Print version ISSN 0103-5053
On-line version ISSN 1678-4790
J. Braz. Chem. Soc. vol.17 no.8 São Paulo Nov./Dec. 2006
Tristan W. Elliott; Nataa Miti; Lawrence R. Gahan; Luke W. Guddat; Gerhard Schenk*
School of Molecular and Microbial Sciences, The University of Queensland, St. Lucia, QLD 4072, Australia
Purple acid phosphatases (PAPs) belong to the family of binuclear metallohydrolases and catalyse the hydrolysis of a large group of phosphoester substrates at acidic pH. Despite structural conservation in their active sites PAPs appear to display mechanistic versatility. Here, aspects of the catalytic mechanism of two PAPs are investigated using the inhibitors vanadate and fluoride as probes. While the magnitude of their vanadate inhibition constants are similar the two enzymes differ with respect to the mode of inhibition; vanadate interacts in a non-competitive fashion with pig PAP (Ki = 40 µmol L-1) while it inhibits red kidney bean PAP competitively (Ki = 30 µmol L-1). Similarly, fluoride also acts as a competitive inhibitor for red kidney bean PAP, independent of pH, while the inhibition of pig PAP by fluoride is uncompetitive at low pH and non-competitive at higher pH, independent of metal ion composition. Furthermore, while fluoride acts as a slow-binding inhibitor in pig PAP it binds rapidly to the catalytic site of the red kidney bean enzyme. Since vanadate and fluoride are proposed to act as transition state and nucleophile mimics, respectively, the observed differences in inhibition kinetics indicate subtle but distinct variations in the reaction mechanism of these enzymes.
Keywords: purple acid phosphatase, catalytic mechanism, kinetics, enzyme inhibition
Fosfatases ácidas púrpuras (PAP) pertencem à família das metalo-hidrolases binucleares que catalisam a hidrólise de um grande grupo de substratos fosfoésteres em pH ácido. Apesar dos seus sítios ativos serem estruturamente conservados as PAP apresentam versatilidade mecanística. Neste trabalho são investigados alguns aspectos do mecanismo catalítico de duas PAP, usando os inibidores vanadato e fluoreto como sondas. Enquanto as magnitudes das constantes de inibição das duas enzimas pelo vanadato são semelhantes, as enzimas diferem com relação ao modo de inibição; vanadato interage de forma não-competitiva com a PAP de porco (Ki = 40 µmol L-1), porém inibe a PAP de feijão competitivamente (Ki = 30 µmol L-1). De modo semelhante, o fluoreto também age como inibidor competitivo da PAP de feijão, independentemente do pH, enquanto que o fluoreto simplesmente interage com o complexo formado pela enzima de porco e seu substrato(PAP-substrato) em pH baixo e inibe de forma não competitiva esta enzima em pH mais alto, independentemente da composição do íon metálico. Além disso, enquanto a inibição pelo fluoreto se dá através da interação lenta com a PAP de porco, ele se liga rapidamente ao sítio catalítico da enzima do feijão. Visto que se propõe que o vanadato e o fluoreto mimetizem o estado de transição e o nucleófilo, respectivamente, as diferenças observadas na cinética de inibição indicam sutis, porém distintas diferenças no mecanismo de reação destas enzimas.
Purple acid phosphatases (PAPs) belong to the family of binuclear metallohydrolases, with members differing widely with respect to physicochemical properties, tissue localisation and proposed biological function.1,2 The characteristic purple colour of these enzymes is due to a charge transfer transition between a ligand (tyrosinate) donor orbital and an acceptor orbital on the ferric ion.1,3,4 PAPs catalyse the hydrolysis of a variety of phosphorylated substrates at acidic to neutral pH, and have been identified in, and characterised from animal, plant and fungal sources.5-8 The enzyme extracted from mammalian organisms is a 35 kDa monomer and contains a redox-active FeIII-FeIII/II centre.9 In contrast, plant PAPs are homodimeric with a molecular mass of 110 kDa and redox-inactive FeIII-ZnII or FeIII-MnII centres.10-12
Plant and mammalian PAPs have very similar geometries at the catalytically relevant active site with all seven metal ion-coordinating residues being invariant.1,6,13-18 Additional residues that play important roles in various aspects of catalysis are also well conserved, including the proposed proton donor to the leaving group (His296 and His195 in red kidney bean and pig PAP, respectively).13-18 The observations that PAPs from different organisms have similar Km values for a variety of substrates and are inhibited to a similar extent by inorganic phosphate also illustrate the structural similarity of the active sites of different PAPs.10,11,19-21
The inhibition of reactivity by a range of antagonists is a common method to investigate an enzyme's catalytic mechanism; additionally such a study may provide valuable information and guidance for the design and development of specific and potent drugs. PAPs from mammalian organisms have been shown to play an integral part in bone metabolism, and an increase in PAP activity is directly linked to osteoporosis,5,22 making this enzyme a major target for the development of anti-osteoporotic chemotherapeutics.21 For metallohydrolases, fluoride and vanadate are known inhibitors which have been shown to coordinate directly to the metal ion(s) in the active site and thus interfere with catalytic turnover.1,20,23-28 The two inhibitors are likely to affect different aspects of catalysis and hence may provide insight into different steps of the reaction mechanism.
The ability of fluoride to readily replace nucleophilic hydroxide groups can provide (i) an insight into the number of labile water/hydroxide binding sites in the active site, and (ii) the role of the terminally bound or bridging hydroxides in the reaction mechanism.26,29 Fluoride, a well established osteogenic agent which promotes osteoblastic proliferation and differentiation at clinically relevant concentrations, inhibits animal PAPs in a pH-dependent manner. The mode of inhibition of the FeZn derivative of bovine spleen PAP changes from uncompetitive at pH 5.0 (Kiuc = 0.2 mmol L-1) to non-competitive at pH 6.5 (Kiuc » 2 mmol L-1; Kic » 3.4 mmol L-1).24 In contrast, for human PAP it has recently been shown that the mode of inhibition is only pH dependent for the enzyme that is proteolytically cleaved in a mobile loop in the vicinity of the active site, changing from non- to uncompetitive as the pH is raised; for the intact form fluoride acts as a non-competitive inhibitor at pH 3.30 and 4.90.20
Stable five-coordinate oxovanadium species are a suitable mimic for the five-coordinate phosphoryl transition state proposed for a number of phosphorolytic reactions.30,31 Previously, it was reported that the inhibition constant of pig PAP for vanadate is 40 µmol L-1 at pH 5.5, and the mode of binding of the inhibitor is non-competitive.23 The di-zinc alkaline phosphatase from Escherichia coli is inhibited by vanadate with similar efficiency (Ki = 12 µmol L-1 at pH 8.0), and the crystal structure of the enzyme-inhibitor complex shows that vanadate binds in a penta-coordinate geometry to the active site with three of its oxygen atoms coordinating the two metal ions in the active site in a tripodal arrangement (Figure 1).25
In this work, the inhibitory effects of fluoride and vanadate on the activity of red kidney bean and pig PAP are assessed and compared with those measured for other PAPs. The mechanistic implications of these studies are also discussed.
All solutions were prepared with analytical grade reagents purchased from Sigma, Merck or Fluka.
Pig PAP was extracted from the uterine fluid of a pregnant sow and the plant PAP was purified from the pulp of red kidney beans as described elsewhere.10,32 In brief, both enzymes underwent an initial ion-exchange chromatography step using CM-cellulose resin, followed by gel filtration on a Sephadex G-75 (pig PAP) or Sephadex S-300 column (red kidney bean PAP). Purified pig PAP was stored at -20 ºC in 100 mmol L-1 acetate buffer at pH 4.9 and red kidney bean PAP was stored in 0.5 mol L-1 NaCl at 4 ºC until further use. Protein concentrations were determined by measuring the absorbance at 280 nm using the specific extinction of 1.41 for a 1 mg mL-1 solution (28.6 µmol L-1) of pig PAP and 2.1 for a 1 mg mL-1 solution (9.1 µmol L-1) of rkbPAP. SDS-Page analysis confirmed the purity of the enzymes.
51V Nuclear Magnetic Resonance Spectroscopy
The 51V NMR spectra were recorded at 132 MHz with a Bruker Avance 400MHz NMR. All experiments were conducted at 25 ºC with a spectrum width of 8064 Hz, no relaxation delay, a 90° pulse angle and an accumulation time of 0.2 s. The chemical shifts reported are relative to the external reference (VOCl3; 0 ppm).
Vanadate stock solutions were prepared by boiling a concentrated solution (200 mmol L-1) of (Na)3VO4 in deionised water (MilliQ) for 10 min to maximise the presence of the VO4 monomers.23 Small volumes from these stocks were added to 0.1 mol L-1 MES buffer, pH 6.2, containing 0.2 mol L-1 KCl and 10% (v/v) D2O to generate final vanadate concentrations of 0.025-2.00 mmol L-1. These solutions matched the conditions employed in the kinetics experiments (see below). Relative amounts of the individual species were obtained by peak integration, and total concentrations were calculated by multiplication of the relative amounts by the total vanadate concentration in solution (Figure 2).
The rates of product formation by pig and red kidney bean PAPs were determined at 25 ºC using a continuous assay with para-nitrophenol phosphate (p-NPP) as substrate. Measurements were carried out at pH 4.90 (0.1 mol L-1 acetate buffer, 0.2 mol L-1 KCl) or pH 6.20 (0.1 mol L-1 MES buffer, 0.2 mol L-1 KCl), the respective pH optima for pig and red kidney bean PAPs.21,33 Product (p-NP) formation was monitored at l = 390 nm with De390 = 342.9 mol-1 L cm-1 and 1834.4 mol-1 L cm-1 at pH 4.90 and pH 6.20, respectively. Substrate concentrations ranged from 1 to 15 mmol L-1. Enzyme concentrations in steady-state assays were 20 nmol L-1 and 2 nmol L-1 for the two enzymes, respectively, and 50 nmol L-1 in stopped-flow measurements. Concentrations of the inhibitors ranged from 0.1 to 25 mmol L-1 (NaF) and 0.01 to 0.5 mmol L-1 (Na3VO4).
All steady-state assays were performed with a Varian Cary50 UV-Vis spectrophotometer with 1 cm path length quartz cuvettes. The possibility of measurable pre-steady state reactions was assessed by stopped-flow kinetics using an Applied Photophysics SX18 stopped-flow spectrometer with a 1 cm path length. The data were analysed using GraphPad Prism 4.0 software or WinCurveFit (Kevin Raner software). The catalytic parameters were evaluated by non-linear regression using the Michaelis-Menten (equation 1) or general inhibition equation (equation 2), respectively:
Here, Vmax (= kcat[E]) and Km are the maximum rate and the Michaelis constant, [S] and [I] the concentrations of substrate and inhibitor, and Kic and Kiuc the equilibrium dissociation constants for competitive and uncompetitive inhibitor binding, respectively.34 Pre-steady state data were analysed with equation 3, where A0 and At represent the absorbance (at 390 nm) of product at time 0 and t, vi and vf the rates in the initial and final (steady state) phases of the reaction, and kobs the rate constant for the change from the fast initial rate to the slower final rate.24,35,36
Results and Discussion
The specific activity of pig PAP at pH 4.9 (optimum pH) and pH 6.2 is 635 U mg-1 (kcat = 370 s-1) and 371 U mg-1 (kcat = 216 s-1), respectively, similar to values reported previously.21,32,37,38 For the red kidney bean enzyme the specific activity at pH 4.9 and pH 6.2 (optimum pH) is ~100 U mg-1 (kcat = 180 s-1) and 170 U mg-1 (kcat = 312 s-1), respectively, also in good agreement with previous studies.10 The kinetic parameters are summarised in Table 1. For both enzymes the Km values for the substrate p-NPP increase as the pH is increased, an observation which is likely to be due to the deprotonation of a histidine residue in the substrate binding pocket of the enzyme.16,39
The inhibitory effect of vanadate on the activity of red kidney bean PAP was determined at optimum pH (pH 6.2). At that pH vanadate monomers tend to oligomerise in solution provided the total concentration of the tetraoxo anion is > 0.25 mmol L-1.23 Since the monomeric form is the main inhibitor of PAPs23 it was essential to estimate the concentration of this species under conditions employed in the kinetic assays. Vanadium-51 (99.75% natural abundance) NMR is a convenient method to measure the relative concentrations of vanadate species in solutions.40 Despite the 7/2 spin, line widths for 51V are relatively narrow and are easily resolved.41 The 51V NMR (Figure 2), indicated that under the conditions applied in the kinetic assays the monomer concentration maximised at ~0.6 mmol L-1. Total vanadate concentrations in the kinetic assays were chosen to yield monomer concentrations ranging from 10 µmol L-1 to 500 mmol L-1. Fitting the data in Figure 3 (equation 2) resulted in Kic = 30 µmol L-1 (Table 2), indicating that vanadate acts as a moderately strongly binding competitive inhibitor. No accurate estimate of the inhibition constant could be obtained at pH 4.9 due to the tighter binding (Ki < 10 µmol L-1) and the complex speciation of vanadate at this pH. For pig PAP the inhibition by vanadate was assessed previously at pH 5.5,23 resulting in a Ki of 40 µmol L-1. In contrast to the red kidney bean enzyme, for pig PAP the inhibition mode appears to be non-competitive with Ki = Kic = Kiuc. Furthermore, the same study has revealed that the substitution of the divalent iron by zinc reduces the inhibitory effect of vanadate (Ki = 360 µmol L-1) but not the mode of inhibition.23 Thus, the protein environments in the active sites of pig and red kidney bean PAPs, but not the metal ion compositions, are likely to be responsible for the different modes of inhibition observed. The results obtained for the red kidney bean enzyme resemble those obtained for the di-ZnII alkaline phosphatase from E. coli, where vanadate acts as a competitive inhibitor with Kic = 12 µmol L-1 at pH 8.0.25 The crystal structure of this enzyme, complexed with vanadate, has been solved and supports the hypothesis that vanadate is a suitable mimic of the proposed five-coordinate phosphoryl transition state (Figure 1). Based on the similarity of the inhibition data it appears likely that red kidney bean PAP has a transition state similar to that observed in E. coli alkaline phosphatase. However, pig PAP may differ from these two enzymes based on the variation in the vanadate inhibition kinetics (non-competitive binding of the inhibitor). Hence, subtle variations in the active site structures may have a significant effect on the formation of the transition state.
The inhibitory effect of fluoride was determined for pig and red kidney bean PAPs at pH 4.9 and pH 6.2 and the data were analysed by non-linear regression using equation 2 (Figure 4). For the pig enzyme the mode of inhibition changes from uncompetitive to non-competitive upon raising the pH (Table 3). A similar result has been reported for the FeIIIZnII derivative of PAP from bovine spleen (Table 3).24 The observation of uncompetitive binding of the inhibitor at low pH indicates that fluoride only interacts with the enzyme-substrate (ES) complex. However, at higher pH fluoride can also bind to the free enzyme, competing with the substrate. The competitive binding site has previously been identified in terms of a terminal coordination to the divalent metal ion in the active site.24,42,43 The observation that metal ion substitutions in the divalent sites of pig and bovine PAP moderately affect the magnitude of the inhibition (but not its mode) is consistent with this assignment (Table 3). At lower pH the substrate binds tighter to the active site, most likely due to interactions between a positively charged histidine residue and the negatively charged phosphate group of the substrate.14-17,20 Consequently, fluoride is not an efficient competitor for interactions between the enzyme and the substrate, resulting in the observed uncompetitive mode of inhibition. Uncompetitive interactions between fluoride and FeIII are clearly demonstrated by the effect of metal ion substitutions on the Kiuc of bovine PAP (Table 3). The inhibition of the AlIIIZnII derivative of bovine PAP at low pH is greatly enhanced in comparison to the GaIIIZnII and FeIIIZnII derivatives, in agreement with the prediction that AlIII is a harder acid than GaIII and FeIII.24 In principle, two possibilities for uncompetitive binding exist (Figure 5), (i) a terminal coordination of fluoride to the trivalent iron, or (ii) the formation of a µ-fluoro complex, where the inhibitor bridges the two metal centres, thus displacing the µ-hydroxo group. From kinetic data alone these two possibilities cannot be distinguished, but EXAFS and resonance Raman spectroscopy have shown that the likely uncompetitive binding mode, at least in pig PAP, is the formation of the µ-fluoro complex.29
The magnitude of the inhibition of red kidney bean PAP by fluoride is similar to that determined for both pig and bovine PAP, but the mode of inhibition is competitive, independent of pH (Table 3). In this respect the plant enzyme resembles intact human PAP, where the mode of fluoride inhibition is also not affected by the change in pH, although for the human enzyme inhibition data were only collected at low pH values (pH 3.3 and pH 4.9; Table 3).20 Interestingly, the mode of fluoride inhibition in intact human PAP is non-competitive, contrasting both red kidney bean PAP and other mammalian PAPs (where the competitive inhibition site is inaccessible at low pH; see above). Upon proteolytic cleavage human PAP displays fluoride inhibition kinetics at pH 4.9 similar to those of pig and bovine PAP.20 It appears thus that the cleaved FeIIIFeII form of human PAP is mechanistically related to pig and bovine PAP, while the intact form of this enzyme is similar to red kidney bean PAP although the apparent lack of fluoride binding to the enzyme-substrate complex in the red kidney bean enzyme suggests a mechanistic variation. Furthermore, the competitive nature of the inhibition of red kidney bean PAP by fluoride indicates that the inhibitor mainly interacts with the divalent metal ion (see above).
Fluoride has been shown to act as a slow binding inhibitor to a number of enzymes, including the bimetallic NiII ureases from jack bean44 and Klebsiella aerogenes,36 and bovine PAP.24 In the presence of fluoride reaction progress curves of urease and bovine PAP are biphasic, indicating a gradual change from an initial uninhibited (ni) to a final inhibited (nf; steady-state) rate as fluoride binds. In both enzymes the rate of fluoride binding (kobs) depends on the concentration of the inhibitor. For FeIIIFeII and FeIIIZnII bovine PAP kobs increases linearly with increasing fluoride concentrations at pH 5.0, reaching a value of ~0.12 s-1 and ~0.25 s-1 at [F-] = 2 mmol L-1, respectively.24 The moderate variation in kobs upon metal ion substitution in the divalent site suggests that the observed slow binding of fluoride is mainly due to the interaction of the inhibitor with the trivalent metal ion. The observation that the rate of fluoride binding drastically increases upon replacing FeIII by AlIII and GaIII is in agreement with this hypothesis.24 In this study the FeIIIFeII pig PAP reaction was monitored at pH 4.9 (optimal pH for activity) at several fluoride concentrations (Figure 6). In the presence of 2 mmol L-1 inhibitor kobs is 0.047 s-1 (Table 4), approximately 40% of the value obtained for bovine PAP, suggesting a conserved mode of interaction between enzyme and inhibitor in animal PAPs. This is not surprising based on the similarity of the inhibition constants determined for the two enzymes (Table 3). An intriguing observation is the fact that the pre-incubation of the enzyme with fluoride does not greatly affect the final steady-state rate (nf) of the reaction, but the initial rates are reduced (Table 4). A similar result has been reported for K. aerogenes urease and has been interpreted in terms of this enzyme existing in two distinct conformations in the resting state, one with low and one with high affinity for fluoride.36 It is thus possible that the resting state of pig PAP occurs in at least two distinct conformations that co-exist in equilibrium. Addition of the substrate shifts this equilibrium in favour of the state with higher fluoride affinity. The existence of at least two distinct conformations in the resting state may explain catalytic variations observed between various mammalian PAPs (e.g. Table 3), and may be associated with the mobile repression loop in the vicinity of the active site.18,20,28
Fluoride inhibition of red kidney bean PAP appears instantaneous (Figure 6), within the technical limitations of the stopped-flow instrument, indicating a vastly increased kobs. Also, prolonged incubation with fluoride did not affect the rate (Table 4). The loss of activity upon incubation for 60 min is small and comparable in the inhibited and uninhibited enzyme (Figure 6). Hence, in agreement with the results above red kidney bean PAP interacts in a distinctly different manner with fluoride than mammalian PAPs. The rapid establishment of inhibition is consistent with fluoride binding predominantly to the divalent metal ion (rapid ligand exchange) and agrees with the observed competitive inhibition (Table 3).
PAPs display a high degree of structural similarity in their active sites, and consequently their catalytic reactions are anticipated to employ the same mechanism. Interestingly, variations are observed in the interactions between representatives of these enzymes and vanadate and fluoride. Since these anions have been proposed to mimic the transition state of phosphorolytic enzymes,25 or displace the reaction-initiating nucleophile,1,24,29 the kinetic variations between red kidney bean and mammalian PAPs indicate that these enzymes employ alternative mechanistic strategies. Specifically, the precise nature of their transition states and the identity of their nucleophiles may vary. A structural understanding of these differences may be particularly significant in terms of the design and development of site-specific inhibitors for PAPs. Considering the crucial role(s) mammalian PAPs have in bone metabolism such inhibitors are anticipated to be promising lead compounds in the development of new anti-osteoporotic chemotherapeutics. Efforts towards these aims are currently in progress in our group.
This work was funded by a grant from the Australian Research Council (DP0558652). The authors would like to thank Ms Eleanor Leung and Ms Fernanda Ely for their assistance.
1. Mitic, N.; Smith, S. J.; Neves, A.; Guddat, L.W.; Gahan, L.R.; Schenk, G.; Chem. Rev. 2006, 106, 3338. [ Links ]
2. Bull, H.; Murray, P. G.; Thomas, D.; Fraser, A. M.; Nelson, P. N.; J. Clin. Pathol.-Mol. Pathol. 2002, 55, 65. [ Links ]
3. Antanaitis, B. C.; Aisen, P.; Lilienthal, H. R.; J. Biol. Chem. 1983, 258, 3166. [ Links ]
4. Yang, Y.; McCormick, J. M.; Solomon, E. I.; J. Am. Chem. Soc. 1997, 119, 11834. [ Links ]
5. Oddie, G. W.; Schenk, G.; Angel, N. Z.; Walsh, N.; Guddat, L. W.; de Jersey, J.; Cassady, A. I.; Hamilton, S. E.; Hume, D. A.; Bone 2000, 27, 575. [ Links ]
6. Schenk, G.; Guddat, L. W.; Ge, Y.; Carrington, L. E.; Hume, D. A.; Hamilton, S.; de Jersey, J.; Gene 2000, 250, 117. [ Links ]
7. Schenk, G.; Korsinczky, M. L. J.; Hume, D. A.; Hamilton, S.; de Jersey, J.; Gene 2000, 255, 419. [ Links ]
8. Flanagan, J. U.; Cassady, A. I.; Schenk, G.; Guddat, L. W.; Hume, D. A.; Gene 2006, 377, 12. [ Links ]
9. Bernhardt, P. V.; Schenk, G.; Wilson, G. J.; Biochemistry 2004, 43, 10387. [ Links ]
10. Beck, J. L.; McConaghie, L. A.; Summors, A. C.; Arnold, W. N.; de Jersey, J.; Zerner, B.; Biochim. Biophys. Acta 1986, 869, 61. [ Links ]
11. Schenk, G.; Ge, Y.; Carrington, L. E.; Wynne, C. J.; Searle, I. R.; Carroll, B. J.; Hamilton, S.; de Jersey, J.; Arch. Biochem. Biophys. 1999, 370, 183. [ Links ]
12. Durmus, A.; Eicken, C.; Spener, F.; Krebs, B.; Biochim. Biophys. Acta, Protein Struct. Mol. Enzymol. 1999, 1434, 202. [ Links ]
13. Sträter, N.; Klabunde, T.; Tucker, P.; Witzel, H.; Krebs, B.; Science 1995, 268, 1489. [ Links ]
14. Klabunde, T.; Sträter, N.; Fröhlich, R.; Witzel, H.; Krebs, B.; J. Mol. Biol. 1996, 259, 737. [ Links ]
15. Guddat, L. W.; McAlpine, A. S.; Hume, D. A.; Hamilton, S.; de Jersey, J.; Martin, J. L.; Structure 1999, 7, 757. [ Links ]
16. Schenk, G.; Gahan, L. R.; Carrington, L. E.; Mitic, N.; Valizadeh, M.; Hamilton, S. E.; de Jersey, J.; Guddat, L. W.; Proc. Natl. Acad. Sci. U. S. A. 2005, 102, 273. [ Links ]
17. Lindqvist, Y.; Johansson, E.; Kaija, H.; Vihko, P.; Schneider, G.; J. Mol. Biol. 1999, 291, 135. [ Links ]
18. Sträter, N.; Jasper, B.; Scholte, M.; Krebs, B.; Duff, A. P.; Langley, D. B.; Han, R.; Averill, B. A.; Freeman, H. C.; Guss, J. M.; J. Mol. Biol. 2005, 351, 233. [ Links ]
19. Ljusberg, L.; Ek-Rylander, B.; Andersson, G.; Biochem. J. 1999, 343, 63. [ Links ]
20. Mitic, N.; Valizadeh, M.; Leung, E. W. W.; de Jersey, J.; Hamilton, S.; Hume, D. A.; Cassady, A. I.; Schenk, G.; Arch. Biochem. Biophys. 2005, 2, 154. [ Links ]
21. Valizadeh, M.; Schenk, G.; Nash, K.; Oddie, G. W.; Guddat, L. W.; Hume, D. A.; de Jersey, J.; Burke, T. R.; Hamilton, S.; Arch. Biochem. Biophys. 2004, 424, 154. [ Links ]
22. Moss, D. W.; Raymond, F. D.; Wile, D. B.; Crit. Rev. Clin. Lab. Sci. 1995, 32, 431. [ Links ]
23. Crans, D. C.; Simone, S.; Holz, R. C.; Que, L., Jr.; Biochemistry 1992, 31, 11731. [ Links ]
24. Pinkse, M. W.; Merkx, M.; Averill, B. A.; Biochemistry 1999, 38, 9926. [ Links ]
25. Holtz, K. M.; Stec, B.; Kantrowitz, E. R.; J. Biol. Chem. 1999, 274, 8351. [ Links ]
26. Cama, E.; Pethe, S.; Boucher, J.; Han, S.; Emig, F. A.; Ash, D. E.; Biochemistry 2004, 43, 8987. [ Links ]
27. Funhoff, E.G.; Bollen, M.; Averill, B. A.; J. Inorg. Biochem. 2005, 272, 2968. [ Links ]
28. Funhoff, E.G.; de Jongh, T. E.; Averill, B. A.; J. Biol. Inorg. Chem. 2005, 10, 550. [ Links ]
29. Wang, X.; Ho, R. Y. N.; Whiting, A. K.; Que, L., Jr.; J. Am. Chem. Soc. 1999, 121, 9235. [ Links ]
30. Lahiri, S. D.; Zhang, G.; Dunaway-Mariano, D.; Allen, K. N.; Science 2003, 299, 2067. [ Links ]
31. Davies, D. R.; Hol, W. G. J.; FEBS Lett. 2004, 577, 315. [ Links ]
32. Campbell, H. D.; Dionysius, D. A.; Keough, D. T.; Wilson, B. E.; de Jersey, J.; Zerner, B.; Biochem. Biophys. Res. Commun. 1978, 82, 615. [ Links ]
33. Truong, N. T.; Naseri, J. I.; Vogel, A.; Rompel, A.; Krebs, B.; Arch. Biochem. Biophys. 2005, 440, 38. [ Links ]
34. Segel, I. H.; Enzyme Kinetics: Behavior and Analysis of Rapid Equilibrium and Steady-State Enzyme Systems, library ed., Wiley: New York, 1993. [ Links ]
35. Cha, S.; Biochem. Pharmacol. 1975, 24, 2177. [ Links ]
36. Todd, M. J.; Hausinger, R. P.; Biochemistry 2000, 39, 5389. [ Links ]
37. Schlosnagle, D. C.; Bazer, F. W.; Tsibris, J. C.; J. Biol. Chem. 1974, 249, 7574. [ Links ]
38. Beck, J. L.; Keough, D. T.; de Jersey, J.; Zerner, B.; Biochim. Biophys. Acta 1984, 791, 357. [ Links ]
39. Merkx, M.; Pinkse, M. W.; Averill, B. A.; Biochemistry 1999, 38, 9914. [ Links ]
40. Butler, A.; Eckert, H.; J. Am. Chem. Soc. 1989, 111, 2802. [ Links ]
41. Crans, D. C.; Shin, P. K.; Inorg. Chem. 1988, 27, 1797. [ Links ]
42. Aquino, M. A. S.; Lim, J.-S.; Sykes, A. G.; J. Chem. Soc. Dalton Trans. 1994, 429. [ Links ]
43. Twitchett, M. B.; Schenk, G.; Aquino, M. A. S.; Yiu, D. T.; Lau, T.-C.; Sykes, A. G.; Inorg. Chem. 2002, 41, 5787. [ Links ]
44. Dixon, N. E.; Blakeley, R. L.; Zerner, B.; Can. J. Biochem. 1980, 58, 481. [ Links ]
Received: May 26, 2006
Published on the web: November 7, 2006