RecQ family helicases catalyze critical genome maintenance reactions in bacterial and eukaryotic cells, playing key roles in several DNA metabolic processes. Mutations in recQ genes are linked to genome instability and human disease. To define the physical basis of RecQ enzyme function, we have determined a 1.8 Å resolution crystal structure of the catalytic core of Escherichia coli RecQ in its unbound form and a 2.5 Å resolution structure of the core bound to the ATP analog ATPγS. The RecQ core comprises four conserved subdomains; two of these combine to form its helicase region, while the others form unexpected Zn2+-binding and winged-helix motifs. The structures reveal the molecular basis of missense mutations that cause Bloom's syndrome, a human RecQ-associated disease. Finally, based on findings from the structures, we propose a mechanism for RecQ activity that could explain its functional coordination with topoisomerase III.
RecQ DNA helicases are ubiquitous enzymes in bacteria and eukaryotes that carry out important functions in genome biology (Cobb et al., 2002; Wu and Hickson, 2002). Like other DNA helicases, RecQ proteins are ATP-dependent molecular motors that unwind double-stranded (ds) DNA. Members of the RecQ family differ from other helicases, however, in their unusual breadth of activities, including roles in DNA replication, recombination, and repair. With their central activities in genome maintenance, it is not surprising that mutation of many known recQ genes leads to genome instability and, in the case of three human recQ genes, to disease. Despite the importance of RecQ proteins, the structural basis of their function has remained poorly defined.
The founding RecQ family member was discovered in Escherichia coli where it functions in the RecF recombination pathway (Nakayama et al., 1984; Umezu et al., 1990). This pathway participates in homologous recombination and repair of ultraviolet light-induced DNA damage (Kowalczykowski et al., 1994). RecQ and other proteins in the RecF pathway appear to catalyze reactions that help repair replication forks that have stalled at sites of DNA damage (Courcelle et al., 1997; Courcelle and Hanawalt, 1999; Courcelle et al., 1999; 2003). In addition, E.coli RecQ helps suppress illegitimate recombination in cells (Hanada et al., 1997). Although the precise cellular substrates on which RecQ proteins act remain a mystery, several reactions catalyzed by E.coli RecQ have been reconstituted in vitro, including ATP-dependent DNA unwinding (Umezu et al., 1990), recombination initiation with RecA and single-stranded (ss) DNA binding protein (SSB) (Harmon and Kowalczykowski, 1998), and plasmid DNA catenation with topoisomerase III (Topo III) and SSB (Harmon et al., 1999). Coordinated activities with recombinases and topoisomerases, as well as DNA unwinding functions, are conserved in a number of eukaryotic RecQ proteins (reviewed in Wu and Hickson, 2001), implying a functional homology among RecQ family members.
Three diseases (Bloom's, Werner's, and Rothmund—Thompson syndromes) can be attributed to mutations of human genes that encode homologs of E.coli RecQ (BLM, Ellis et al., 1995; WRN, Yu et al., 1996; RECQ4, Kitao et al., 1999). While each of these syndromes has distinct clinical manifestations, they all share a predisposition to cancer. A common feature of these disorders is pronounced genomic instability, which is characterized by heightened levels of homologous recombination and/or chromosomal deletions (reviewed in Karow et al., 2000). Several disease-linked nonsense and frame-shift mutations in WRN, BLM, and RECQ4, as well as all known BLM missense mutations associated with Bloom's syndrome, map to regions that are conserved across the RecQ family of enzymes.
Three regions conserved among bacterial and eukaryotic RecQ proteins have been identified by sequence analysis: helicase, RecQ-conserved (RecQ-Ct), and Helicase-and-RNaseD-C-terminal (HRDC) domains (Figure 1A; Morozov et al., 1997). The helicase and RecQ-Ct regions are the best conserved regions among RecQ proteins, with some RecQs lacking an identifiable HRDC domain altogether. The RecQ family helicase region contains sequence motifs that are broadly conserved among DNA unwinding enzymes (Gorbalenya and Koonin, 1993). These motifs link the energy of nucleoside triphosphate binding and hydrolysis to DNA unwinding. The structure and function of the RecQ-Ct region is more poorly understood since it appears to be unique to RecQ proteins. However, evidence indicates that this region is essential for RecQ function. Two disease-causing BLM missense mutations map to the enzyme's RecQ-Ct region (Ellis et al., 1995; Foucault et al., 1997) and abolish BLM ATPase and helicase activities in vitro (Bahr et al., 1998). Mutation and deletion analyses in the Saccharomyces cerevisiae RecQ homolog (Sgs1) have also shown that this region is essential for in vivo function (Mullen et al., 2000; Onoda et al., 2000; Ui et al., 2001). Together, the helicase and RecQ-Ct regions form the core, conserved sequence that defines the RecQ family of enzymes.
Domain mapping experiments with E.coli RecQ have demonstrated that the conserved helicase and RecQ-Ct regions fold together to form a single 59 kDa structural domain (RecQΔC) (Bernstein and Keck, 2003). The isolated RecQΔC domain is active as a DNA-dependent ATPase and can unwind DNA with essentially the same specific activity as full-length E.coli RecQ, indicating that it is the catalytic core of the enzyme (Bernstein and Keck, 2003). The 9 kDa HRDC domain appears to modulate DNA binding activity of the catalytic core but is not necessary for enzyme function in vitro (Bernstein and Keck, 2003). Similarly, an S.cerevisiae Sgs1 variant that lacks its C-terminal HRDC domain can complement the increased DNA damage sensitivity phenotype of sgs1Δ cells (Mullen et al., 2000; Mullen et al., 2001), implying that the HRDC domain is dispensable for at least some activities in vivo. In addition, a recent study has shown that a catalytic core fragment of the human BLM protein that includes just its helicase and RecQ-Ct regions is active in vitro (Janscak et al., 2003). These findings demonstrate that the evolutionarily conserved domain shared among RecQ proteins also forms the structural and catalytic core of the RecQ enzyme family.
Beyond low-resolution domain mapping, a number of other studies have revealed important structural features of RecQ helicases. First, sequence analysis places RecQ family members in the Superfamily 2 (SF2) group of enzymes (Gorbalenya and Koonin, 1993). While structurally similar to Superfamily 1 (SF1) enzymes, SF2 helicases are more similar to each other in sequence within their helicase domains than they are to SF1 enzymes. Secondly, the NMR structure of the S.cerevisiae Sgs1 HRDC domain has been determined (Liu et al., 1999), revealing a domain that shares structural similarity with auxiliary DNA-binding domains in E.coli Rep and Bacillus stearothermophilus PcrA helicases (Subramanya et al., 1996; Korolev et al., 1997). Although this domain is not required for E.coli RecQ function and is not preserved in all RecQ family members, solution of this structure makes an important link to other well-studied helicases. Finally, a number of contradictory studies have investigated the active oligomeric state of RecQ helicases. Three findings indicate that RecQ proteins form oligomeric structures that may be important for their function: (i) E.coli RecQ hydrolyzes ATP with a Hill coefficient of 3 when unwinding DNA, implying that multiple ATPase sites interact during DNA strand separation (Harmon and Kowalczykowski, 2001); (ii) the human BLM protein forms homooligomeric ring structures (Karow et al., 1999); and (iii) Drosophila melanogaster RecQ5 forms homooligomers (Kawasaki et al, 2002). However, other recent findings may indicate that RecQ proteins can operate as monomers. These include a biochemical analysis of E.coli RecQ in centrifugation and kinetic experiments where it was concluded that the enzyme functions as a monomer (Xu et al, 2003), and biochemical experiments with catalytically active recombinant fragments of the human BLM protein that no longer forms hexameric rings but instead exist as monomers (Janscak et al., 2003). Thus the question of the active oligomeric state of RecQ proteins remains unresolved.
To examine the physical basis of RecQ function, we have determined two high-resolution X-ray crystal structures of the conserved catalytic core of E.coli RecQ. The core domain comprises four apparent subdomains; two of the subdomains combine to form the helicase region and the remaining two join to form the RecQ-Ct region of RecQ. The RecQ-Ct subdomains include one that folds as a platform of helices that binds a Zn2+ ion using four conserved cysteine residues and another that forms an unexpected winged-helix (WH) subdomain. The WH motif shares significant structural similarity with other DNA binding proteins, thus identifying a likely DNA binding site in E.coli RecQ. Based on the structures, we propose a mechanism of action that could explain the coordination of RecQ proteins with Topo III. Furthermore, our structures reveal the molecular basis of missense mutations that cause Bloom's syndrome. Together, these structures reveal the first high-resolution images of the enzymatic core conserved among RecQ family members.
Results and discussion
Structure determination of the RecQΔC domain
We first attempted to crystallize full-length E.coli RecQ protein, but extensive crystallization trials yielded no crystals. This result could have been due to flexibility that has been observed between the catalytic core and HRDC domains of E.coli RecQ (Bernstein and Keck, 2003) leading to structural heterogeneity that would hinder crystallization. Since we had characterized the catalytic core domain (RecQΔC) and found that it has essentially the same specific activities as full-length E.coli RecQ in ATPase and helicase assays (Bernstein and Keck, 2003), we subjected RecQΔC to crystallization trials as well and were able to crystallize it in a form that diffracted to 1.8 Å resolution (Table I). The crystal form contained one molecule per asymmetric unit. Crystals of selenomethionine-substituted RecQΔC were used to determine the structure of the domain using single-wavelength anomalous dispersion (SAD) phasing methods (Table I). The final refined model includes both the helicase and RecQ-Ct regions of the protein (residues 1 to 516 of RecQΔC, Figure 1B and C).
Table 1. Data collection, phasing, and refinement
Rsym = ΣΣj|Ij − <I>|/ΣIj, where Ij is the intensity measurement for reflection j and <I> is the mean intensity for multiply recorded reflections.
Rwork, free = Σ||Fobs| − |Fcalc||/|Fobs|, where the working and free R-factors are calculated using the working and free reflection sets, respectively. The free reflections (5% of the total) were held aside throughout refinement.
The RecQΔC structure reveals a modular, tri-lobed molecule that is comprised of four apparent structural subdomains (Figure 1C). The molecule is roughly 40 × 60 × 70 Å in size and forms a Y-shaped structure with major clefts apparent on its surface. The two N-terminal subdomains form distinct lobes of the molecule that combine to make the helicase region. The remaining two subdomains form the RecQ-Ct region, which is the third lobe of the molecule.
Helicase region of RecQ
The two N-terminal subdomains of RecQΔC abut to form a deep cleft in the protein (Figure 1C). Conserved helicase sequence motifs (Gorbalenya and Koonin, 1993) line the cleft walls in an arrangement similar to that observed in other helicase structures (Caruthers and McKay, 2002) (Figure 2A). The RecQΔC helicase region is most similar in structure to helicase domains in other SF2 helicases, including three RNA helicases [Methanococcus jannaschii putative RNA helicase (Story et al., 2001), S.cerevisiae eIF4a (Caruthers et al., 2000), hepatitis C virus NS3 helicase (Yao et al., 1997)], and Thermotoga maritima RecG DNA helicase (Singleton et al., 2001), as well as the helicase domain in Archaeoglobus fulgidus reverse gyrase (Rodriguez and Stock, 2002). The RecQΔC structure also shares significant but lesser structural homology with SF1 DNA helicases and other ATP-binding proteins (see discussion below).
Based upon structural features of the RecQΔC helicase region that are conserved in other helicases, we hypothesized that ATP and ssDNA would bind to distinct sites within the helicase region, as indicated in Figure 2A. Consistent with this prediction, a second crystal structure of RecQΔC soaked in ATPγS, an ATP analog, and Mn2+ showed clear Fo–Fc difference electron density for ATPγS and a metal ion in the predicted ATP binding site (Figure 2B). The adenine moiety is packed between Tyr23 and Arg27 side chains and hydrogen bonds are formed between the N6 and N7 atoms of the adenine and Gln30 of RecQ motif 0. This adenine binding mode likely explains the preference of ATP as a cofactor in E.coli RecQ reactions (Umezu et al., 1990). Structural aspects of adenine binding by PcrA helicase (Subramanya et al., 1996) are strikingly similar to those observed in RecQΔC. The ATPγS triphosphate is bound to RecQΔC by Lys53 and several backbone amides in motif I, and through a Mn2+ ion that makes water-mediated contacts with Ser54 of motif I and Asp146 of motif II.
The presence of a ssDNA binding site between the RecQΔC helicase subdomains is predicted by its structural similarity to PcrA (Velankar et al., 1999), Rep (Korolev et al., 1997), and NS3 (Kim et al., 1998) helicases solved with bound nucleic acid. In these structures, ssDNA binds to the two helicase lobes at a cleft that is on the opposite face from the ATP binding site. The interactions with ss nucleic acid are predominantly through either hydrophobic association with the DNA bases (Velankar et al., 1999), ionic interactions with the substrate backbone (Kim et al., 1998), or a combination of hydrophobic and ionic interactions with the nucleic acid substrate (Korolev et al., 1997). However, an alternative DNA binding mechanism has recently been suggested based on the T.maritima RecG helicase structure. In the RecG model, the helicase domain is proposed to bind to dsDNA and to act as a dsDNA translocase (Singleton et al., 2001). Evidence supporting this model are that the path of dsDNA in the DNA-bound RecG structure extrapolates to the helicase domain (Singleton et al., 2001) and that RecG's ATPase activity is significantly more sensitive to stimulation by dsDNA than ssDNA (Whitby and Lloyd, 1998). While the RecQΔC helicase region is structurally similar to that in RecG, E.coli RecQ's ATPase activity is ssDNA-dependent with only low levels of ATPase activity stimulated by dsDNA (Umezu et al., 1990), and ssDNA-binding features similar to those found in PcrA are present in RecQΔC (see discussion below). Although we cannot rule out a RecG-type dsDNA translocase mechanism based on the structure of RecQΔC, the available evidence does not support this type of reaction. We currently favor a model for RecQΔC DNA binding where ssDNA binds between the two helicase subdomains as has been observed in PcrA, Rep, and NS3 helicases. Elucidation of the structural basis of RecQ DNA binding will require further experimental characterization.
RecQ-Ct region of RecQ
The function of the RecQ-Ct region in RecQ-catalyzed reactions has not been well defined. RecQ-Ct sequences are not found in proteins outside of the RecQ family and previous functional characterization of this region in S.cerevisiae Sgs1 (Mullen et al., 2000; Onoda et al., 2000; Ui et al., 2001), as well as in murine (Bahr et al., 1998) and human (Janscak et al., 2003) BLM proteins has been limited to mutational analyses. These studies indicate the importance of the RecQ-Ct region, but have not resolved its structure or function(s).
The RecQΔC structure shows that the RecQ-Ct region comprises two conserved subdomains. The first forms a platform of helices that is sandwiched between the helicase subdomains of RecQΔC and the rest of the RecQ-Ct region (Figures 1C and 3A). Inspection of the electron density map revealed that the side chains from four highly conserved cysteine residues at the ends of two of these helices were arrayed around a single intense electron density peak. This peak was modeled as a Zn2+ ion since X-ray fluorescence experiments demonstrated that Zn2+ was present in the crystals in spite of its exclusion from any solutions used to purify or crystallize RecQΔC (data not shown). A second indication that this electron density peak identified a bound Zn2+ ion came from biochemical analysis of E.coli RecQ (Figure 3B). In these experiments, the Zn2+ content and the number of solvent-accessible thiol groups in E.coli RecQ were analyzed. The results indicated that E.coli RecQ copurifies with stoichiometric amounts of Zn2+. In addition, dialysis of E.coli RecQ against DTT and EDTA removed ∼2/3 of the bound Zn2+ and uncovered an additional 3–4 solvent-accessible thiol groups, consistent with the Zn2+ binding site being comprised of 3–4 cysteines near the surface of RecQ. These biochemical data correlate well with the observed binding site in the structure.
Given the strong conservation of the Zn2+-binding site among RecQ proteins (Figure 1B), it is perhaps not surprising that functional analyses have shown this region to be important for RecQ function. BLM missense mutation sites in the RecQ-Ct region mutate codons for cysteine residues in BLM protein that are analogous to residues 380 or 397 in E.coli RecQ (Ellis et al., 1995; Foucault et al., 1997; see discussion below). In addition, mutated S.cerevisiae SGS1 genes fail to complement the DNA-damage sensitivity and hyperrecombination phenotypes in an sgs1Δ strain when any of the analogous Zn2+-binding site cysteine residues have been altered (Onoda et al., 2000; Ui et al., 2001). Finally, a number of point mutations in residues analogous to RecQΔC Zn2+-liganding cysteines in either the human BLM protein catalytic core (Janscak et al., 2003) or in E.coli RecQ (M.C.Zittel and J.L.Keck, unpublished observation) result in variants that are difficult to purify due perhaps to rapid proteolysis, indicating that Zn2+ binding to this region may stabilize the protein. The RecQ Zn2+-binding motif is unlike previously observed zinc finger folds (Krishna et al., 2003), and does not have substantial structural similarity with any other known proteins. Future experiments will therefore be needed to determine its specific function in RecQ. Potential functions could include thermodynamic stabilization of the protein and/or acting as a DNA or protein binding site, all of which have been observed for Zn2+-binding domains in other proteins (Berg and Shi, 1996).
The second RecQ-Ct subdomain forms a specialized helix–turn–helix fold called a WH subdomain, which has been found to act as a DNA-binding motif in many proteins (Gajiwala and Burley, 2000; Figure 4A). The RecQ WH fold is structurally homologous to WH domains found in reverse gyrase (Rodriguez and Stock, 2002) and other type-IA topoisomerases (Lima et al., 1994; Mondragon and DiGate, 1999) as well as to several other DNA binding proteins, including the E.coli catabolite gene activator protein (CAP) (Schultz et al., 1991). The intersection of the RecQ WH and Zn2+-binding helical subdomains creates a large cleft on the surface of the protein. Several features of this cleft suggest that it can serve as a binding site for dsDNA: (i) the expected dsDNA binding face of the WH fold, including the putative DNA binding ‘recognition helix’, forms an exposed wall of the cleft; (ii) several residues that mediate WH/DNA phosphate interactions in other proteins are conserved in the RecQ WH domain (Figure 4B); and (iii) superposition of the dsDNA from the CAP/DNA co-crystal structure onto the WH RecQ fold demonstrates that the cleft could accommodate dsDNA without needing to significantly alter the structure of the RecQ-Ct region (Figure 4C). In support of this dsDNA binding model, we have found that a recombinant HRDC domain fragment from E.coli RecQ, which would be localized near the putative dsDNA binding site on the RecQ-Ct region in the full-length protein, has a strong binding preference for dsDNA over ssDNA (D.A.Bernstein and J.L.Keck, unpublished observation). dsDNA binding by the HRDC domain could serve as a clamp to stabilize dsDNA binding to the catalytic core. This model is consistent with previous observations of different DNA binding stabilities between E.coli RecQ and RecQΔC (Bernstein and Keck, 2003).
Comparison of RecQΔC to SF1 and SF2 helicases
Sequence analysis of RecQ proteins have placed them among the SF2 group of helicases (Gorbalenya and Koonin, 1993), which includes several members with known structures. Consistent with its sequence alignment with other SF2 enzymes, the RecQΔC structure is more closely related to other SF2 family members in structure than to SF1 enzymes. For example, the two RecQΔC helicase lobes align better with hepatitis C virus NS3 helicase (Yao et al., 1997), an SF2 enzyme (DALI Z-score = 14.9 for 224 Cα atoms) than with PcrA helicase (Subramanya et al., 1996), the SF1 enzyme that is most structurally similar to RecQΔC (Z-score = 9.8 for 244 Cα atoms) (Holm and Sander, 1993) (Figure 5). Nevertheless, RecQΔC's similarity with PcrA is still informative. As mentioned above, RecQΔC's mode of ATP binding is quite similar to that seen in PcrA. In addition, a patch of conserved aromatic and charged residues in RecQΔC (residues 156–159, C-terminal to helicase motif II in RecQΔC) map to the same relative surface location as similar residues in PcrA that are used in DNA binding (residues 257–260, C-terminal to motif III in PcrA) (Velankar et al, 1999). This structural conservation between RecQΔC and PcrA could indicate that the enzymes use conserved mechanisms of DNA binding and unwinding. RecQΔC primarily differs from other helicases by its novel accessory elements in the RecQ-Ct domain (Figure 5). These features will most likely prove critical to the specialized functions of RecQ proteins.
Structural basis of Bloom's syndrome missense mutations
Several recessive mutations in the human BLM, WRN, and RECQ4 genes are known to cause Bloom's, Werner's, and Rothmund—Thompson syndromes, respectively. Many of the mutations in BLM and all known disease-associated alleles in WRN and RECQ4 are nonsense or frame-shift mutations that would express truncated versions of the proteins (Kitao et al., 1999). In WRN protein, these mutations lead to mislocalization in the cell due to failure to express the C-terminal nuclear localization sequence (Matsumoto et al., 1997). A similar rationale might also explain the phenotypes of BLM nonsense alleles (Matsumoto et al., 1998). In addition to nonsense and frame-shift mutations, seven missense mutations in BLM leading to single amino acid changes in the protein are known to cause Bloom's syndrome (Ellis et al., 1995; Foucault et al., 1997; Barakat et al., 2000; Rong et al., 2000). Three of these mutations have been shown to inactivate the murine BLM protein in vitro (Bahr et al., 1998), implying that the missense mutations cause disease as a result of enzymatic failure. All seven known disease-linked BLM missense mutations map to the RecQ family catalytic core domain, with five of them occurring in residues identically conserved within the E.coli RecQ sequence. Given the ability of a catalytically active fragment of human BLM protein to complement mutation of the recQ gene in E.coli (Janscak et al., 2003), the RecQΔC structure provides an excellent model for rationalizing the biophysical basis underlying known BLM missense mutations.
Five of the seven BLM missense mutations map to the helicase region of the protein: Gln672Arg, Ile841Thr, Cys878Arg, Gly891Glu, and Cys901Tyr (Ellis et al., 1995; Barakat et al., 2000; Rong et al., 2000). Three of these positions are conserved in RecQΔC (Gln30, Ile192 and Gly239), whereas the two cysteines are poorly conserved among RecQ helicases. The RecQΔC structures reveal plausible effects of these missense mutations that could impair enzyme function. The first mutation, Gln→Arg, would likely diminish ATP binding to RecQ, since the equivalent Gln in RecQΔC (Gln30) contacts the adenine moiety of the nucleotide cofactor directly through hydrogen bonds (Figure 2B). Mutation of this conserved Gln results in loss of ATPase and helicase activity in the murine BLM protein (Bahr et al., 1998), consistent with its observed role in ATP binding. The other BLM helicase mutations are likely to affect protein folding or stability (Figure 2A). Both the Ile→Thr and Gly→Glu mutations introduce polar side chains into the hydrophobic core of the helicase subdomains, which would likely destabilize folded BLM protein and could inactivate the enzyme.
The two remaining disease-linked BLM missense mutations, Cys1036Phe and Cys1055Ser (Ellis et al., 1995; Foucault et al., 1997), alter residues analogous to two that directly bind Zn2+ in RecQΔC (Figure 3A). These mutations introduce either a large hydrophobic group (Phe) or a poor Zn2+ ligand (Ser) into the structure. Either mutation could reduce Zn2+ binding, thus altering the structure of this region of the enzyme. Previous studies have shown that these mutations inactivate the murine BLM protein in vitro (Bahr et al., 1998), thus highlighting the importance of the Zn2+-binding region to proper RecQ family function.
Model for RecQ catalytic function
Using structural information from the RecQΔC structures, we have constructed a general model for RecQ activity. Two likely DNA binding sites are present in RecQΔC: a ssDNA binding site that is similar to those observed in other helicases (Figure 2A), and a putative dsDNA binding site in the RecQ-Ct region (Figure 4C). An arrangement in which the RecQ-Ct region binds dsDNA and ssDNA is bound between the helicase subdomains therefore seems plausible in RecQ (Figure 6). We predict that the 3′ ssDNA end of unwound DNA would be bound to the helicase region, since RecQ proteins unwind dsDNA in a 3′→5′ direction (Umezu et al., 1990). RecQ helicase activity would produce 3′ and 5′ ss segments of unwound DNA as potential substrates for enzymatic partners of RecQ that require ssDNA, such as RecA (Harmon and Kowalczykowski, 1998) or Topo III (Harmon et al., 1999). Moreover, conserved surface features of RecQ, such as the Zn2+-binding subdomain, could provide protein–protein interaction sites or additional DNA binding surfaces. Since our structure is of a monomer of RecQΔC, but full-length E.coli RecQ might function as an oligomer in DNA unwinding (Harmon and Kowalczykowski, 2001), it is not clear whether the ds and ss portions of DNA being unwound by RecQ would bind to the same or different protomers in a RecQ oligomer. In addition, DNA binding could alter the domain arrangement in RecQΔC as has been observed for PcrA helicase (Velankar et al, 1999). Future studies will be required to investigate the structural dynamics associated with DNA binding in E.coli RecQ.
Insights into the nature of RecQ functions with topoisomerase III
Important functional interactions between RecQ and Topo III homologs have been reported for many organisms (reviewed in Wu and Hickson, 2001; Oakley and Hickson, 2002; Wang, 2002), but a model explaining their joint activity has been hampered by the lack of structural information on RecQ. DNA unwinding by a helicase such as RecQ creates domains of (+) and (−) supercoiled DNA (Liu and Wang, 1987; Peter et al., 1998). The ssDNA product from DNA unwinding is a substrate for Topo III, which selectively relaxes (−) supercoiled DNA (DiGate and Marians, 1988). Thus, the net product of RecQ/Topo III activities would likely be (+) supercoiled DNA. As previously proposed, this reaction would constitute a ‘reverse gyrase’ activity (Gangloff et al., 1994). Reverse gyrases have thus far been found only in thermophilic eubacteria and archaea, and they contain both helicase and type-IA topoisomerase domains (reviewed in Champoux, 2001). The RecQΔC structure reveals an important clue as to how RecQ might have evolved to support a reverse gyrase-like activity, since its major subdomains are structurally homologous to the helicase and WH regions of A.fulgidis reverse gyrase (Rodriguez and Stock, 2002). In addition, RecQΔC has a Zn2+-binding domain, an element that is lacking in bacterial and yeast Topo III homologs but present in other type-IA topoisomerases, such as reverse gyrase (Champoux, 2001). We propose that RecQ and Topo III could function together in a manner similar to reverse gyrase using functional domains supplied by both proteins. Interaction between RecQ and Topo III could position Topo III in close proximity to ssDNA produced by the RecQ helicase domain, thereby providing Topo III with substrate. The joint action of RecQ and Topo III may not rely on processive DNA unwinding but could involve a local melting of DNA by RecQ and relaxation by Topo III. This reverse gyrase-like activity could be an important common step in many RecQ-mediated DNA remodeling functions in cells.
The structures of the catalytic core of E.coli RecQ presented here yield insights into the molecular origins of human diseases that stem from mutations of recQ genes and offer new clues that will help elucidate the biochemical mechanisms used by the RecQ family of DNA helicases. These findings help pave the way for uncovering the precise functions of RecQ proteins in cellular genome maintenance reactions.
Materials and methods
Protein expression and purification
T7-overexpression plasmids encoding either full-length E.coli RecQ or RecQΔC (residues 1–523) preceded by a His6 affinity-purification tag were constructed, and the proteins were overexpressed and purified as previously described (Bernstein and Keck, 2003). Selenomethionine-incorporated RecQΔC was expressed as described in Van Duyne et al. (1993), and was purified as for the unsubstituted protein, except that 0.8 mM Tri(2-carboxyethyl) phosphine hydrochloride (TCEP) was added to all buffers, the NaCl concentration of all buffers was adjusted to 500 mM, and the ion exchange purification step was eliminated from the purification procedure.
Crystallization of RecQΔC
Native or selenomethionine-incorporated RecQΔC was dialyzed against buffer containing 10 mM Tris pH 8.0 and 500 mM ammonium acetate. Crystals of native RecQΔC were grown by hanging drop vapor diffusion by mixing 0.9 μl of 20 mg/mL protein, 0.2 μl of 100 mM MnCl2, and 0.9 μl of well solution [0.5% polyethylene glycol (PEG) 1000, 2–4% PEG400, 50 mM MES pH 6.5, 50 mM ammonium sulfate] and equilibrating at room temperature for several days. Crystals measuring ∼200 μm × ∼100 μm × ∼50 μm of symmetry P21 with unit cell length a = 65, b = 54 and c = 78 Å, β = 110.7° were formed. This crystal form has one molecule of RecQΔC per asymmetric unit. Isomorphous selenomethionine-incorporated RecQΔC crystals were grown by microseeding with native crystals. Crystals were stabilized by transferring into a cryoprotectant solution (3% PEG1000, 50 mM HEPES pH 7.5, 10 mM MnCl2, 25% ethylene glycol) and frozen in liquid nitrogen. Crystals with ATPγS bound were obtained by soaking native RecQΔC crystals in 2.5% PEG1000, 50 mM HEPES pH 7.5, 10 mM ATPγS, 5 mM MgCl2, for 3 days at room temperature, and were then transferred to cryoprotectant buffer and frozen in liquid nitrogen.
Molecular replacement solution of nucleotide-bound RecQΔC
The ATPγS/Mn2+-bound RecQΔC structure was solved by molecular replacement using AMORE (Navaza, 2001) with the unbound RecQΔC structure as a search model. The molecular replacement solution was refined with REFMAC/ARP (Lamzin and Wilson, 1993; Murshudov et al., 1997) and by manually rebuilding the model using O (Jones et al., 1991). Since the nucleotide soaking solution contained 5 mM MgCl2 but the cryoprotectant used to stabilize the crystals prior to freezing included 10 mM MnCl2, the identity of the bound metal was ambiguous. We therefore attempted to refine the structure with either a Mg2+ or a Mn2+ ion in the binding site. Placing a Mn2+ ion in the site satisfied the observed scattering, whereas using a Mg2+ ion left substantial positive difference electron density and refined the atomic B-factor of the metal to an unrealistically low value. Therefore, the metal was modeled as a Mn2+ ion. E.coli RecQ has essentially the same level of ATPase activity using either Mg2+ or Mn2+ as a cofactor (Umezu et al., 1990). The final model contains residues 1–516 excluding residues 296–299 for which electron density was not observed. No bond angles for this model fall into disallowed regions of Ramachandrian space.
Quantitation of Zn2+ bound to E.coli RecQ
The Zn2+ content of purified full-length E.coli RecQ was measured using 4-(2-pyridylazo)resorcinol (PAR), a reporter dye that absorbs light at 490 nm when bound to Zn2+ (Hunt et al., 1984). Zn2+ was extracted from a sample of purified RecQ by dialysis against 20 mM Tris pH 8.0, 300 mM NaCl, 10% glycerol, 10 mM EDTA, 1 mM DTT, at 4°C overnight. One hundred microliters of untreated RecQ or Zn2+-extracted RecQ (in 10% glycerol, 300 mM NaCl, 20 mM Tris–HCl pH 8.0) was incubated with 60 μg Proteinase K at 37°C for 1 h. Two microliters of 5 mM PAR was then added to each sample and their absorbances at 490 nm were measured and compared to a standard curve of ZnCl2 samples at a range of concentrations using an identical sample preparation procedure as described above, but omitting RecQ. RecQ concentrations were determined as in Bernstein and Keck, (2003).
Quantitation of free thiol groups in E.coli RecQ
[thiolsfree] in E.coli RecQ and Zn2+-extracted RecQ were determined by measuring the absorbance at 412 nm following reaction of 5,5′-dithiobis (2-nitrobenzoic acid) (DTNB) with thiols in the protein as described in Riddles et al. (1983). Ten microliters of 10 mM DTNB (in 0.1 M NaPhosphate pH 8.0) was added to 10 μl of untreated or Zn2+-extracted E.coli RecQ (in 10% glycerol, 300 mM NaCl, 20 mM Tris–HCl pH 8.0) and diluted into 300 μl of 0.1 M NaPhosphate pH 8.0. Samples were incubated at room temperature for 1 h and their absorbances at 412 nm were measured. These values were converted to [thiolsfree] as described in Riddles et al. (1983).
Model coordinates and structure factors have been deposited in the Protein Data Bank under accession codes 1OYW and 1OYY.
We thank James Holton (Advanced Light Source beamline 8.3.1) and the Advanced Photon Source beamline staff (BioCARS beamline 14-BMC) for assistance in data collection, and Bruker AXS for generous use of their instrumentation. R.J.Bennett, J.M.Berger, D.A.Brow, E.A.Craig, J.E.Dahlberg and E.Shor contributed helpful discussions. This work was supported by a grant from the NIH to J.L.K. (GM068061), start-up funds from the University of Wisconsin, and a grant from the University of Wisconsin Medical School under the Howard Hughes Medical Institute Research Resources Program for Medical Schools. D.A.B. was supported in part by an NIH training grant in Molecular Biophysics (GM08293).