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Nuclear Quantum Tunneling in the Light-activated Enzyme Protochlorophyllide Oxidoreductase

2008; Elsevier BV; Volume: 284; Issue: 6 Linguagem: Inglês

10.1074/jbc.m808548200

1083-351X

Derren J. Heyes, Michiyo Sakuma, Sam P. de Visser, Nigel S. Scrutton,

Photochemistry and Electron Transfer Studies

In chlorophyll biosynthesis, the light-activated enzyme protochlorophyllide oxidoreductase catalyzes trans addition of hydrogen across the C-17–C-18 double bond of the chlorophyll precursor protochlorophyllide (Pchlide). This unique light-driven reaction plays a key role in the assembly of the photosynthetic apparatus, but despite its biological importance, the mechanism of light-activated catalysis is unknown. In this study, we show that Pchlide reduction occurs by dynamically coupled nuclear quantum tunneling of a hydride anion followed by a proton on the microsecond time scale in the Pchlide excited and ground states, respectively. We demonstrate the need for fast dynamic searches to form degenerate “tunneling-ready” configurations within the lifetime of the Pchlide excited state from which hydride transfer occurs. Moreover, we have found a breakpoint at -27 °C in the temperature dependence of the hydride transfer rate, which suggests that motions/vibrations that are important for promoting light-activated hydride tunneling are quenched below -27 °C. We observed no such breakpoint for the proton-tunneling reaction, indicating a reliance on different promoting modes for this reaction in the enzyme-substrate complex. Our studies indicate that the overall photoreduction of Pchlide is endothermic and that rapid dynamic searches are required to form distinct tunneling-ready configurations within the lifetime of the photoexcited state. Consequently, we have established the first important link between photochemical and nuclear quantum tunneling reactions, linked to protein dynamics, in a biologically significant system. In chlorophyll biosynthesis, the light-activated enzyme protochlorophyllide oxidoreductase catalyzes trans addition of hydrogen across the C-17–C-18 double bond of the chlorophyll precursor protochlorophyllide (Pchlide). This unique light-driven reaction plays a key role in the assembly of the photosynthetic apparatus, but despite its biological importance, the mechanism of light-activated catalysis is unknown. In this study, we show that Pchlide reduction occurs by dynamically coupled nuclear quantum tunneling of a hydride anion followed by a proton on the microsecond time scale in the Pchlide excited and ground states, respectively. We demonstrate the need for fast dynamic searches to form degenerate “tunneling-ready” configurations within the lifetime of the Pchlide excited state from which hydride transfer occurs. Moreover, we have found a breakpoint at -27 °C in the temperature dependence of the hydride transfer rate, which suggests that motions/vibrations that are important for promoting light-activated hydride tunneling are quenched below -27 °C. We observed no such breakpoint for the proton-tunneling reaction, indicating a reliance on different promoting modes for this reaction in the enzyme-substrate complex. Our studies indicate that the overall photoreduction of Pchlide is endothermic and that rapid dynamic searches are required to form distinct tunneling-ready configurations within the lifetime of the photoexcited state. Consequently, we have established the first important link between photochemical and nuclear quantum tunneling reactions, linked to protein dynamics, in a biologically significant system. Hydrogen transfer reactions are fundamental chemical processes that are essential for almost all biological reactions. H-transfer by tunneling is an important feature of these reactions in enzymes (1Kohen A. Cannio R. Bartolucci S. Klinman J.P. Nature.. 1999; 399: 496-499Google Scholar, 2Garcia-Viloca M. Gao J. Karplus M. Truhlar D.G. Science.. 2004; 303: 186-195Google Scholar, 3Masgrau L. Roujeinikova A. Johannissen L.O. Hothi P. Basran J. Ranaghan K.E. Mulholland A.J. Sutcliffe M.J. Scrutton N.S. Leys D. Science.. 2006; 312: 237-241Google Scholar), but mechanistic understanding of how protein motions (from the millisecond to sub-picosecond time domain) facilitate the H-tunneling reactions remains elusive (4Benkovic S.J. Hammes-Schiffer S. Science.. 2003; 301: 1196-1202Google Scholar, 5Benkovic S.J. Hammes-Schiffer S. Science.. 2006; 312: 208-209Google Scholar, 6Boehr D.D. McElheny D. Dyson H.J. Wright P.E. Science.. 2006; 313: 1638-1642Google Scholar). A major limitation has been the inability to synchronously trigger catalysis on ultrafast time scales for the majority of enzymes that require mixing strategies to initiate the reaction. However, by using the light-activated enzyme, protochlorophyllide oxidoreductase (POR 4The abbreviations used are: POR, NADPH:protochlorophyllide oxidoreductase; Pchlide, protochlorophyllide; Chlide, chlorophyllide; KIE, kinetic isotope effect; SIE, solvent isotope effect; DFT, density functional theory. ; EC 1.3.1.33) (7Heyes D.J. Hunter C.N. Trends Biochem. Sci.. 2005; 30: 642-649Google Scholar), we have triggered two enzymatic H-transfer reactions using a single pulse of light, and we show these reactions occur sequentially by quantum tunneling in a pre-formed enzyme-substrate complex. This has provided a unique opportunity to analyze these reactions at physiological and cryogenic temperatures, on very fast time scales, that are experimentally inaccessible with other enzyme systems. POR catalyzes the trans addition of hydrogen across the C-17–C-18 double bond of the chlorophyll precursor protochlorophyllide (Pchlide) to produce chlorophyllide (Chlide) (7Heyes D.J. Hunter C.N. Trends Biochem. Sci.. 2005; 30: 642-649Google Scholar), a unique light-driven reaction in the synthesis of the most abundant pigment on earth, which plays a key role in the assembly of the photosynthetic apparatus (8Lebedev N. Timko M.P. Photosyn. Res.. 1998; 58: 5-23Google Scholar, 9Aronsson H. Sundqvist C. Dahlin C. Plant Mol. Biol.. 2003; 51: 1-7Google Scholar). In addition to POR, nonflowering land plants, algae, and cyanobacteria possess a light-independent Pchlide reductase, which consists of three separate subunits and allows these organisms to produce Chlide in the dark (10Bröcker M.J. Virus S. Ganskow S. Heathcote P. Heinz D.W. Schubert W.D. Jahn D. Moser J. J. Biol. Chem.. 2008; 283: 10559-10567Google Scholar). However, despite its biological significance, the detailed mechanism of this light-activated catalysis remains poorly understood. Low temperature spectroscopy has identified a number of steps in the reaction cycle, including an initial light-driven reaction (11Heyes D.J. Ruban A.V. Wilks H.M. Hunter C.N. Proc. Natl. Acad. Sci. U. S. A.. 2002; 99: 11145-11150Google Scholar, 12Heyes D.J. Heathcote P. Rigby S.E.J. Palacios M.A. van Grondelle R. Hunter C.N. J. Biol. Chem.. 2006; 281: 26847-26853Google Scholar) and subsequent dark reactions (13Heyes D.J. Ruban A.V. Hunter C.N. Biochemistry.. 2003; 42: 523-528Google Scholar, 14Heyes D.J. Hunter C.N. Biochemistry.. 2004; 43: 8265-8271Google Scholar, 15Heyes D.J. Sakuma M. Scrutton N.S. J. Biol. Chem.. 2007; 282: 32015-32020Google Scholar). In the reaction, reduction of Pchlide by NADPH in the POR-NADPH-Pchlide complex involves hydride transfer from the pro-S face of NADPH to the C-17 atom of Pchlide (16Begley T.P. Young H. J. Am. Chem. Soc.. 1989; 111: 3095-3096Google Scholar). The valence of the C-18 atom is satisfied by the transfer of a proton from a conserved Tyr residue (Fig. 1), a finding based on previous site-directed mutagenesis studies (17Wilks H.M. Timko M.P. Proc. Natl. Acad. Sci. U. S. A.. 1995; 92: 724-728Google Scholar) and the structural homology model of the Synechocystis enzyme (18Townley H.E. Sessions R.B. Clarke A.R. Dafforn T.R. Griffiths W.T. Proteins.. 2001; 44: 329-335Google Scholar). The remaining dark reactions involve a series of ordered product release and cofactor binding steps, which are linked to conformational changes in the enzyme (13Heyes D.J. Ruban A.V. Hunter C.N. Biochemistry.. 2003; 42: 523-528Google Scholar, 14Heyes D.J. Hunter C.N. Biochemistry.. 2004; 43: 8265-8271Google Scholar, 15Heyes D.J. Sakuma M. Scrutton N.S. J. Biol. Chem.. 2007; 282: 32015-32020Google Scholar). In addition, previous ultrafast measurements on POR have revealed that spectral changes on the picosecond time scale are likely to represent conformational changes that occur before the reduction of Pchlide (19Heyes D.J. Hunter C.N. van Stokkum I.H. van Grondelle R. Groot M.L. Nat. Struct. Biol.. 2003; 10: 491-492Google Scholar, 20Dietzek B. Kiefer W. Hermann G. Popp J. Schmitt M. J. Phys. Chem. B.. 2006; 110: 4399-4406Google Scholar, 21Zhao G.J. Han K.L. Biophys. J.. 2008; 94: 38-46Google Scholar, 22Sytina O. Heyes D.J. Hunter C.N. Alexandre M.T. van Stokkum I.H.M. van Grondelle R. Groot M.L. Nature.. 2008; 456: 1001-1004Google Scholar). Moreover, prior excitation with a laser pulse leads to a more efficient conformation of the active site and an enhancement in the catalytic efficiency of the enzyme (22Sytina O. Heyes D.J. Hunter C.N. Alexandre M.T. van Stokkum I.H.M. van Grondelle R. Groot M.L. Nature.. 2008; 456: 1001-1004Google Scholar). However, a detailed description of the light-driven chemical steps is currently lacking. To access this chemistry we have now synchronized the turnover of the POR-NADPH-Pchlide complex (assembled in the dark) by using a 6-ns laser pulse tuned to the Soret region of the Pchlide absorbance spectrum for analysis in the nanosecond to microsecond time domain. We have combined kinetic analysis with studies of both the temperature and isotopic dependence of the rate of hydride and proton transfer to derive information on the mechanism of H-transfer in the photoexcited state of the ternary enzyme-substrate complex. Sample Preparation—Recombinant POR from Thermosynechococcus elongatus was overexpressed in Escherichia coli and purified as described (14Heyes D.J. Hunter C.N. Biochemistry.. 2004; 43: 8265-8271Google Scholar). Pchlide was purified as described (14Heyes D.J. Hunter C.N. Biochemistry.. 2004; 43: 8265-8271Google Scholar). Deuterated pro-S NADPH (NADP2H) was purified and analyzed for chemical and isotopic purity as described (23Pudney C.R. Hay S. Sutcliffe M.J. Scrutton N.S. J. Am. Chem. Soc.. 2006; 128: 14053-14058Google Scholar). Solvent isotope effects were measured using deuterated buffer systems made with D2O, d8-glycerol (both Goss Scientific), and deuterated sucrose, which was produced by exchange into D2O. For solvent isotope effect measurements, POR was deuterated by exchange into a deuterated buffer system containing 50 mm Tris, pH 7.5, 100 mm NaCl, and 1 mm dithiothreitol. Laser Photoexcitation Measurements—Photoexcitation of POR ternary complexes (POR-NADPH-Pchlide) was by excitation at 450 nm, using an optical parametric oscillator of a Q-switched Nd-YAG laser (Brilliant B, Quantel) in a cuvette of 1-cm path length as described (15Heyes D.J. Sakuma M. Scrutton N.S. J. Biol. Chem.. 2007; 282: 32015-32020Google Scholar). Laser pulses (∼60 mJ) were between 6 and 8 ns in duration. Absorption transients were recorded at 696 and 681 nm using an LKS-60 flash photolysis instrument (Applied Photophysics Ltd.) with the detection system (comprising probe light, first monochromator, sample, second monochromator, and photomultiplier) at right angles to the incident laser beam. Rate constants were observed from the average of at least five time-dependent absorption measurements by fitting to a single exponential function. For studies of the temperature dependence of rate constants, reaction components were assembled in the dark in a volume of 1 ml and contained 100 μm POR (or deuterated enzyme), 250 μm NADPH (or NADP2H), and 30 μm Pchlide in 44% glycerol and 20% sucrose containing 50 mm Tris-HCl, pH 7.5, 0.1% Genapol, 0.1% β-mercaptoethanol. Control experiments in the absence of any cryoprotectant confirmed that the respective kinetic and solvent isotope effects were not influenced by the presence of glycerol or sucrose. Density Functional Theory (DFT) Calculations—Calculations followed previous procedures (24de Visser S.P. J. Am. Chem. Soc.. 2006; 128: 9813-9824Google Scholar) and used the hybrid density functional method B3LYP (25Becke A.D. J. Chem. Phys.. 1993; 98: 5648-5652Google Scholar) in combination with a 6-311+G* basis set on all atoms (26Hehre W.J. Ditchfield R. Pople J. J. Chem. Phys.. 1972; 56: 2257-2261Google Scholar). Full geometry optimizations were performed in Jaguar 7.0 with a dielectric constant of ϵ = 5.7 included using the self-consistent reaction field model (27Schrödinger LLC Jaguar 7.0. Schrödinger LLC, Portland, OR2007Google Scholar). The theoretical model for the reduction of the C-17–C-18 bond of Pchlide contains the pigment without side chains, except for the propionate chain that is attached to C-17, which is replaced by an ethyl group to keep the overall charge of the model neutral. In addition, the nicotinamide ring of NADPH and phenol (for the Tyr-193 side chain) was added to the model, and they function as hydride and proton donors, respectively. To prevent the NADPH and phenol groups from undergoing excessive changes during the geometry optimizations, a constraint was placed on one of the atoms of each group with respect to the magnesium atom of the Pchlide. This did not cause any problems during the geometry optimization. The total model had stoichiometry of MgC36N6H30O3 and overall charge of 0. All calculations followed established procedures in the field (24de Visser S.P. J. Am. Chem. Soc.. 2006; 128: 9813-9824Google Scholar) and use the hybrid density functional method B3LYP (25Becke A.D. J. Chem. Phys.. 1993; 98: 5648-5652Google Scholar), as implemented in Jaguar 7.0 (27Schrödinger LLC Jaguar 7.0. Schrödinger LLC, Portland, OR2007Google Scholar) in combination with 6-311+G* basis set on all atoms (26Hehre W.J. Ditchfield R. Pople J. J. Chem. Phys.. 1972; 56: 2257-2261Google Scholar). Structures were fully optimized in Jaguar, followed by an analytical frequency calculation. Obtained gas-phase results predicted a stepwise reaction process via a radical intermediate between two consecutive hydrogen abstraction reactions, which is in disagreement with the experiment. We subsequently added a dielectric constant of ϵ = 5.7 in combination with a probe radius of 2.72 Å, as is commonly used for theoretical studies of enzyme mechanism and has been shown to be a good representative of environmental perturbations generated by an enzyme (28Shaik S. Kumar D. de Visser S.P. Altun A. Thiel W. Chem. Rev.. 2005; 105: 2279-2328Google Scholar, 29de Visser S.P. Oh K. Han A.-R. Nam W. Inorg. Chem.. 2007; 46: 4632-4641Google Scholar). Calculations, with a dielectric constant incorporated, predicted the charge distributions of intermediates and products that are consistent with sequential hydride and proton transfer. Therefore, only results in which a dielectric constant was included were used for the final calculations. Despite the large electronic differences between the gas-phase and solvent-based calculations, the differences in optimized geometries were actually quite small. The solvent optimized structures have little radical character, and hence the group spin densities are close to zero. Sequential Kinetic Mechanism for Hydride and Proton Transfer—Photoexcitation of the POR-NADPH-Pchlide complex generates an intermediate at 696 nm (Fig. 2A) with a rate constant of 2.02 ± 0.21 × 106 s-1 at 25 °C. Similar traces obtained between 665 and 720 nm define the “action spectrum” for this step (Fig. 2A, inset) and reveal that this species is identical to the intermediate observed in earlier studies (11Heyes D.J. Ruban A.V. Wilks H.M. Hunter C.N. Proc. Natl. Acad. Sci. U. S. A.. 2002; 99: 11145-11150Google Scholar), thus providing the first direct kinetic link to previous cryogenic measurements. In addition, this step has a primary kinetic isotope effect (KIE) of ∼2, when measurements are repeated with pro-S NADP2H, which confirms that the hydride transfer reaction from coenzyme to Pchlide (Fig. 1, reaction A) is significantly faster than any other reported hydride transfer reaction in biology. At longer times following laser initiation of catalysis, the 696 nm trace decays over ∼100 μs (rate constant = 25.3 ± 1.5 × 103 s-1 at 25 °C; Fig. 2B) and is accompanied by an absorbance increase at 681 nm with a similar rate constant (Fig. 2C). Action spectra, generated from a series of kinetic traces (wavelength range 660–720 nm), confirm that the new intermediate has an absorbance peak centered at ∼680 nm (Fig. 2B, inset), which has previously been shown to represent the POR-NADP+-Chlide product complex (13Heyes D.J. Ruban A.V. Hunter C.N. Biochemistry.. 2003; 42: 523-528Google Scholar, 14Heyes D.J. Hunter C.N. Biochemistry.. 2004; 43: 8265-8271Google Scholar). A solvent isotope effect (SIE) of ∼2.2 at 25 °C was measured for this step, implying that it represents the proton transfer reaction (Fig. 1, reaction B). Importantly, the SIE associated with reaction A is close to unity, which suggests that the SIE on the second step is a specific probe of proton transfer to substrate. Also, the lack of a KIE in reaction B indicates that hydride transfer only occurs during reaction A (Table 1) and provides conclusive proof of a sequential hydride transfer followed by proton transfer mechanism.TABLE 1The rates of the hydride transfer and proton transfer steps in the presence of either pro-S NADPH or S-NADP2H and in either H2O or 2H2O buffers All rates were measured at 25 °C as described under “Experimental Procedures.”SampleHydride transferProton transferRateKIERateSIEs–1 × 106s–1 × 103NADPH in H2O2.02 ± 0.21125.3 ± 1.51NADP2H in H2O1.00 ± 0.142.03 ± 0.3525.6 ± 3.10.99 ± 0.14NADPH in 2H2O1.79 ± 0.221.13 ± 0.1811.5 ± 1.12.20 ± 0.24NADP2H in 2H2O0.89 ± 0.122.25 ± 0.3810.6 ± 0.42.39 ± 0.17 Open table in a new tab Both H-transfer Reactions Proceed via Quantum Mechanical Tunneling—We extended our analysis of hydride and proton transfer to cover a wide temperature range (-80 °C to +50 °C), and in particular to cryogenic temperatures, a regime that is difficult for thermally activated enzyme systems that require mixing methods for reaction initiation. Data were analyzed in the form of Eyring plots (Fig. 3), which provides thermodynamic parameters for each step (Tables 2 and 3) and reveals that both H-transfer reactions proceed by quantum mechanical tunneling. The proton transfer rate is strongly dependent on temperature (ΔH‡ = 74.8 kJ mol-1), and the SIE is temperature-dependent with an inverse extrapolated Eyring prefactor ratio (A′H/A′D = 0.041) (Fig. 3A and Table 2). This is consistent with a proton-tunneling reaction, which requires fast (sub-picosecond) promoting motions coupled to the reaction coordinate (30Knapp M.J. Klinman J.P. Eur. J. Biochem.. 2002; 269: 3113-3121Google Scholar, 31Masgrau L. Basran J. Hothi P. Sutcliffe M.J. Scrutton N.S. Arch. Biochem. Biophys.. 2004; 428: 41-51Google Scholar) within the model for environmentally coupled hydrogen tunneling (32Kuznetsov A.M. Ulstrup J. Can. J. Chem.. 1999; 77: 1085-1096Google Scholar, 33Knapp M.J. Ricert K. Klinman J.P. J. Am. Chem. Soc.. 2002; 124: 3865-3874Google Scholar). This involves motion to achieve the reactant and product well degeneracy required for tunneling, and gated motion along the H-transfer coordinate (indicated by the temperature dependence of the KIE) to enhance nuclear wave function overlap for the transferring proton (30Knapp M.J. Klinman J.P. Eur. J. Biochem.. 2002; 269: 3113-3121Google Scholar, 31Masgrau L. Basran J. Hothi P. Sutcliffe M.J. Scrutton N.S. Arch. Biochem. Biophys.. 2004; 428: 41-51Google Scholar). The lack of a breakpoint in the Eyring plot suggests that the gated motion is coupled to the proton tunneling coordinate at all temperatures studied (-80 °C to +50 °C).TABLE 2Thermodynamic parameters for the proton transfer step in the POR-catalyzed reaction The enthalpies of activation, ΔH‡, and the entropies of activation, ΔS‡, have been calculated by fitting the temperature dependence data to the Eyring equation for each step.H2OD2OΔH‡ (kJ mol–1)74.8 ± 0.884.6 ± 0.3ΔΔH‡ (kJ mol–1)9.8 ± 0.8ΔS‡ (J mol–1 K–1)65.7 ± 0.892.2 ± 0.4lnA′31.7 ± 0.434.9 ± 0.1A′H/A′D0.041 ± 0.016 Open table in a new tab TABLE 3Thermodynamic parameters for the hydride transfer step in the POR-catalyzed reaction The enthalpies of activation, ΔH‡, and the entropies of activation, ΔS‡, have been calculated by fitting the temperature dependence data to the Eyring equation for each step.Above –27 °CBelow –27 °CNADPHNADPDNADPHNADPDΔH‡ (kJ mol–1)9.3 ± 0.417.5 ± 0.527.2 ± 0.527.7 ± 0.9ΔΔH‡ (kJ mol–1)8.2 ± 0.60.4 ± 1.0ΔS‡ (J mol–1 K–1)–94.4 ± 1.2–73.2 ± 1.1–21.8 ± 0.3–32.4 ± 0.8lnA′12.4 ± 0.215.0 ± 0.221.1 ± 0.319.9 ± 0.5A′H/A′D0.08 ± 0.023.6 ± 2.0 Open table in a new tab By contrast, the faster light-activated hydride transfer step shows a clear breakpoint at -27 °C in the Eyring plot with both protiated and deuterated NADPH (Fig. 3B). Above -27 °C the reaction has a relatively weak temperature dependence (ΔH‡ = 9.3 kJ mol-1 for NADPH) but becomes considerably more temperature-dependent below the breakpoint (ΔH‡ = 27.2 kJ mol-1) (Table 3). At temperatures below the breakpoint, the KIE is measurably independent of temperature, and the prefactor ratio (A′H/A′D = 3.59) is similar in value to the observed KIE, indicating quantum tunneling of hydride in the absence of an experimentally detectable (i.e. dominant) gating motion, coupled to the hydride transfer coordinate (3Masgrau L. Roujeinikova A. Johannissen L.O. Hothi P. Basran J. Ranaghan K.E. Mulholland A.J. Sutcliffe M.J. Scrutton N.S. Leys D. Science.. 2006; 312: 237-241Google Scholar, 34Johannissen L.O. Hay S. Scrutton N.S. Sutcliffe M.J. J. Phys. Chem. B.. 2007; 111: 2631-2638Google Scholar). This contrasts with the situation at temperatures above -27 °C, where the KIE is dependent on temperature and the prefactor ratio is less than unity (A′H/A′D = 0.077), consistent with the need for a more dominant gating motion along the hydride transfer coordinate (30Knapp M.J. Klinman J.P. Eur. J. Biochem.. 2002; 269: 3113-3121Google Scholar). DFT Calculations Confirm the Catalytic Mechanism—To gain further insights into the reaction mechanism, we set up a theoretical model representing the important features of the system (Fig. 4; supplemental Fig. S1). We have assumed a starting reactant complex (R) that involves Pchlide forming a long range complex with NADPH and the phenol group of the Tyr proton donor. Full geometry optimizations were performed in a dielectric constant of magnitude ϵ = 5.7, which has been shown to correctly predict the values of an enzyme-mimicked environment (35Blomberg L.M. Blomberg M.R.A. Siegbahn P.E.M. J. Biol. Inorg. Chem.. 2004; 9: 923-935Google Scholar, 36de Visser S.P. Inorg. Chem.. 2006; 45: 9551-9557Google Scholar). The overall reaction mechanism is endothermic (63.9 kJ mol-1) and involves hydride transfer from NADPH to the C-17 atom of Pchlide to give an intermediate (I) via transition state TS1, followed by the subsequent proton transfer reaction to form the product complex (P) via barrier TS2. A time-dependent density functional theory calculation (37Frisch M.J. Trucks G.W. Schlegel H.B. Scuseria G.E. Robb M.A. Cheeseman J.R. Montgomery Jr., J.A. Vreven T. Kudin K.N. Burant J.C. Millam J.M. Iyengar S.S. Tomasi J. Barone V. Mennucci B. Cossi M. Scalmani G. Rega N. Petersson G.A. Nakatsuji H. Hada M. Ehara M. Toyota K. Fukuda R. Hasegawa J. Ishida M. Nakajima T. Honda Y. Kitao O. Nakai N. Klene M. Li X. Knox J.E. Hratchian H.P. Cross J.B. Adamo C. Jaramillo J. Gomperts R. Stratmann R.E. Yazyev O. Austin A.J. Cammi R. Pomelli C. Ochterski J.W. Ayala P.Y. Morokuma K. Voth G.A. Salvador P. Dannenberg J.J. Zakrzewski V.G. Dapprich S. Daniels A.D. Strain M.C. Farkas O. Malick D.K. Rabuck A.D. Raghavachari K. Foresman J.B. Ortiz J.V. Cui Q. Baboul A.G. Clifford S. Cioslowski J. Stefanov B.B. Liu G. Liashenko A. Piskorz P. Komaromi I. Martin R.L. Fox D.J. Keith T. Al-Laham M.A. Peng C.Y. Nanayakkara A. Challacombe M. Gill P.M.W. Johnson B. Chen W. Wong M.W. Gonzalez C. Pople J.A. Gaussian-03. Revision C.01, Gaussian, Inc, Wallingford, CT2004Google Scholar) on the reactant geometry shows that a close manifold of electronic states is accessible with the lowest Franck-Condon transition located at 210 kJ mol-1 (2.18 eV). The system then has sufficient energy to cross the hydride transfer barrier via quantum mechanical tunneling and relax back to the ground state potential energy surface to form the intermediate complex. The subsequent barrier (ΔG‡ = 67.7 kJ mol-1 at 298 K) of the proton transfer step, leading to product formation, is of much lower energy on the ground state potential energy surface and is in excellent agreement with the experimental data shown above in Fig. 3. Charge distributions (Fig. 4) confirm that the I is formed by hydride transfer, generating a positively charged NADP+ group (QNADPH = 1.16) and a double negatively charged Pchlide (QPchlide =-2.09), consistent with a change in hybridization (sp2 to sp3) for the C-17 atom of Pchlide. The theoretical reaction energetics agree closely with those observed from our temperature dependence studies of the hydride and proton transfer kinetics (Table 2 and Table 3) and confirm that the light-activated sequential transfer of hydride (excited state) and proton (ground state) is an appropriate chemical mechanism for the POR-catalyzed reduction of Pchlide. Our theoretical model demonstrates the need for light activation to drive an overall endothermic reaction from the Pchlide excited state. A consequence is that a dynamic search for “tunneling-ready” configurations (i.e. reactant configurations in which donor and acceptor wells become degenerate (23Pudney C.R. Hay S. Sutcliffe M.J. Scrutton N.S. J. Am. Chem. Soc.. 2006; 128: 14053-14058Google Scholar)) must occur within the lifetime of the photoexcited state. Significantly, there is a loss of amplitude for the hydride and proton transfer signals at lower temperatures (Fig. 3C), which suggests that dynamic searches for the tunneling-ready configuration are impeded as the temperature is reduced and that relaxation from the excited state becomes dominant. This model is supported by the presence of the -27 °C breakpoint for the hydride transfer reaction. Below the breakpoint, the lack of a measurable temperature dependence on the KIE implies that quenching of gated motion along the hydride transfer coordinate will impede hydride tunneling as the wavefunction overlap becomes less optimal (30Knapp M.J. Klinman J.P. Eur. J. Biochem.. 2002; 269: 3113-3121Google Scholar, 31Masgrau L. Basran J. Hothi P. Sutcliffe M.J. Scrutton N.S. Arch. Biochem. Biophys.. 2004; 428: 41-51Google Scholar). In addition, the observed increase in the temperature dependence of the hydride transfer rate below the transition point reflects the increased energetic cost of tunneling in the absence of an “assisting” motion coupled to the hydride transfer coordinate. By necessity, this implies that the system rarely reaches a tunneling-ready conformation, but when it does, it is at an ideal donor-acceptor distance. Conclusions—In conclusion, we have established a direct link between light-activated chemistry and nuclear tunneling in a biologically important enzyme system. Furthermore, by extending our studies of light activation to cryogenic regimes, we have shown that gated motion along the H-transfer coordinate enhances the tunneling reaction. In contrast to the slower dynamic searches that generally limit H-transfer rates in thermally activated enzyme systems (1Kohen A. Cannio R. Bartolucci S. Klinman J.P. Nature.. 1999; 399: 496-499Google Scholar, 38Basran J. Sutcliffe M.J. Scrutton N.S. Biochemistry.. 1999; 38: 3218-3222Google Scholar, 39Hammes-Schiffer S. Benkovic S.J. Annu. Rev. Biochem.. 2006; 75: 519-541Google Scholar), we have demonstrated that fast dynamic searches within the lifetime of the excited state are required to reach a tunneling-ready configuration. Viewed globally, light-driven nuclear tunneling enables photosynthetic organisms to make chlorophyll despite the large and opposing thermodynamic gradient for this crucial reaction. The National Service of Computational Chemistry Software is acknowledged for providing valuable CPU time. Download .pdf (.15 MB) Help with pdf files