Phosphorus-31 nuclear magnetic resonance of dihydroxyacetone phosphate in the presence of triosephosphate isomerase. The question of nonproductive binding of the substrate hydrate

Labile Metabolite Profiling in Human Blood Using Phosphorus NMR Spectroscopy

Phosphorus metabolites occupy a unique place in cellular function as critical intermediates and products of cellular metabolism. Human blood is the most widely used biospecimen in the clinic and in the metabolomics field, and hence an ability to profile phosphorus metabolites in blood, quantitatively, would benefit a wide variety of investigations of cellular functions in health and diseases. Mass spectrometry (MS) and nuclear magnetic resonance (NMR) spectroscopy are the two premier analytical platforms used in the metabolomics field. However, detection and quantitation of phosphorus metabolites by MS can be challenging due to their lability, high polarity, structural isomerism, and interaction with chromatographic columns. The conventionally used 1H NMR, on the other hand, suffers from poor resolution of these compounds. As a remedy, 31P NMR promises an important alternative to both MS and 1H NMR. However, numerous challenges including the instability of phosphorus metabolites, their chemical shift sensitivity to solvent composition, pH, salt, and temperature, and the lack of identified metabolites have so far restricted the scope of 31P NMR. In the current study, we describe a method to analyze nearly 25 phosphorus metabolites in blood using a simple one-dimensional (1D) NMR spectrum. Establishment of the identity of unknown metabolites involved a combination of (a) comprehensively analyzing an array of 1D and two-dimensional (2D) 1H/31P homonuclear and heteronuclear NMR spectra of blood; (b) mapping the central carbon metabolic pathway; (c) developing and using 1H and 31P spectral and chemical shift databases; and finally (d) confirming the putative metabolite peaks with spiking using authentic compounds. The resulting simple 1D 31P NMR-based method offers an ability to visualize and quantify the levels of intermediates and products of multiple metabolic pathways, including central carbon metabolism, in one step. Overall, the findings represent a new dimension for blood metabolite analysis and are anticipated to greatly impact the blood metabolomics field.

Phosphorus NMR and Its Application to Metabolomics

Stable isotopes are routinely employed by NMR metabolomics to highlight specific metabolic processes and to monitor pathway flux. 13C-carbon and 15N-nitrogen labeled nutrients are convenient sources of isotope tracers and are commonly added as supplements to a variety of biological systems ranging from cell cultures to animal models. Unlike 13C and 15N, 31P-phosphorus is a naturally abundant and NMR active isotope that does not require an external supplemental source. To date, 31P NMR has seen limited usage in metabolomics because of a lack of reference spectra, difficulties in sample preparation, and an absence of two-dimensional (2D) NMR experiments, but 31P NMR has the potential of expanding the coverage of the metabolome by detecting phosphorus-containing metabolites. Phosphorylated metabolites regulate key cellular processes, serve as a surrogate for intracellular pH conditions, and provide a measure of a cell's metabolic energy and redox state, among other processes. Thus, incorporating 31P NMR into a metabolomics investigation will enable the detection of these key cellular processes. To facilitate the application of 31P NMR in metabolomics, we present a unified protocol that allows for the simultaneous and efficient detection of 1H-, 13C-, 15N-, and 31P-labeled metabolites. The protocol includes the application of a 2D 1H-31P HSQC-TOCSY experiment to detect 31P-labeled metabolites from heterogeneous biological mixtures, methods for sample preparation to detect 1H-, 13C-, 15N-, and 31P-labeled metabolites from a single NMR sample, and a data set of one-dimensional (1D) 31P NMR and 2D 1H-31P HSQC-TOCSY spectra of 38 common phosphorus-containing metabolites to assist in metabolite assignments.

Active-Site Glu165 Activation in Triosephosphate Isomerase and Its Deprotonation Kinetics

Triosephosphate isomerase (TIM) catalyzes the interconversion between dihydroxyacetone phosphate (DHAP) and d-glyceraldehyde 3-phosphate (GAP) via an enediol(ate) intermediate. The active-site residue Glu165 serves as the catalytic base during catalysis. It abstracts a proton from C1 carbon of DHAP to form the reaction intermediate and donates a proton to C2 carbon of the intermediate to form product GAP. Our difference Fourier transform infrared spectroscopy studies on the yeast TIM (YeTIM)/phosphate complex revealed a C═O stretch band at 1706 cm^-1 from the protonated Glu165 carboxyl group at pH 7.5, indicating that the p K_a of the catalytic base is increased by >3.0 pH units upon phosphate binding, and that the Glu165 carboxyl environment in the complex is still hydrophilic in spite of the increased p K_a. Hence, the results show that the binding of the phosphodianion group is part of the activation mechanism which involves the p K_a elevation of the catalytic base Glu165. The deprotonation kinetics of Glu165 in the μs to ms time range were determined via infrared (IR) T-jump studies on the YeTIM/phosphate and ("heavy enzyme") [U-¹³C,-¹⁵N]YeTIM/phosphate complexes. The slower deprotonation kinetics in the ms time scale is due to phosphate dissociation modulated by the loop motion, which slows down by enzyme mass increase to show a normal heavy enzyme kinetic isotope effect (KIE) ∼1.2 (i.e., slower rate in the heavy enzyme). The faster deprotonation kinetics in the tens of μs time scale is assigned to temperature-induced p K_a decrease, while phosphate is still bound, and it shows an inverse heavy enzyme KIE ∼0.89 (faster rate in the heavy enzyme). The IR static and T-jump spectroscopy provides atomic-level resolution of the catalytic mechanism because of its ability to directly observe the bond breaking/forming process.

Difference FTIR Studies of Substrate Distribution in Triosephosphate Isomerase

Triosephosphate isomerase (TIM) catalyzes the interconversion between dihydroxyacetone phosphate (DHAP) and d-glyceraldehyde 3-phosphate (GAP), via an enediol(ate) intermediate. Determination of substrate population distribution in the TIM/substrate reaction mixture at equilibrium and characterization of the substrate-enzyme interactions in the Michaelis complex are ongoing efforts toward the understanding of the TIM reaction mechanism. By using isotope-edited difference Fourier transform infrared studies with unlabeled and 13C-labeled substrates at specific carbon(s), we are able to show that in the reaction mixture at equilibrium the keto DHAP is the dominant species and the populations of aldehyde GAP and enediol(ate) are very low, consistent with the results from previous X-ray structural and 13C NMR studies. Furthermore, within the DHAP side of the Michaelis complex, there is a set of conformational substates that can be characterized by the different C2═O stretch frequencies. The C2═O frequency differences reflect the different degree of the C2═O bond polarization due to hydrogen bonding from active site residues. The C2═O bond polarization has been considered as an important component for substrate activation within the Michaelis complex. We have found that in the enzyme-substrate reaction mixture with TIM from different organisms the number of substates and their population distribution within the DHAP side of the Michaelis complex may be different. These discoveries provide a rare opportunity to probe the interconversion dynamics of these DHAP substates and form the bases for the future studies to determine if the TIM-catalyzed reaction follows a simple linear reaction pathway, as previously believed, or follows parallel reaction pathways, as suggested in another enzyme system that also shows a set of substates in the Michaelis complex.

Common enzymological experiments allow free energy profile determination

The determination of a complete set of rate constants [free energy profiles (FEPs)] for a complex kinetic mechanism is challenging. Enzymologists have devised a variety of informative steady-state kinetic experiments (e.g., Michaelis-Menten kinetics, viscosity dependence of kinetic parameters, kinetic isotope effects, etc.) that each provide distinct information regarding a particular kinetic system. A simple method for combining steady-state experiments in a single analysis is presented here, which allows microscopic rate constants and intrinsic kinetic isotope effects to be determined. It is first shown that Michaelis-Menten kinetic parameters (kcat and Km values), kinetic isotope efffets, solvent viscosity effects, and intermediate partitioning measurements are sufficient to define the rate constants for a reversible uni-uni mechanism with an intermediate, EZ, between the ES and EP complexes. Global optimization provides the framework for combining the independent experimental measurements, and the search for rate constants is performed using algorithms implemented in the biochemical software COPASI. This method is applied to the determination of FEPs for both alanine racemase and triosephosphate isomerase. The FEPs obtained from global optimization agree with those in the literature, with important exceptions. The method opens the door to routine and large-scale determination of FEPs for enzymes.

Dihydroxyacetone phosphate, DHAP, in the crystalline state: monomeric and dimeric forms

It was shown that dihydroxyacetone phosphate may exist in both monomeric DHAP (C(3)H(7)O(6)P) and dimeric DHAP-dimer (C(6)H(14)O(12)P(2)) form. Monomeric DHAP was obtained in the form of four crystalline salts: CaCl(DHAP) x 2.9H(2)O (7a), Ca(2)Cl(3)(DHAP) x 5H(2)O (7b), CaCl(DHAP) x 2H(2)O (7c), and CaBr(DHAP) x 5H(2)O (7d) by crystallization from aqueous solutions containing DHAP acid and CaCl(2) or CaBr(2), or by direct crystallization from a solution containing DHAP precursor and CaCl(2). At least one of the salts is stable and may be stored in the crystalline state at room temperature for several months. The dimeric form was obtained by slow saturation of free DHAP syrup with ammonia at -18 degrees C and isolated in the form of its hydrated diammonium salt (NH(4))(2)(DHAP-dimer) x 4H(2)O (8). The synthesis of the compounds, their crystallization, and crystal structures determined by X-ray crystallography are described. In all 7a-d monomeric DHAP exists in the monoanionic form in an extended (in-plane) cisoid conformation, with both hydroxyl and ester oxygen atoms being synperiplanar to the carbonyl O atom. The crucial structural feature is the coordination manner, in which the terminal phosphate oxygen atoms act as chelating as well as bridging atoms for the calcium cations. Additionally, the DHAP monoanions chelate another Ca(2+) by the alpha-hydroxycarbonyl moiety, in a manner observed previously in dihydroxyacetone (DHA) calcium chloride complexes. In dimeric 8 the anion is a trans isomer with the dioxane ring in a chair conformation with the hydroxyl groups in axial positions and the phosphomethyl group in an equatorial position.

Enzymatic catalysis of proton transfer at carbon: activation of triosephosphate isomerase by phosphite dianion

More than 80% of the rate acceleration for enzymatic catalysis of the aldose-ketose isomerization of (R)-glyceraldehyde 3-phosphate (GAP) by triosephosphate isomerase (TIM) can be attributed to the phosphodianion group of GAP [Amyes, T. L., O'Donoghue, A. C., and Richard, J. P. (2001) J. Am. Chem. Soc. 123, 11325-11326]. We examine here the necessity of the covalent connection between the phosphodianion and triose sugar portions of the substrate by "carving up" GAP into the minimal neutral two-carbon sugar glycolaldehyde and phosphite dianion pieces. This "two-part substrate" preserves both the alpha-hydroxycarbonyl and oxydianion portions of GAP. TIM catalyzes proton transfer from glycolaldehyde in D2O, resulting in deuterium incorporation that can be monitored by 1H NMR spectroscopy, with kcat/Km = 0.26 M-1 s-1. Exogenous phosphite dianion results in a very large increase in the observed second-order rate constant (kcat/Km)obsd for turnover of glycolaldehyde, and the dependence of (kcat/Km)obsd on [HPO32-] exhibits saturation. The data give kcat/Km = 185 M-1 s-1 for turnover of glycolaldehyde by TIM that is saturated with phosphite dianion so that the separate binding of phosphite dianion to TIM results in a 700-fold acceleration of proton transfer from carbon. The binding of phosphite dianion to the free enzyme (Kd = 38 mM) is 700-fold weaker than its binding to the fleeting complex of TIM with the altered substrate in the transition state (Kd = 53 muM); the total intrinsic binding energy of phosphite dianion in the transition state is 5.8 kcal/mol. We propose a physical model for catalysis by TIM in which the intrinsic binding energy of the substrate phosphodianion group is utilized to drive closing of the "mobile loop" and a protein conformational change that leads to formation of an active site environment that is optimally organized for stabilization of the transition state for proton transfer from alpha-carbonyl carbon.

Substrate product equilibrium on a reversible enzyme, triosephosphate isomerase

The highly efficient glycolytic enzyme, triosephosphate isomerase, is expected to differentially stabilize the proposed stable reaction species: ketone, aldehyde, and enediol(ate). The identity and steady-state populations of the chemical entities bound to triosephosphate isomerase have been probed by using solid- and solution-state NMR. The 13C-enriched ketone substrate, dihydroxyacetone phosphate, was bound to the enzyme and characterized at steady state over a range of sample conditions. The ketone substrate was observed to be the major species over a temperature range from -60 degrees C to 15 degrees C. Thus, there is no suggestion that the enzyme preferentially stabilizes the reactive intermediate or the product. The predominance of dihydroxyacetone phosphate on the enzyme would support a mechanism in which the initial proton abstraction in the reaction from dihydroxyacetone phosphate to D-glyceraldehyde 3-phosphate is significantly slower than the subsequent chemical steps.

Structural characterization of Ru-bleomycin complexes by resonance Raman, circular dichroism, and NMR spectroscopy

A series of spectroscopic techniques including absorption and CD spectra, resonance Raman spectra, and (1)H NMR as well as electrospray mass spectrometry have shown that Ru(II) ion binds to bleomycin, forming an equimolar complex, similarly to Fe(II), i.e., via the secondary amine nitrogen, the pyrimidine ring nitrogen, the deprotonated peptide bond nitrogen of the histydyl residue, and the histidine imidazole nitrogen, which are bound in the equatorial positions, and the alpha-amino nitrogen of beta-aminoalanine, which coordinates in the apical position above pH 7. The reaction of Ru(II)-BLM with O(2), H(2)O(2),or PhIO leads to formation of the oxy species in which only one oxygen atom is bound to metal ion. According to our data, the reaction of Ru(II)-BLM complex with oxygen species leads to different product than that suggested for Fe(II)-BLM. The formation of the BLM-Ru-O-Ru-BLM dimeric unit, similar to that found for sterically unhindered Ru porphyrins, seems to be the most likely.

Solution-state NMR investigations of triosephosphate isomerase active site loop motion: ligand release in relation to active site loop dynamics

Product release is partially rate determining in the isomerization reaction catalyzed by Triosephosphate Isomerase, the conversion of dihydroxyacetone phosphate to D-glyceraldehyde 3-phosphate, probably because an active-site loop movement is necessary to free the product from confinement in the active-site. The timescale of the catalytic loop motion and of ligand release were studied using 19F and 31P solution-state NMR. A 5'-fluorotryptophan was incorporated in the loop N-terminal hinge as a reporter of loop motion timescale. Crystallographic studies confirmed that the structure of the fluorinated enzyme is indistinguishable from the wild-type; the fluorine accepts a hydrogen bond from water and not from a protein residue, with minimal perturbation to the flexible loop stability. Two distinct loop conformations were observed by 19F NMR. Both for unligated (empty) and ligated enzyme samples a single species was detected, but the chemical shifts of these two distinct species differed by 1.2 ppm. For samples in the presence of subsaturating amounts of a substrate analogue, glycerol 3-phosphate, both NMR peaks were present, with broadened lineshapes at 0 degrees C. In contrast, a single NMR peak representing a rapid average of the two species was observed at 30 degrees C. We conclude that the rate of loop motion is less than 1400 s(-1) at 0 degrees C and more than 1400 s(-1) at 30 degrees C. Ligand release was studied under similar sample conditions, using 31P NMR of the phosphate group of the substrate analogue. The rate of ligand release is less than 1000 s(-1) at 0 degrees C and more than 1000 s(-1) at 30 degrees C. Therefore, loop motion and product release are probably concerted and likely to represent a rate limiting step for chemistry.

Conserved residues in the mechanism of the E. coli Class II FBP-aldolase

The two classes of fructose-1,6-bisphosphate aldolase both catalyse the reversible cleavage of fructose 1,6-bisphosphate into dihydroxyacetone phosphate and glyceraldehyde 3-phosphate. The Class I aldolases use Schiff base formation as part of their catalytic mechanism, whereas the Class II enzymes are zinc-containing metalloproteins. The mechanism of the Class II enzymes is less well understood than their Class I counterparts. We have combined sequence alignments of the Class II family of enzymes with examination of the crystal structure of the enzyme to highlight potentially important aspartate and asparagine residues in the enzyme mechanism. Asp109, Asp144, Asp288, Asp290, Asp329 and Asn286 were targeted for site-directed mutagenesis and the resulting proteins purified and characterised by steady-state kinetics using either a coupled assay system to study the overall cleavage reaction or using the hexacyanoferrate (III) oxidation of the enzyme bound intermediate carbanion to investigate partial reactions. The results showed only minor changes in the kinetic parameters for the Asp144, Asp288, Asp290 and Asp329 mutants, suggesting that these residues play only minor or indirect roles in catalysis. By contrast, mutation of Asp109 or Asn286 caused 3000-fold and 8000-fold decreases in the kcat of the reaction, respectively. Coupled with the kinetics measured for the partial reactions the results clearly demonstrate a role for Asn286 in catalysis and in binding the ketonic end of the substrate. Fourier transform infra-red spectroscopy of the wild-type and mutant enzymes has further delineated the role of Asp109 as being critically involved in the polarisation of the carbonyl group of glyceraldehyde 3-phosphate.

Phosphorus-31 nuclear magnetic resonance spectroscopy reveals two conformational forms of chloroacetol phosphate-bound triosephosphate isomerase

Chloroacetol phosphate covalently reacts with Glu-165 in the catalytic center of triosephosphate isomerase. Reaction of the enzyme with the substrate analogue results in two 31P resonances at 6.8 and 5.5 ppm. Dissociation with guanidinium chloride results in a single resonance at 4.5 ppm. Reassociation and redimerization of the triosephosphate isomerase-chloroacetol phosphate complex restores only the resonance at 5.5 ppm. The two 31P resonances appear to represent different conformations of the enzyme which are trapped upon reaction with the affinity label.

Polarization of substrate carbonyl groups by yeast aldolase: investigation by Fourier transform infrared spectroscopy

The infrared spectrum of the complex of D-fructose 1,6-bisphosphate bound to yeast aldolase displays three spectral features between 1700 and 1800 cm-1. One of these (at 1730 cm-1) corresponds to the carbonyl group of enzyme-bound D-fructose 1,6-bisphosphate and/or dihydroxyacetone phosphate. The frequency of this band, which is unaffected by the removal of the intrinsic zinc ion from the enzyme, demonstrates that this carbonyl group is not significantly polarized when the substrate binds to the enzyme. In contrast, the spectral band assigned to the carbonyl group of enzyme-bound D-glyceraldehyde 3-phosphate (at 1706 cm-1) appears at a frequency 24 cm-1 lower than when this substrate is in aqueous solution. This shift indicates considerable polarization of the carbonyl group when D-glyceraldehyde 3-phosphate is bound at the active site. The third spectral feature (at 1748 cm-1), which is observed only in the presence of potassium ion, probably corresponds to an enzymic carboxyl group in a nonpolar environment.

31P NMR studies on the interaction of deoxyuridylate with thymidylate synthase

The 31P nuclear magnetic resonance signal of deoxyuridylate was studied in the presence and absence of thymidlate synthase. In the absence of enzyme the chemical shift of deoxyuridylate is pH dependent with a pKa of 6.25. In the presence of enzyme, a peak corresponding to the dianioinc form of deoxyuridylate is observed which is independent of pH between pH 5.7 and pH 7.4. The pKa of the phosphate in the deoxyuridylate-thymidylate synthase complex is therefore less than 5. The release of inorganic phosphate from deoxyuridylate catalyzed by contaminating phosphatase was also observed.