Skip to main content
NIHPA Author Manuscripts logoLink to NIHPA Author Manuscripts
. Author manuscript; available in PMC: 2012 Apr 20.
Published in final edited form as: J Am Chem Soc. 2011 Mar 24;133(15):5683–5685. doi: 10.1021/ja111457h

Kinetic challenges facing oxalate, malonate, acetoacetate and oxaloacetate decarboxylases

Richard Wolfenden 1, Charles A Lewis Jr 1, Yang Yuan 1
PMCID: PMC3077560  NIHMSID: NIHMS283578  PMID: 21434608

Abstract

To compare the power of the corresponding enzymes as catalysts, the rates of uncatalyzed decarboxylation of several aliphatic acids (oxalate, malonate, acetoacetate and oxaloacetate) were determined at elevated temperatures and extrapolated to 25 °C. In the extreme case of oxalate, the rate of the uncatalyzed reaction at pH 4.2 was 5 × 10−12 s−1, implying a 2.5 × 1013-fold rate enhancement by oxalate decarboxylase. Whereas the enzymatic decarboxylation of oxalate requires O2 and MnII, the uncatalyzed reaction is unaffected by the presence of these cofactors and appears to proceed by heterolytic elimination of CO2.


To be useful at the limited concentrations at which they are present within cells (< 10−4 M),1 enzymes must act rapidly on their substrates. But in the absence of enzymes, biological reactions proceed with half-lives ranging from <1 minute for the dehydration of bicarbonate2 to >1 billion years for the decarboxylation of glycine.3 Those rate enhancements are of interest in estimating the power of enzymes and artificial catalysts and their expected sensitivity to transition state analogue inhibitors. Here, we compare the rates of spontaneous and enzymatic decarboxylation of oxalate with those of malonate, acetoacetate and oxaloacetate.

Kinetic experiments on the monoanions of malonate, acetoacetate and oxaloacetate were conducted in potassium phosphate buffer (pH 6.8), where the corresponding decarboxylases are maximally active.46 The nonenzymatic decarboxylation of oxalate was examined in potassium acetate buffer (pH 4.2), because oxalate decarboxylase is maximally active near pH 4.2.7 Phosphate and acetate buffers were chosen because acetic acid and the phosphoric acid monoanion—like the acids undergoing decarboxylation—exhibit near-zero (<1 kcal/mol) heats of proton dissociation,8 canceling the effects of varying temperature on the state of ionization of each substrate. Samples of the potassium salt of each acid (0.01 M) in potassium acetate or phosphate buffer (0.1 M) were introduced into quartz tubes, sealed under vacuum and placed in convection ovens for various intervals at temperatures maintained within ±1.5 °C as indicated by ASTM thermometers. For each acid, the range of temperatures examined is indicated in Table 1. After cooling, samples were diluted with D2O containing pyrazine (5 × 10−4 M), added as an integration standard. In each case, 1H NMR showed quantitative conversion of the carboxylic acid to the expected product of decarboxylation. Rates of decarboxylation of malonate and acetoacetate were estimated by monitoring the disappearance of the reactants, and each reaction followed simple first order kinetics to completion. In the cases of oxaloacetate (whose C-H protons exchange rapidly with solvent water) and oxalate (with no carbon-bound protons), rates were estimated by monitoring the appearance of their decarboxylation products, pyruvate and formate. At each temperature, times of heating (between 2 and 72 hours) were chosen so that consumption of the reactant had proceeded to between 15% and 85% completion, yielding individual rate constants with estimated errors of ± 3%. These rate constants, plotted as a logarithmic function of 1/T (Kelvin), showed a linear relationship over the full range of temperatures examined, and were used to estimate the enthalpy of activation (ΔH) and the rate constant for each reaction at 25 °C (knon). The results are shown in Table 1, and are included in further detail, along with values previously reported for these and other decarboxylation reactions, in Supporting Information.

Table 1.

Rate constants at 25 °C (s−1), and thermodynamics of activation (kcal/mol) for the decarboxylation of oxaloacetate, acetoacetate and malonate at pH 6.8, and of oxalate at pH 4.3 (Values for the pure monoanions in italics) (Supporting Information).

Reactant (product) k25°, s−1 ΔG ΔH TΔS range

Oxaloacetate (pyruvate) 2.8 × 10−5 23.6 17.2 −6.4
9.2 × 105 24.2 17.2 7.0 23–70°

Acetoacetate (acetone) 3.0 × 10−7 26.2 23.5 −2.7
3.0 × 107 26.2 23.5 2.7 23–61°

Malonate (acetate) 1.2 × 10−10 30.9 30.0 −0.9
1.5 × 109 29.4 30.0 +0.6 80–130°

Oxalate (formate) 1.1 × 10−12 33.7 26.9 −6.8
1.8 × 1012 33.3 26.9 6.6 150–190°

Rate constants observed for the decarboxylation of the monoanions of oxaloacetic, acetoacetic acid and malonic acid monoanions fall close to a linear Brønsted plot based on the pKa values of the carbon acids produced by decarboxylation (Figure 1), yielding a slope (β = −0.7) consistent with the development of substantial negative charge at the site where CO2 elimination occurs.

Figure 1.

Figure 1

Rate constants at pH 6.8 and 25 °C for decarboxylation of the monoanions of iminomalonate (IM), oxaloacetate (OA), aminomalonate (AM),15 acetoacetate (AA), trichloroacetate (TA)16, malonate (MA), cyanoacetate (CA),17 glycine (GL)3 and 1-methylorotate (MeO)18 plotted as a logarithmic function of the pKa values of the products of their decarboxylation as carbon acids (Supporting Information).

Enzymes use various strategies to catalyze these decarboxylation reactions, employing an imine-forming lysine residue in the case of acetoacetate, or a divalent cation (Mg, Mn, Zn or Co) in the case of oxaloacetate, whose intervention would be expected to stabilize a transition state with carbanionic character. In the absence of enzymes, those reactions are catalyzed by amines9 and divalent cations10 respectively. The enzymatic elimination of CO2 from malonate is a more complex process involving preliminary formation of a malonyl-enzyme thioester that appears to be the species that actually undergoes decarboxylation.5 Oxalate decarboxylase catalyzes a relatively difficult reaction (Table 1), using both a divalent cation (MnII) and molecular oxygen as cofactors.11,12 as noted below. Amino acid decarboxylations generally involve transimination of enzyme-bound PLP (or a pyruvoyl-enzyme), and PLP by itself has been shown to act as an effective catalyst.3,13

Figure 2 shows that the kcat values of these enzymes fall within a relatively narrow range (Supporting Information); but that because of major differences in the rates of the uncatalyzed reactions, these enzymes vary greatly in the rate enhancements (kcat/knon) that they produce. Particularly striking is oxalate decarboxylase from B. subtilis, which is maximally active near pH 4.2 (the pKa value of the oxalic acid monoanion), where it exhibits a kcat value of 28 s−1 (per Mn atom)7 and generates a rate enhancement of 2.5 × 1013 (Table 2).

Figure 2.

Figure 2

Half-lives at 25 °C for decarboxylation of glycine,3 malonate, acetoacetate and oxaloacetate at pH 6.8, and of oxalate at the pH 4.3, in the presence (kact) and absence (knon) of the corresponding decarboxylases.

Table 2.

Rate enhancements produced by decarboxylases at 25 °C.

Reactant k25°, s−1 kcat, s−1 (ref) kcat/knon
Oxaloacetate, pH 6.8 2.8 × 10−5 7.5 × 103 (6) 2.7 × 108
Acetoacetate, pH 6.8 3.0 × 10−7 1.6 × 103 (4) 5.3 × 109
Oxalate, pH 4.3 1.1 × 10−12 28 (7) 2.5 × 1013
Glycine, pH 6.8 3 2.0 × 10−17 1.4 × 103 (3) 7 × 1019

The low intrinsic reactivity of oxalate seems understandable in view of the absence of electron-withdrawing groups that might facilitate CO2 elimination. It is therefore not surprising that oxalate decarboxylase has evolved a special strategy for catalyzing this difficult reaction. The action of oxalate decarboxylase has been shown to involve a radical mechanism in which O2, an essential cofactor, combines with MnII in such a way as to permit single electron transfers that facilitate cleavage of the cleavage of bound oxalate without requiring formation of a formyl dianion as a discrete intermediate.14,19 In the cases of oxaloacetate and acetoacetate decarboxylation, amines and metal ion cofactors have been shown to act as catalysts in the absence of the apoenzyme. However, experiments at elevated temperatures (150–200 °C) show that the rate of nonenzymatic decarboxylation of oxalate is not enhanced significantly in solutions to which manganese sulfate (1 M) has been added, or by the further addition of oxygen (1 × 10−3 M) or hydrogen peroxide (1 M). Thus, the decarboxylation of oxalate appears to proceed by entirely different mechanisms in the presence and absence of enzyme.

Supplementary Material

1_si_001

Acknowledgments

We thank the National Institutes of Health for supporting this work (Grant # GM-18325).

Footnotes

Supporting Information Available Present and previously reported rate constants for the nonenzymatic decarboxylation of oxaloacetate, acetoacetate, malonate and oxalate. pKa values of carbon acid produced by decarboxylation. Properties of enzymes catalyzing the decarboxylation of oxaloacetate, acetoacetate, malonate and oxalate.

References

  • 1.Albe KR, Butler MH, Wright BE. J Theoret Biol. 1990;143:163–195. doi: 10.1016/s0022-5193(05)80266-8. [DOI] [PubMed] [Google Scholar]
  • 2.Roughton FJW. J Am Chem Soc. 1941;63:2930–2934. [Google Scholar]
  • 3.Snider MJ, Wolfenden R. J Am Chem Soc. 2000;122:11507–11508. [Google Scholar]
  • 4.Highbarger LA, Gerlt JA, Kenyon GL. Biochemistry. 1996;35:41–46. doi: 10.1021/bi9518306. [DOI] [PubMed] [Google Scholar]
  • 5.Kim KS, Byun HS. J Biol Chem. 1994;269:29636–29641. [PubMed] [Google Scholar]
  • 6.Narayanan BC, Niu W, Han Y, Zou J, Mariano PS, Dunaway-Mariano D, Herzberg O. Biochemistry. 2008;47:167–182. doi: 10.1021/bi701954p. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 7.Svedruzic D, Liu Y, Reinhardt LA, Wroclawska E, Cleland WW, Richards NGJ. Arch Biochem Biophys. 2007;464:36–47. doi: 10.1016/j.abb.2007.03.016. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 8.Edsall JT, Wyman J. Biophysical Chemistry. Vol. 1. Academic Press; New York: 1958. pp. 452–453. [Google Scholar]
  • 9.(a) Wiig EO. J Phys Chem. 1928;32:961–981. [Google Scholar]; (b) Pedersen KJ. J Phys Chem. 1937;38:559–571. [Google Scholar]; (c) Guthrie JP, Jordan F. J Am Chem Soc. 1972;94:9136–9141. [Google Scholar]
  • 10.(a) Steinberger R, Westheimer FH. J Am Chem Soc. 1951;73:429–435. [Google Scholar]; (b) Gelles T, Salama A. Acta Chem Scand. 1958;12:3689–3693. [Google Scholar]; (c) Raghavan NV, Leussing DL. J Am Chem Soc. 1974;96:7147–7149. [Google Scholar]
  • 11.Emiliani E, Riera B. Biochem Biophys Acta. 1968;167:414–421. doi: 10.1016/0005-2744(68)90221-0. [DOI] [PubMed] [Google Scholar]
  • 12.Moomaw EW, Angerhofer A, Moussatche P, Ozarowski A, Garcia-Rubio I, Richards NGJ. Biochemistry. 2009;48:6116–6125. doi: 10.1021/bi801856k. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 13.Zabinski RF, Toney M. J Am Chem Soc. 2001;123:193–198. doi: 10.1021/ja0026354. [DOI] [PubMed] [Google Scholar]
  • 14.Tanner A, Bowater L, Fairhurst SA, Bornemann S. J Biol Chem. 2001;276:43627–43634. doi: 10.1074/jbc.M107202200. [DOI] [PubMed] [Google Scholar]
  • 15.Callahan BP, Wolfenden R. J Am Chem Soc. 2004;126:4514–4515. doi: 10.1021/ja031720j. [DOI] [PubMed] [Google Scholar]
  • 16.Verhoek FH. J Am Chem Soc. 1934;56:571–577. [Google Scholar]
  • 17.Richard JP, Williams G, Gao J. J Am Chem Soc. 1999;121:715–726. [Google Scholar]
  • 18.Radzicka A, Wolfenden R. Science. 1995;267:90–93. doi: 10.1126/science.7809611. [DOI] [PubMed] [Google Scholar]
  • 19.Imaram W, Saylor BT, Centonze CP, Richards NGJ, Angerhofer A. Free Rad Biol Med. 2011;50:1009–1015. doi: 10.1016/j.freeradbiomed.2011.01.023. [DOI] [PMC free article] [PubMed] [Google Scholar]

Associated Data

This section collects any data citations, data availability statements, or supplementary materials included in this article.

Supplementary Materials

1_si_001

RESOURCES