pol V (Fijalkowska et al., 1997). Overall, the data strongly support the idea that in recA730 strains, and in SOS-induced cells in general, there is a competition between the major replicase (HE) and error-prone Pol V (Fijalkowska et al., 1997; Timms & Bridges, 2002; Vandewiele et al., 2002).
As SOS induction leads to enhanced levels of both Pol V and Pol IV, the participation of the latter in the SOS mutator activity also requires consideration. To address this question, our group showed that deletion of Pol IV from recA730 cells (recA730 ΔdinB::kan) reduced mutagenesis relative to the dinB+recA730 strain by at least twofold (Kuban et al., 2006). As loss of Pol V (ΔumuDC recA730 strain) completely abolishes the recA730 mutator effect (Witkin & Kogoma, 1984; Sweasy et al., 1990), it was concluded that both Pol V and Pol IV are required for full expression of the mutator effect, with Pol V playing the critical role, presumably in extending the primary mismatch. Pol IV may participate in further extension of the Pol V-generated product, thereby improving the likelihood that the mismatch-containing DNA is ultimately converted into a mutation (Kuban et al., 2006).
Studies of the strandedness of the Pol V-mediated SOS mutator effect clearly indicated that the effect results primarily, if not exclusively, from events during lagging-strand replication (Maliszewska-Tkaczyk et al., 2000; Kuban et al., 2005). This preference mimics that of the Pol IV mutator effect and, to some extent, the PolBex mutator effect (see above). Clearly, the lagging strand is more accessible for accessory polymerases. This is consistent with the greater dissociativity of HE in the lagging strand. See also Fig. 4.
Role of DNA polymerase I (Pol I)
DNA polymerase I, encoded by the polA gene, was the first polymerase ever identified (Bessman et al., 1956; De Lucia & Cairns, 1969). Pol I is the most abundant DNA polymerase in E. coli (~ 400 molecules per cell) (Kornberg & Baker, 1992). Pol I, a 103-kDa protein, possesses three enzymatic activities: the 5′→3′ polymerase, a 5′→3′ exonuclease, and a 3′→5′ proofreading exonuclease (Joyce & Grindley, 1984). The polymerase and 5′→3′ exonuclease activities enable Pol I to fulfill its primary role in DNA replication: to remove RNA primers and fill the resulting gap during the maturation of Okazaki fragments in the lagging strand (Okazaki et al., 1971). Pol I also fills gaps generated during DNA repair and recombination (Cooper & Hanawalt, 1972; Kornberg & Baker, 1992; Friedberg et al., 2006). Pol I, which is presumably capable of interacting with the β-processivity clamp, is a competent high-fidelity enzyme and should be capable, in principle, of competing with HE, similar to Pol II and Pol IV (López de Saro & O'Donnell, 2001).
The role of Pol I in chromosomal replication fidelity has been investigated (Curti et al., 2009; Makiela-Dzbenska et al., 2009, 2011), most productively using a proofreading-deficient variant of Pol I (polAexo mutant), analogously to the polBex mutant described above. The logic behind these experiments is again that small, normally error-free, contributions of Pol I would be observable as an increase in the mutation frequency when substituted by its error-prone proofreading-deficient counterpart. A 1.5- to 4-fold increase in mutant frequencies was observed in polAexo cells, indicating that Pol I indeed plays a role in fidelity. Three separate observations in these studies led us to further define this role: (1) the polAexo mutator effect has a lagging-strand preference, (2) there is no synergism between the polAexo mutator effect and the mutator effects exerted by other DNA polymerases or replication defects, and (3) no competition could be demonstrated between Pol I, on the one hand, and Pol II and Pol IV on the other. Based on these results, we concluded that Pol I does not compete directly at the growing point in the replication fork. Instead, the fidelity role of Pol I is concerned primarily with the error-free processing of the Okazaki fragment gaps, consistent with the established role of Pol I in the maturation of Okazaki fragments. In E. coli, Okazaki fragments average between 1000–2000 nucleotides, while the length of RNA primers is 10–20 nucleotides (Zechner et al., 1992a, b). Thus, Pol I is likely responsible for 1–2% of DNA synthesis in the lagging strand. However, if even such a relatively small fraction of chromosomal DNA is synthesized by an enzyme that is 50- to 100-fold less accurate (polAexo) than Pol III, then a 2% contribution in DNA replication may produce a twofold increase in the chromosomal error rate. See Fig. 4 for inclusion of Pol I in the overall chromosomal fidelity scheme.
Role of the Pol III HE τ subunit in fidelity and polymerase switching
The dnaX gene encodes both the τ and γ subunits of HE (Fig. 2). τ is the gene's full-length (643 amino acid) product, while γ is a truncated product lacking the C-terminal residues because of a translational frameshifting event at residues 428–430 (Flower & McHenry, 1986; Blinkowa & Walker, 1990). While γ, as part of the γδδ′ complex, is responsible for loading and unloading the β-clamps from DNA (reviewed in Bowman et al., 2005), τ fulfills several additional critical functions, both structurally and mechanistically, owing to its unique C-terminus (for a review, see McHenry, 2011). Foremost, τ dimerizes the two pol III cores within HE, creating the dimeric polymerase that is capable of copying the two DNA strands simultaneously. τ interacts with the DnaB helicase (Gao & McHenry 2001) and regulates in this manner the speed of the replication fork (Dallmann et al., 2000). τ also controls the cycling of the lagging-strand polymerase, as it mediates the release of the Pol III core from its β-processivity clamp upon the completion of Okazaki fragments (Leu et al., 2003; López de Saro et al., 2003). Based on the central role of τ within HE, including its direct interaction with both the leading- and lagging-strand polymerase, a role of τ in determining the fidelity of HE, either directly or via an effect on polymerase switching, might be expected. Indeed, a survey of several dnaX(Ts) mutants revealed a mutator phenotype, at permissive temperatures, for the dnaX36 and dnaX2016 alleles (Pham et al., 2006). The dnaX36 mutator was considered particularly interesting because its underlying mutation (E601K) is located in the C-terminus of DnaX and is hence unique to τ (Pham et al., 2006). Analysis of the specificity of mutagenesis of the dnaX36 mutator revealed a unique pattern: transversion base substitutions as well as (−1) frameshifts in nonrun sequences are specifically enhanced (Pham et al., 2006). Based on these and other data, it was concluded that τ subunit is an important factor in controlling the accuracy of chromosomal replication. Further, its effect is likely mediated at the processing stage of HE-made replication errors – rather than the initial error production by HE.
Studies on the strandedness of the dnaX36 mutator effect revealed that the effect applied to both strands, although with a slight preference for the lagging strand (Gawel et al., 2011). It was also found that the dnaX36 mutator effect was largely independent of dinB and that hence it is not mediated by an increased switch-over of HE to error-prone Pol IV. On the other hand, an enhancement of the dnaX36 mutator effect was observed in the ΔpolB background, most pronounced for the lagging strand (Gawel et al., 2011). These results indicate that Pol II plays a role in preventing mutations in dnaX36 strains and that this role may be more important in lagging-strand replication. This is in contrast to the situation in dnaX+ strains, where the ΔpolB has no effect (Rangarajan et al., 1997; Banach-Orlowska et al., 2005). This suggests that in the dnaX36 mutant Pol II has increased access to the replication fork and that in this case Pol II acts to prevent mutations (Gawel et al., 2008; 2011). Part of this role of Pol II is to outcompete access by Pol IV, because the dnaX36 ΔpolB ΔdinB triple mutant has reduced mutability relative to the dnaX36 ΔpolB strain (Gawel et al., 2008, 2011).
The important role of Pol II in preventing replication errors was demonstrated most dramatically when dnaX36 was combined with the polBex1 proofreading deficiency. In this case, the polBex1 deficiency increased the mutant frequencies dramatically (20- to 50-fold) above the dnaX36 level, and this was true for both leading and lagging strands. The strong polBex1 mutator effect resulting from the Pol II proofreading deficiency is not dependent on the action of Pol IV, because the dnaX36 polBex1 ΔdinB triple mutant behaved essentially as the dnaX36 polBex1 strain (Gawel et al., 2008; 2011). This again indicates that Pol II is very effective in preventing access by Pol IV. Overall, these results highlight the important role that Pol II can play in controlling the fidelity. It should be noted that within the favored model of Pol II as a back-up proofreader for HE-made insertion errors, a 50-fold mutant frequency increase by the polBex1 allele could indicate that some 98% of Pol III errors become a substrate for Pol II. When the normal, wild-type Pol II is present, these errors are efficiently removed by Pol II's proofreading activity, while in case of the polBex1 allele, they have a high chance of being extended by Pol II to fix the error into a potential mutation (Gawel et al., 2008, 2011).
What do these results tell us about the fidelity function of τ subunit? The defect in dnaX36 is in Domain V of DnaX, which is responsible for the α–τ interaction (Gao & McHenry 2001; Pham et al., 2006; Su et al., 2007). The relevance of this location to the mutator effect was further evidenced by the isolation of an additional set of dnaX mutators with properties similar to dnaX36 and all located in Domain V (Pham et al., 2006). Thus, an altered or impaired α–τ interaction underlies the observed mutator effect. It may be that the impaired α–τ interaction leads to more frequent Pol III dissociations. If so, the sole fidelity function of τ would be to keep HE together in its dimeric state and on the primer templates; upon dissociation, less accurate polymerases may take a turn, accounting for the mutator phenotype. While this is a possibility, the model does not readily account for (1) the strength of the dnaX36 mutator effect (too much synthesis by error-prone enzymes required), (2) the independence of the mutator effect of Pol IV, the major candidate for error-prone interference, (3) the substantial mutator effect of dnaX36 ΔpolB ΔdinB strains (i.e. even in the absence of Pol II and Pol IV), as well as (4) the unusual specificity of the mutator effect: preferential enhancement of transversion base substitutions as well as −1 frameshifts in nonrun sequences (Pham et al., 2006; Gawel et al., 2008, 2011).
As a preferred model, we have suggested that the fidelity function of τ results from its role in assisting HE when it is faced with terminal mismatches created by the α subunit (Maliszewska-Tkaczyk et al., 2000; Banach-Orlowska et al., 2005; Kuban et al., 2005; Gawel et al., 2008; Makiela-Dzbenska et al., 2009). Terminal mismatches are more difficult to extend (Perrino & Loeb, 1989; Mendelman et al., 1990; Joyce et al., 1992; Kim & McHenry, 1996) and temporary stalling will ensue. In most cases, this stalling will lead to a conformational switch moving the primer terminus to the exonuclease (proofreading) subunit leading to the removal of the incorrect nucleotide. However, a subset of errors may be refractory to this mechanism (Kim & McHenry, 1996; Pham et al., 2006), leading to a longer-lived type of stalling, which may impede the progress of the replication fork. Evidence for this type of HE stalling has been obtained in in vitro fidelity experiments (Pham et al., 2006; R. M. Schaaper, unpublished data). We propose that, in vivo, this type of stalling is sensed and remedied by τ subunit, leading to the removal of the error and continuation of DNA synthesis. This role of τ as sensor for a stalled polymerase is similar to, and may share features with the proposed sensing role of τ in the lagging strand that leads to the release of the polymerase in this strand when it reaches the end of the Okazaki fragment (Leu et al., 2003; López de Saro et al., 2003; McInerney et al., 2007).
This τ-mediated fidelity mechanism operates on both leading and lagging strands (Gawel et al., 2011). How τ promotes error removal is not yet known, but in the simplest case it may involve enforcing the required conformational switch in α that places the erroneous terminal nucleotide in the ε exonuclease site. Alternatively, τ may dislodge Pol III and channel the mismatch toward the exonuclease of Pol II or, possibly, to the third Pol III core if present at the replication fork (Georgescu et al., 2012). Obviously, in the absence of this τ function (as in the dnaX36 mutant), this mechanism is inoperative, and Pol III may eventually extend the mismatch, accounting for the dnaX mutator effect. This model is supported by the specificity of the dnaX mutator effect: transversions and nonrun (−1) frameshifts are specifically enhanced. Polymerase stalling is most pronounced at transversion mismatches (purine–purine or pyrimidine–pyrimidine mispairs) (Perrino & Loeb, 1989; Mendelman et al., 1990; Joyce et al., 1992; Kim & McHenry, 1996), and their ability to be proofread may also be limited (Kim & McHenry, 1996; Pham et al., 1998, 1999). Forced extension of such mismatches will naturally lead to transversion base-pair substitutions or, a preferred option in permissible sequence contexts, (−1) frameshifts by misalignment of the incorrect base on the next complementary template base (Mo & Schaaper, 1996; Pham et al., 1998, 1999).
Summary and concluding remarks
The results of the studies clearly indicate that the accessory DNA polymerases of E. coli can, at least occasionally, obtain access to the replication fork and participate in chromosomal replication, affecting in this manner the overall replication fidelity and the resulting bacterial mutation rate. Depending on the polymerase, the effect may be to improve the fidelity (for the proofreading-proficient enzymes, such as Pol I or Pol II) or to produce an increased number of mutations (for the error-prone polymerases, Pol IV or V). Our data and interpretations are presented most straightforwardly using the cartoon of Fig. 4.
In a most parsimonious model, DNA Pol III HE, as an efficient and high-speed polymerase machine, is not expected to give way to accessory polymerases unless provoked by conditions impeding its progress. One such case, most relevant to the fidelity issue, is the expected stalling on terminal mismatches, from which it is difficult to continue synthesis especially for high-efficiency enzymes with ‘tight’ catalytic sites (Beard & Wilson 2003). We have indicated this in Fig. 4, where HE is temporarily stalled on a (e.g. T:T or A:A) mismatch. If the mismatch cannot be rapidly proofread by HE, the enzyme may temporarily release the 3′ terminus, providing access opportunities for accessory polymerases. Entry by an exonuclease-proficient enzyme like Pol II would lead to the removal of the terminal mismatch, especially because DNA polymerases – when first binding to a primer terminus – do so with their exonuclease site rather than the polymerase site (Johnson, 1993). This represents the basis of the postulated role of Pol II as a back-up proofreader for Pol III-mediated replication errors. Importantly, our data indicate that Pol II performs this role in both the leading and lagging strands.
Under conditions where Pol IV or Pol V is present at elevated levels, they too can gain access to the abandoned primer termini. However, they have to compete with Pol II. Our results clearly indicate that, for example, the mutagenic potential of Pol IV is strongly limited by the presence of Pol II (Banach-Orlowska et al., 2005; Gawel et al., 2008, 2011). However, the issues are clearly more complicated than the simple model might suggest, as Pol IV and Pol V, in contrast to Pol II, appear restricted in their actions primarily to the lagging strand. Thus, the dissociative events at terminal mismatches in the two strands are likely to be different mechanistically, perhaps reflective of the normally different behavior of the Pol III core in the two strands (highly processive vs. discontinuous in leading vs. lagging strands, respectively). It may be that the polymerase switch in the leading strand follows a prescribed and controlled pattern that favors the recruitment of Pol II or a return of Pol III itself, while the switch in the lagging strand may resemble more a ‘free-for-all’ type of switch.
The precise nature of these events remains to be determined, although, as discussed above, the action of τ subunit is likely to be a critical factor, acting as a sensor for stalled polymerases and/or as a switch that remedies the stalled situation. One particular class of dnaX mutants, exemplified by dnaX36, displays a unique mutator effect that appears fully consistent with a malfunctioning of this τ-mediated sensing and/or switching mechanism, and in these strains, Pol III might be forced to extend errors that would normally be resolved. Additional genetic experiments as well as biochemical approaches will be needed to provide further insight into these intriguing mechanisms.
The other important issue that needs to be further addressed is why in normal, wild-type cells the fidelity of lagging-strand replication is several-fold higher than that of the leading strand. It was suggested that the lagging-strand replication has at least one additional mechanism available for error correction, possibly related to more facile polymerase dissociation in this strand (Fijalkowska et al., 1998). If enhanced dissociation leads to more frequent engagement of Pol II, the greater fidelity of lagging-strand replication could be readily explained. Consistent with this idea is the stronger lagging-strand mutator effect associated with the exonuclease-deficient polBex1 allele (Banach-Orlowska et al., 2005). However, the situation is not so simple, as in the polBex1 strain an inversion of strand bias is actually observed for some of the tested lacZ markers (i.e. leading-strand replication is now more accurate). Thus, this question will also require further investigation.
The authors thank Drs K. Bebenek and A. Clausen for their careful reading of the manuscript for this paper. The work described in this review was supported by grant 2 PO4A 061 30 (to I.J.F. and P.J.) from the Polish Ministry of Science and Higher Education, and project number Z01 ES065086 of the Intramural Research Program of the NIH, National Institute of Environmental Health Sciences (to RMS), and by the Foundation for Polish Science TEAM Program (to I.J.F.).
I.J.F., R.M.S. and P.J. contributed equally to this paper.