|Home | About | Journals | Submit | Contact Us | Français|
Human topoisomerase IIα utilizes a two-metal-ion mechanism for DNA cleavage. One of the metal ions (M12+) is believed to make a critical interaction with the 3′-bridging atom of the scissile phosphate, while the other (M22+) is believed to interact with a non-bridging oxygen of the scissile phosphate. Based on structural and mutagenesis studies of prokaryotic nucleic acid enzymes, it has been proposed that the active site divalent metal ions interact with type II topoisomerases through a series of conserved acidic amino acid residues. The homologous residues in human topoisomerase IIα are E461, D541, D543, and D545. To address the validity of these assignments and to delineate interactions between individual amino acids and M12+ and M22+, we individually mutated each of these acidic amino acid residues in topoisomerase IIα to either cysteine or alanine. Mutant enzymes displayed a marked loss of catalytic and DNA cleavage activity as well as a reduced affinity for divalent metal ions. Additional experiments determined the ability of wild-type and mutant topoisomerase IIα enzymes to cleave an oligonucleotide substrate that contained a sulfur atom in place of the 3′-bridging oxygen of the scissile phosphate in the presence of Mg2+, Mn2+, or Ca2+. Based on the results of these studies, we conclude that the four acidic amino acid residues interact with metal ions in the DNA cleavage/ligation active site of topoisomerase IIα. Furthermore, we propose that M12+ interacts with E461, D543, and D545 and M22+ interacts with E461 and D541.
Fundamental nuclear processes, such as replication and recombination, often generate tangles and knots in DNA (1–3). If these topological alterations in the genetic material are not successfully resolved, the ability of chromosomes to segregate during mitosis will be severely impeded (2–5).
DNA tangles and knots are removed by type II topoisomerases (2, 4, 6–9). These essential enzymes act by generating transient double-stranded breaks in DNA and passing an intact double helix through the break (4, 10). Like many enzymes that break or rejoin nucleic acids, type II topoisomerases require divalent metal ions as cofactors for catalysis (11). Magnesium appears to be the physiological metal ion used by these enzymes (11). Recent studies indicate that human topoisomerase IIα and IIβ both utilize a two-metal-ion mechanism for DNA cleavage (12, 13). This mechanism is similar to those proposed for the scission reaction of DNA gyrase (a bacterial type II topoisomerase) (14) as well as the polymerization reactions of primases and some DNA polymerases (15–17).
During the DNA cleavage reaction of topoisomerase IIα and IIβ, one divalent metal ion (metal ion 1) makes an important interaction with the 3′-bridging oxygen atom of the scissile phosphate (12, 13). This interaction accelerates rates of enzyme-mediated DNA scission, most likely by stabilizing the leaving group (12–14). A second metal ion (metal ion 2) appears to contact a non-bridging atom of the scissile phosphate in the active site of topoisomerase IIβ (13). This interaction plays a significant role in DNA cleavage mediated by the β isoform and greatly stimulates scission. As proposed previously, metal ion 2 is believed to stabilize the DNA transition state and/or help deprotonate the active site tyrosine (12–14, 18). Although topoisomerase IIα has an absolute requirement for metal ion 2 (12), the role of this divalent cation in its DNA cleavage reaction is unclear. It is not definitive as to whether it interacts with a non-bridging oxygen in the active site of topoisomerase IIα. However, if the interaction exists, it does not affect rates of DNA cleavage.
Type IA topoisomerases, type II topoisomerases, and primases share a conserved region known as the TOPRIM domain (19, 20). This region has been implicated in coordinating divalent metal ions that are used during nucleic acid cleavage, ligation, and polymerization reactions (14, 19–21). Based on structural studies of Escherichia coli topoisomerase III, primase (dnaG), and DNA gyrase, together with mutagenesis studies of DNA gyrase, it has been proposed that the divalent metal ions in the active sites of type II topoisomerases interact with the protein through a series of conserved acidic amino acid residues (Figure 1) (14, 18, 19, 22). The homologous residues in human topoisomerase IIα are E461, D541, D543, and D545 (23). These assignments are consistent with a recent crystallographic structure of the catalytic core of yeast topoisomerase II in a non-covalent complex with DNA (24). However, this latter structure contained only one divalent metal ion and the active site tyrosine residue was located too far from the scissile bond to support DNA cleavage. Thus, specific interactions between individual amino acids and the two divalent metal ions in the DNA cleavage/ligation active site of type II topoisomerases have yet to be fully elucidated.
In an effort to more completely define interactions between divalent metal ions and type II topoisomerases, we carried out a series of kinetic and mutagenesis studies with topoisomerase IIα. Results confirm an important role for E461, D541, D543, and D545 in DNA cleavage mediated by the human enzyme and delineate contacts between individual amino acid residues and metal ions 1 and 2.
Wild-type and mutant human topoisomerase IIα proteins were expressed in Saccharomyces cerevisiae JEL1Δtop1 cells and purified as described previously (25–27). Individual point mutations in human topoisomerase IIα were generated using the PCR-based Lightning Mutagenesis Kit (Strategene). D541, D543, D545, and E461 were individually mutated to either Cys or Ala in the inducible overexpression YEpWOB6 plasmid. Primer sequences were as follows: D545C forward 5′ – GGAAGATAATGATTATGACAGATCAGGACCAATGTGGTTCCCACATC – 3′; reverse 5′ – GATGTGGGAACCACATTGGTCCTGATCTGTCATAATCATTATCTTCC – 3′; D545A forward 5′ – GGAAGATAATGATTATGACAGATCAGGACCAAGCTGGTTCCCACATC – 3′; reverse 5′ – GATGTGGGAACCAGCTTGGTCCTGATCTGTCATAATCATTATCTTCC – 3′; D543C forward 5′ – GGAAGATAATGATTATGACAGATCAGTGCCAAGATGGTTCCCACATC – 3′; reverse 5′ – GATGTGGGAACCATCTTGGCACTGATCTGTCATAATCATTATCTTCC – 3′; D543A forward 5′ – GGAAGATAAGATTATGACAGATCAGGCCCAAGATGGTTCCCACATC – 3′; reverse 5′ – GATGTGGGAACCATCTTGGGCCTGATCTGTCATAATCATTATCTTCC – 3′; D541C forward 5′ – GGAAGATAATGATTATGACATGTCAGGACCAAGATGGTTCCCACATC – 3′; reverse 5′ – GATGTGGGAACCATCTTGGTCCTGACATGTCATAATCATTATCTTCC – 3′; D541A forward 5′ – GGAAGATAATGATTATGACAGCTCAGGACCAAGATGGTTCCCACATC – 3′; reverse 5′ – GATGTGGGAACCATCTTGGTCCTGAGCTGTCATAA TCATTATCTTCC – 3′; E461C forward 5′ – GAGTGTACGCTTATCCTGACTTGTGGAGATTCAGCCAAAACTTTGGCTG – 3′; reverse 5′ – CAGCCAAAGTTTTGGCTGAATCTCCACAAGTCAGGATAAGCGTACACTC – 3′; and E461A forward 5′ – GAGTGTACGCTTATCCTGACTGCGGGAGATTCAGCCAAAACTTTGGCTG – 3′; reverse 5′ – CAGCCAAAGTTTTGGCTGAATCTCCCGCAGTCAGGATAAGCGTACACTC – 3′. In all cases, mutant topoisomerase IIα genes were isolated and sequenced before being transformed into JEL1Δtop1 yeast cells. The purity of mutant enzymes was assessed by polyacrylamide gel electrophoresis. Proteins were visualized with coomassie or silver stains (data not shown). Enzymes were >95% homogeneous. Contamination with yeast topoisomerase II was too low to quantify (<0.2%), as determined by western blot analysis using antibodies directed against the yeast type II enzyme.
A 50 bp duplex oligonucleotide was designed using a previously identified topoisomerase II cleavage site from pBR322 (28). Wild-type oligonucleotide sequences were generated using an Applied Biosystems DNA synthesizer. The 50-mer top and bottom sequences were 5′-TTGGTATCTGCGCTCTGCTGAAGCC↓AGTTACCTTCGGAAAAAGAGTTGGT-3′ and 5′-ACCAACTCTTTTTCCGAAGGT↓AACTGGCTTCAGCAGAGCGCAGATACCAA-3′, respectively. The arrow denotes the point of scission by topoisomerase II. The top strand was composed of two shorter sequences that produced a nick at the location of the scissile bond.
DNA containing a single 3′-bridging phosphorothiolate linkage was synthesized as described previously (29). The location of the phosphorothiolate was at the normal scissile bond on the bottom strand. Substrates containing a racemic phosphorothioate in place of the non-bridging scissile bond oxygens of the bottom strand were synthesized by Operon.
[γ-32P]ATP (~5000 Ci/mmol) was obtained from ICN. Single-stranded oligonucleotides were labeled on their 5′-termini using T4 polynucleotide kinase (New England Biolabs). Following labeling and gel purification, complementary oligonucleotides were annealed by incubation at 70 °C for 10 min and cooling to 25 °C.
DNA cleavage assays were carried out by the procedure of Deweese et al. (29). DNA cleavage reactions with wild-type or mutant human topoisomerase IIα proteins contained 200 nM enzyme and 100 nM double-stranded oligonucleotide in a total of 10 μL of DNA cleavage buffer [10 mM Tris-HCl, pH 7.9, 135 mM KCl, 0.1 mM EDTA, and 2.5% glycerol]. Unless otherwise noted, the concentration of the divalent cation added to reaction mixtures was 5 mM. In some cases, the concentration of divalent cation (MgCl2, MnCl2, or CaCl2) was varied and/or combinations of the cations were used. Experiments that monitored DNA cleavage over a range that included divalent cation concentrations below 1 mM utilized cleavage buffer that lacked EDTA. Reactions were initiated by the addition of enzyme and were incubated for 0 to 30 min at 37 °C. DNA cleavage products were trapped by the addition of 2 μL of 10% SDS followed by 2 μL of 250 mM NaEDTA, pH 8.0. Proteinase K (2 μL of 0.8 mg/mL) was added to digest the enzyme. Cleavage products were resolved by electrophoresis in a 14% denaturing polyacrylamide gel. To inhibit oxidation of cleaved oligonucleotides containing 3′-terminal –SH moieties and the formation of multimers in the gel, 100 mM DTT was added to the sample loading buffer. DNA cleavage products were visualized and quantified using a Bio-Rad Molecular Imager.
Pre-equilibrium DNA cleavage reactions were monitored for 0.5 s to 3 s using a KinTek model RQF-3 chemical quench flow apparatus (Austin, TX). Cleavage was initiated by rapidly mixing two independent solutions. The first contained a noncovalent complex formed between human topoisomerase IIα and 32P-labeled oligonucleotide in cleavage buffer that lacked divalent cation. The second solution contained cleavage buffer in which the concentration of MgCl2 was 2 times higher than normal (concentration of MgCl2 in the final reaction mixture ranged from 0.5–10 mM). The two solutions were mixed at 37 °C, and DNA cleavage was quenched with 1% SDS (v/v final concentration). Products were processed and analyzed as described above.
Pre-steady-state data were fitted using the program DynaFit (30). Best fits were obtained for plots of time courses versus metal ion concentration using least-squares regression by Levenberg-Marquardt methods. The full analysis is included in Supporting Information.
DNA relaxation assays were performed according to the procedure of McClendon et al. (31). Reactions mixtures contained 0.5–20 nM wild-type or 20 nM mutant human topoisomerase IIα proteins, 1 mM ATP, and 5 nM negatively supercoiled pBR322 in a total of 20 μL of 10 mM Tris-HCL, pH 7.9, 175 mM KCl, 5 mM MgCl2, 0.1 mM NaEDTA, and 2.5% glycerol. Mixtures were incubated at 37 °C for 0–20 min and stopped by the addition of 3 μL of 0.5% SDS and 77 mM EDTA. Samples were mixed with 2 μL of agarose gel loading buffer [60% sucrose in 10 mM Tris-HCl (pH 7.9), 0.5% bromophenol blue (w/v), and 0.5% xylene cyanol FF (w/v)] and subjected to electrophoresis in 1% agarose gels in 100 mM Tris-borate, pH 8.3, and 2 mM EDTA. Gels were stained for 30 min with 0.5 μg/mL ethidium bromide. DNA bands were visualized by UV light and were quantified using an Alpha Innotech digital imaging system (San Leandro, CA). DNA relaxation was monitored by the loss of the initial supercoiled substrate.
Plasmid DNA cleavage reactions were performed using the procedure of Fortune and Osheroff (32). Reaction mixtures contained 200 nM wild-type or mutant human topoisomerase II proteins and 5 nM negatively supercoiled pBR322 DNA in 20 μL of DNA cleavage buffer containing 5 mM MgCl2 and 100 μM etoposide or amsacrine. DNA cleavage mixtures were incubated for 6 min at 37 °C. DNA cleavage complexes were trapped by adding 2 μL of 5% SDS followed by 2 μL of 250 mM Na2EDTA (pH 8.0). Proteinase K was added (2 μL of a 0.8 mg/mL solution), and reaction mixtures were incubated for 30 min at 37 °C to digest topoisomerase II. Samples were mixed with 2 μL of agarose gel loading buffer, heated for 2 min at 45 °C, and subjected to electrophoresis in 1% agarose gels in 40 mM Tris-acetate (pH 8.3) and 2 mM EDTA containing 0.5 μg/mL ethidium bromide. Double-stranded DNA cleavage was monitored by the conversion of negatively supercoiled plasmid DNA to linear molecules. DNA bands were visualized and quantified as described above.
As discussed earlier, human topoisomerase IIα utilizes a two-metal-ion mechanism for its DNA scission reaction. Based on the relative abilities of Mn2+ and Ca2+ to support cleavage of wild-type oligonucleotides and substrates containing 3′-bridging phosphorothiolates, it was proposed that metal ion 1 bound to topoisomerase IIα with an affinity that was ~10–fold higher than that of metal ion 2 (12). However, the interaction of the physiological metal ion, Mg2+, with topoisomerase IIα has not been explored in detail. Therefore, a kinetic approach was employed to further define the parameters of Mg2+ utilization by topoisomerase IIα.
As a first step, the cleavage of a wild-type substrate was determined over a Mg2+ concentration range of 1 μM to 10 mM (Figure 2). To simplify the analysis and increase baseline levels of scission, we used a substrate that contained a nick at the scissile bond of the unlabeled strand (12). Previous work has demonstrated that the presence of the nick enhances both the rate and level of DNA cleavage on the opposite strand (12, 33).
Optimal DNA cleavage was observed at ~2.5–5.0 mM Mg2+. The decrease in enzyme activity at higher metal ion concentrations has been observed for other type II topoisomerases and most likely represents an ionic strength effect (36).
At the low end of the Mg2+ concentration range, the dependence of the metal ion appeared to be biphasic in nature. This biphasic metal ion concentration dependence suggests that there are two Mg2+ sites in the DNA cleavage/ligation domain of topoisomerase IIα and that both need to be filled in order to support scission. The initial (i.e., high affinity) phase appears to be completely filled somewhere between ~100–250 μM Mg2+, implying an apparent KD value for this site that probably is less than 100 μM. Based on the results of previous studies (12, 13), we propose that this high affinity interaction represents the binding of Mg2+ to the site of metal ion 1. One-half maximal DNA cleavage activity was observed at ~1.0–1.5 mM Mg2+. This finding suggests that Mg2+ binds to the site of metal ion 2 with an apparent KD value that is in this latter concentration range. By comparison, the concentration of free Mg2+ within the cell is estimated to be ~0.5–1.5 mM (34).
To extend the above experiments, the intrinsic KD value of human topoisomerase IIα for Mg2+ was determined by analyzing the metal ion dependence of the pre-equilibrium kinetics of enzyme-mediated DNA cleavage. Experiments utilized a Mg2+ concentration range of 0.5–10 mM. Since both metal ions 1 and 2 must be present in order to support DNA cleavage, we started at a concentration at which the first metal ion binding site was likely to be saturated. Thus, data from the kinetic analysis reflect primarily the interaction of Mg2+ with the second, or low affinity, metal ion binding site. In addition, since the substrate used for these studies contained a nick at the scissile bond on the unlabeled strand, the enzyme can cleave only the scissile bond on the labeled strand. As a result, the overall equation describing the reaction being monitored is reduced to the following:
Plots of percent DNA cleavage versus cation concentration were fitted to a single-exponential equation to generate apparent rate constants for the reaction at each concentration. Apparent rate constants were then plotted versus cation concentration (Figure 3) and analyzed using the program DynaFit (30).
The analysis was performed using a series of values for the forward cleavage (k2) and reverse ligation (k−2) reaction rates. In all cases, best fits were obtained at k−2/k2 ratios in the range of ~40–500, implying that topoisomerase IIα ligates DNA considerably faster than it cleaves the double helix. This finding is consistent with the fact that the human type II enzyme maintains very low equilibrium levels of covalent enzyme-cleaved DNA complexes (E•DNA*•Metal) (4, 10, 33, 35).
Finally, over a wide range of k1 and k−1, best fits always yielded a k−1/k1 ratio (i.e., KD value) of ~1.2 mM. This apparent KD for the binding of Mg2+ to the second metal ion site is similar to the value obtained in the equilibrium titration experiment discussed above.
Based on crystallographic and mutagenesis studies with bacterial topoisomerases and primase, it has been proposed that divalent metal ions are coordinated to human topoisomerase IIα through a series of acidic amino acid residues (see Figure 1) (12, 14, 18–22). Metal ion 1 is postulated to interact with E461, D543, and D545, while metal ion 2 is postulated to interact with E461 and D541 (12). These residues are highly conserved among the type IA and type IIA families of topoisomerases (19, 21, 23).
To address the validity of these assignments in human topoisomerase IIα, the four acidic amino acids were individually mutated to either Ala (to remove functional groups) or Cys (to potentially enhance interactions with thiophilic divalent metal ions). Each of the mutant enzymes was purified and characterized. As seen in Figure 4, the overall catalytic activity of the mutant enzymes, assessed by the ability to relax negatively supercoiled plasmid DNA in the presence of 5 mM Mg2+, was dramatically reduced as compared to that of the wild-type enzyme. Even the most active of the mutant enzymes, hTop2αD541C, required 10– to 20–fold higher enzyme concentrations than wild-type topoisomerase IIα to achieve similar rates of DNA relaxation. The least active mutant enzyme, hTop2αE461A, required >40–fold higher concentrations.
In order to examine the roles of the acidic amino acids in coordinating divalent metal ions during the scission reaction, the ability of the mutant enzymes to cleave negatively supercoiled DNA in the presence of 5 mM Mg2+ was determined. Equilibrium levels of cleavage generated by the mutant enzymes were too low to quantify reliably. Therefore, cleavage experiments were carried out in the presence of either 100 μM etoposide or amsacrine. Both of these anticancer drugs are potent topoisomerase II poisons that increase levels of enzyme-mediated DNA scission by interfering with the ability of topoisomerase II to ligate cleaved molecules. Once again, all of the mutant enzymes displayed a level of activity that was considerably lower than that of wild-type topoisomerase IIα (Figure 5). Together with the DNA relaxation results, these findings provide strong evidence that E461, D541, D543, and D545 play important roles in catalysis mediated by human topoisomerase IIα.
In addition to the requirement for divalent metal ions in the DNA cleavage/ligation active site of type II topoisomerases, these enzymes also utilize a divalent metal to coordinate the high energy ATP cofactor in a separate ATPase active site (36). To ensure that the mutations affected metal ion coordination only in the cleavage/ligation active site, the ability of two mutant enzymes to hydrolyze ATP in absence of DNA was determined using a thin layer chromatography technique (37). hTop2αE461C and hTop2αD543C were chosen for this study because they represent one of the least active and one of the most active mutants, respectively. Despite the fact that both mutant enzymes displayed a relaxation activity that was less than 5% that of wild-type, rates of ATP hydrolysis were ~70% and 200% that of wild-type topoisomerase IIα (data not shown). Since the effects of the mutations on ATPase activity did not reflect their effects on DNA relaxation, it is concluded that the primary defect in the enzymes is their inability to cleave DNA efficiently.
In an effort to delineate interactions between specific amino acid residues and metal ions 1 and 2, the ability of wild-type topoisomerase IIα and the mutant enzymes to cleave a series of oligonucleotides was assessed. Three different substrates were employed for these experiments. All had the same nucleotide sequence. However, one contained a wild-type 3′-bridging oxygen at the scissile bond, while the other two substituted a sulfur atom at either the non-bridging (phosphorothioate) or 3′-bridging (phosphorothiolate) position. In addition to the different substrates, DNA cleavage was determined in the presence of 5 mM Mg2+, Mn2+, or Ca2+. Within this series, Mn2+ is the “softest,” or most thiophilic metal, and Mg2+ and Ca2+ are harder, or less thiophilic (38–40). Soft metal ions often prefer sulfur over oxygen as an inner-sphere ligand, while hard metals usually coordinate more readily with oxygen (16, 38–43). If there is a direct interaction between the metal ion and a scissile phosphate atom (or a sulfur-containing amino acid) that facilitates catalysis, relative levels or rates of scission with substrates containing a sulfur atom in place of the oxygen should increase in the presence of soft (thiophilic) metals (12, 16, 41–43). Conversely, less cleavage should be generated in reactions that contain hard metals (12, 16, 41–43).
As seen in Figure 6 (Top), compared to wild-type human topoisomerase IIα, levels of cleavage of the wild-type substrate were dramatically reduced for all of the mutant enzymes. Mutations at D545 and E461 resulted in enzymes that displayed almost no cleavage activity, while marginal levels of cleavage were observed with the D543 and D541 mutant enzymes. It is notable that hTop2αD541C and hTop2αD543C, which among the D->C mutations displayed the greatest ability to cleave DNA in the presence of Mg2+, also displayed the greatest ability to relax plasmid DNA in the presence of Mg2+. However, a similar correlation was not observed among the D->A mutations.
In all cases, poor activity was seen with the substrate that contained the non-bridging phosphorothioate (Figure 6 Middle). This is consistent with the previous finding that this substrate generally is cleaved more poorly than wild-type oligonucleotides.
Unlike the other substrates, oligonucleotides that contain a 3′-bridging phosphorothiolate cannot be ligated appreciably by topoisomerase IIα (29). As a result, much higher levels of cleavage complexes accumulate with this substrate. This property provides a more sensitive assay to determine the ability of a given enzyme to cleave DNA.
As observed with the wild-type and non-bridging phosphorothioate oligonucleotides, hTop2αE461C and hTop2αE461A displayed virtually no ability to cleave the 3′-bridging phosphorothiolate substrate (Figures 6 Bottom, 7, and 8). This finding is consistent with the proposal that E461 plays an important role in coordinating both metal ions 1 and 2. However, in contrast to the E461 mutants, modest to high levels of DNA scission were generated by most of the aspartic acid mutants (Figures 6 Bottom, 7, and 8). In all cases, higher levels and rates of cleavage were observed in the D->C than in the D->A mutants when Mn2+ was employed as the divalent metal ion. Since Mn2+ is a thiophilic metal ion, this finding implies a direct interaction between divalent cations and D541, D543, and D545.
hTop2αD545C and hTop2αD545A cleaved the 3′-bridging phosphorothiolate, but did so only in the presence of Mn2+. The fact that the DNA cleavage activity of the D545 mutants can be rescued only in the presence of a thiophilic metal ion and an S–P scissile bond strongly suggests that this residue coordinates metal ion 1, as predicted by the two-metal ion model for topoisomerase IIα. As determined by the metal ion concentration required to yield ½ maximal DNA cleavage, hTop2αD545C and hTop2αD545A displayed reduced affinities for Mn2+ [apparent KD ≈ 2.5 mM for each mutant as compared to ~14 μM for the wild-type enzyme (Figure 7)] and decreased rates of cleavage [rate ≈ 1000-fold lower than that of the wild-type enzyme (Figure 8)].
hTop2αD543C and hTop2αD543A cleaved the phosphorothiolate substrate in the presence of all three metal ions (Mg2+, Mn2+, or Ca2+). However, the highest levels of scission always were observed with Mn2+, the most thiophilic metal ion of the three. Once again, these data support the proposed interaction of D543 with metal ion 1. As above, hTop2αD543C and hTop2αD543A displayed decreased affinities for Mn2+ [apparent KD ≈ 20 μM and 140 μM, respectively (Figure 7)] and decreased rates of cleavage [rates ≈ 2- and 40-fold lower than that of the wild-type enzyme, respectively (Figure 8)].
The interpretation of results with hTop2αD541C and hTop2αD541A is less straightforward. The two-metal-ion mechanism predicts that D541 interacts with metal ion 2. The finding that hTop2αD541A cannot be rescued more than a few percent by any of the divalent metal ions (Figures 6 Bottom, 7, and 8) is consistent with this postulate. hTop2αD541C is, however, rescued by Mn2+, but not by the other two divalent cations. As above, the affinity of Mn2+ (apparent KD ≈ 34 μM, Figure 7) and rates of DNA cleavage (rate ≈ 10-fold lower than that of the wild-type enzyme, Figure 8) were reduced as compared to topoisomerase IIα. The fact that the cleavage activity of the 3′-bridging S–P bond is seen only in the presence of a thiophilic metal ion could imply that D541 coordinates with metal ion 1 rather than 2. However, if this latter interpretation were correct, it is likely that hTop2αD541A would also support DNA cleavage in the presence of Mn2+, as observed for hTop2αD545A and hTop2αD543A. Therefore, an alternative and more likely explanation for the Mn2+-specific activity of hTop2αD541C is that D541 binds metal ion 2, and the –SH group of the cysteine (which is not present in the D->A mutation) rather than the S–P scissile bond coordinates the metal ion. Further experimentation will be necessary to resolve this issue more fully.
Topoisomerase IIα utilizes two metal ions to support its DNA cleavage activity. This was demonstrated by experiments that compared levels of DNA cleavage monitored in the presence of Ca2+, Mn2+, or a combination of the two divalent metal ions (12). Near saturating concentrations of Ca2+ were paired with sub-saturating concentrations of Mn2+. Rates of scission of a 3′-bridging phosphorothiolate substrate generated by wild-type topoisomerase IIα in the presence of both cations were >10–fold higher than predicted by the arithmetic sum of cleavage seen when either individual metal ion was employed (12).
Similar experiments were carried out with two mutant enzymes, hTop2αD543C and hTop2αD541C. These two enzymes were chosen because both supported high levels of DNA scission with the 3′-bridging phosphorothiolate in the presence of Mn2+. Results are shown in Figure 9. In both cases, there was a greater than predicted effect of the two metal ions on DNA cleavage. Therefore, it appears that the mutant enzymes still employ a two-metal-ion mechanism for topoisomerase II-mediated DNA cleavage.
It is notable that the two-metal-ion enhancement of DNA scission with hTop2αD543C and hTop2αD541C was not as great as observed with the wild-type enzyme. This finding is consistent with the fact that neither mutant enzyme is able to utilize Ca2+ nearly as well as wild-type topoisomerase IIα. Consequently, the effect of the two metal ions, while present, is reduced.
Based on previous structural, mutagenesis, and kinetic studies, it has been proposed that human type II topoisomerases utilize a two-metal ion mechanism for their DNA cleavage reaction (Figure 10) (12–14). In this model, there is an important interaction between metal ion 1 and the 3′-bridging atom of the scissile phosphate that accelerates rates of enzyme-mediated DNA cleavage. There also appears to be an interaction between metal ion 2 and a non-bridging oxygen of the scissile phosphate. This interaction plays a significant role in DNA cleavage mediated by topoisomerase IIβ (13). Although topoisomerase IIα has an absolute requirement for metal ion 2, the proposed interaction with the non-bridging oxygen has only a modest effect on rates of DNA cleavage.
Previous studies have predicted an interaction between several acidic amino acid residues and the metal ions in type II topoisomerases. Mutagenesis studies have confirmed the importance of some of these residues in the bacterial type II enzyme, DNA gyrase, and in human topoisomerase IIβ (14, 22). However, the importance of the homologous residues in human topoisomerase IIα (E461, D541, D543, and D545) had not been demonstrated. In addition, while interactions between specific amino acid residues and metal ions 1 and 2 have been proposed, assignments have not been validated by enzymological studies for any type II enzyme.
Experiments were carried out that monitored DNA relaxation and cleavage (levels, rates, and metal ion concentration dependence) by mutant enzymes in which four acidic amino acid residues were individually converted to either a cysteine or an alanine. Results of these studies confirm the importance of E461, D541, D543, and D545 for the activity of human topoisomerase IIα and strongly suggest that each plays a role in metal ion binding. Furthermore, we propose that D543 and D545 play an important role in coordinating metal ion 1, that D541 plays an important role in coordinating metal ion 2, and that E461 plays an important role in coordinating both metal ions. The present study refines the two-metal-ion model for human topoisomerase II and provides a better-developed platform for additional studies regarding the role of metal ions in topoisomerase II-mediated processes.
We thank Jo Ann Byl for helpful discussions regarding the preparation of mutant enzymes and ATP hydrolysis. We are grateful to Amanda C. Gentry, Adam C. Ketron, and Steven L. Pitts for critical reading of the manuscript. We thank Dr. Robert Eoff for instrument training and helpful discussions regarding rapid quench kinetics.
†This work was supported by National Institutes of Health research grants GM33944 and GM53960. JED was a trainee under grant T32 CA09592 from the National Institutes of Health.
SUPPORTING INFORMATION AVAILABLE