Skip to main content
NIHPA Author Manuscripts logoLink to NIHPA Author Manuscripts
. Author manuscript; available in PMC: 2015 Feb 5.
Published in final edited form as: J Am Chem Soc. 2014 Feb 18;136(8):2930–2939. doi: 10.1021/ja500215j

Long-Range Electron Tunneling

Jay R Winkler 1,, Harry B Gray 1,
PMCID: PMC3986022  NIHMSID: NIHMS564426  PMID: 24499470

Abstract

Electrons have so little mass that in less than a second they can tunnel through potential energy barriers that are several electron-volts high and several nanometers wide. Electron tunneling is a critical functional element in a broad spectrum of applications, ranging from semiconductor diodes to the photosynthetic and respiratory charge transport chains. Prior to the 1970s, chemists generally believed that reactants had to collide in order to effect a transformation. Experimental demonstrations that electrons can transfer between reactants separated by several nanometers led to a revision of the chemical reaction paradigm. Experimental investigations of electron exchange between redox partners separated by molecular bridges have elucidated many fundamental properties of these reactions, particularly the variation of rate constants with distance. Theoretical work has provided critical insights into the superexchange mechanism of electronic coupling between distant redox centers. Kinetics measurements have shown that electrons can tunnel about 2.5 nm through proteins on biologically relevant timescales. Longer-distance biological charge flow requires multiple electron tunneling steps through chains of redox cofactors. The range of phenomena that depends on long-range electron tunneling continues to expand, providing new challenges for both theory and experiment.


The propensity of light particles to tunnel through potential energy barriers was recognized early in the development of quantum mechanics. At first the phenomenon was exclusively the purview of physicists: in January, 1928, Oppenheimer invoked electron tunneling (although not by name) through a potential barrier to explain electric-field-induced emission from atoms;1 five months later, Fowler and Nordheim published their landmark work describing field-induced electron emission from cold metals;2 then, in September, 1928, Gurney and Condon rationalized α-particle decay in terms of tunneling;3 and two months later Gamow published a quantitative tunneling model that closely reproduced the empirical Geiger-Nuttal relationship between α-decay lifetime and particle energy.4

Solid-state physicists discovered the importance of tunneling in the middle of the 20th century. Many of the new devices developed by the rapidly expanding semiconductor electronics industry depended on electrons tunneling through potential energy barriers. In 1934, Clarence Zener formulated a theory of field-induced electron tunneling between energy bands in solid dielectrics.5 The semiconductor devices developed 15 years later at Bell labs appeared to exhibit this phenomenon, leading William Shockley to name them Zener diodes.6 Later, Leo Esaki found that thin heavily doped p-n junctions exhibited negative resistance in the low-voltage regime (tunnel diodes), a phenomenon readily explained by quantum mechanical tunneling of electrons through the junction.7 Today the physics of semiconductors is understood in great detail, owing to the vigorous interplay between theory and experiment that has occurred over many years. And, in recent years, the electronics industry has begun to move to the nanoscale to take advantage of groundbreaking work in conducting polymers,811 molecular wires,12 and molecular electronic devices.1316

Chemistry

In the final third of the 20th century, chemists began to explore the role of electron tunneling in reactions between molecular species. The semiclassical theory of electron-transfer (ET) (eq. 1) reactions

kET=4π3h2λkBTHAB2exp(-(ΔG°+λ)24λkBT) (1)

formulated by, inter alia, Marcus,17,18 Levich, and Dogonadze19 provided a theoretical underpinning for countless experimental investigations. The theory expresses the specific rate of ET between two weakly interacting redox centers held at fixed distance and orientation in terms of the standard free-energy change for the reaction (ΔG°), a parameter describing the extent of nuclear reorientation and reorganization accompanying electron transfer (λ), and the electronic coupling strength between reactants and products at the transition-state nuclear configuration (HAB). The exponential factor reflects the probability of forming the activated complex for the reaction; HAB2 describes the probability of electron tunneling from donor to acceptor in the activated complex.

The Gaussian free-energy dependence of the specific rate is a unique feature of homogeneous electron transfer reactions and, in favorable cases, rates are observed to decrease as driving forces increase beyond λ (inverted effect) (Figure 1). The fact that energy-saving charge-separation reactions in photosynthetic reaction centers are faster than energy-wasting recombination processes has been rationalized in terms of inverted effects.20,21 Often, however, inverted behavior is masked by the production of electronically excited products so that rates tend to plateau at high driving forces. Marcus recognized that chemiluminescent electron-transfer reactions are a manifestation of inverted driving-force effects.22 Rate-limiting diffusion of reactants in bimolecular ET reactions further frustrated the search for inverted behavior. The fluorescence quenching work of Rehm and Weller is likely the best known example of this phenomenon.23 Because of these obstacles, some of the earliest observations of inverted driving-force effects were found in return electron transfer reactions in photogenerated geminate radical pairs,24 as well as in bimolecular return reactions.25 Ultimately, molecules with electron donors and acceptors linked by covalent bonds were prepared and ET kinetics measurements produced several unequivocal demonstrations of inverted behavior.26,27 The theory leading to eq. 1 treats nuclear motions classically. Quantum mechanical refinements indicate that reorganization in high-frequency vibrational modes will substantially attenuate the magnitude of the inverted effect (Figure 1).2832

Figure 1.

Figure 1

Theoretical driving-force dependence of electron transfer reactions (T = 295 K). Classical treatment of nuclear rearrangements (blue) based on λ = 0.8 eV(ref. 18). The intersecting parabolas represent reactant (red) and product (green) potential energy surfaces along the reaction coordinate for normal (left), optimized (middle), and inverted (right) driving forces. A quantum mechanical treatment (cyan: one classical mode, λ = 0.5 eV; one quantum mode, λ = 0.3 eV, ħω = 1500 cm−1) predicts damped inverted behavior (ref. 32).

A common approach to overcome the diffusion problem involved immobilization of electron donors and acceptors in rigid solvents. Reactions were initiated pulse radiolytically33 or photochemically3439 and kinetics were interpreted in terms of random distributions of redox partners.4042 Two parameters were extracted from the data: a rate constant for ET at close contact ( kETo); and an exponential distance decay constant β(kET=kEToe-β(r-r0)) that describes the efficiency of long-range coupling. In square barrier tunneling models, β depends on the height of the barrier and the effective electron mass.43 Although square-barrier tunneling models accurately predict the exponential distance dependence of long-range ET reactions, they provide no insight into how the properties of the bridging medium determine the coupling strength.

Superexchange tunneling models gained favor over geometric barrier models because they describe long-range couplings in terms of the electronic structure of the intervening medium. The theory of superexchange interactions, formulated first by Kramers44 and later by Anderson,45 rationalized interactions between magnetic centers separated by nonmagnetic ions. Halpern and Orgel generalized the superexchange theory to describe inner-sphere electron transfer processes,46 and McConnell used perturbation theory to elaborate the model for electron donor-acceptor molecules separated by an oligomeric bridge composed of j identical repeat units (Figure 2).47 McConnell’s familiar result (eq. 2)

Figure 2.

Figure 2

Orbital diagram representation of the states mediating electron-transfer superexchange coupling. The electron transfers from the orbital on the left to an equivalent one on the right. Electronic coupling can be mediated by excess electron (e coupling) or hole states (h+ coupling on the intervening bridge.

HAB=hDbΔε(hbbΔε)j-1hbA (2)

describes HAB in terms of the energy gap between electron (or hole) states on the donor (or acceptor) and electron (or hole) states of the bridging medium (Δε) and the coupling strengths between: the donor and the bridge hole or electron states (hDb); the acceptor and the bridge states (hbA); and adjacent bridge states (hbb). The theory predicts that HAB will be an exponential function of j and, hence, that rates will be exponential functions of donor-acceptor distance (r), in agreement with geometric barrier models. Taking the length of a bridge element as δ, the empirical distance decay constant can be defined in terms of superexchange parameters (eq. 3).

β=-2δln(hbbΔε) (3)

Measurements of ET in rigid solvents are readily interpreted in terms of superexchange coupling models. Following work by Ponce,38 Wenger found that β depended on the properties of the glass: 25% aqueous H2SO4, 16.0(5) nm−1; 2-methyl-tetrahydrofuran (2-MTHF), 16.2(5) nm−1; toluene, 12.3(5) nm−1 (Figure 3).39 The coupling efficiencies indicate that electron tunneling through 2.5 nm of toluene is several thousand times faster than tunneling across the same distance in 2-MTHF or 25% aqueous H2SO4. The smaller energy gaps (Δε) to electron or hole states of toluene, compared to the analogous gaps for 2-MTHF or 25% H2SO4, likely account for the variation in β values. The decay constant for tunneling through an oligoxylene bridged donor-acceptor pair was found to be 7.6(5) nm−1;39 tunneling across 2.5 nm of this bridge would be over ten thousand times faster than tunneling through toluene. The likely explanation for this difference is that the coupling mediated by the C-C bond between xylene rings (hbb) is substantially greater than that associated with van der Waals contacts between toluene molecules in the solvent glass.

Figure 3.

Figure 3

Distance dependence of rate constants for electron tunneling through solvent glasses (2-MTHF, blue; 25% aqueous H2SO4, cyan; toluene, green) and across oligoxylene bridges (red) (refs. 38, 39).

The appealing simplicity of eqs 2 and 3 conceals some quantitative difficulties with the one-electron nearest-neighbor superexchange model. Several studies of ET across saturated alkane bridges,26,4850 particularly in self-assembled monolayers (SAM) of normal alkanes on gold electrodes, have produced β values of ~10 nm−1 (Figure 4).5153 Taking δ = 0.154 nm leads to the estimate hbbΔε0.5, a value that barely fulfills McConnell’s perturbation theory requirements (i.e., |hbb|Δε1). Direct measurements of hbb and Δε are not feasible, but spectroscopic data can provide insights into their relative magnitudes. Estimates of energy gaps to hole states are relatively straightforward. The gas-phase ionization energies of saturated alkanes decrease as the number of carbon atoms increases: C2H6, IE(adiabatic) = 11.52 eV; C11H24, 9.65 eV (Figure 5).54,55 This progression is consistent with modest delocalization of σ-bonding electrons as the carbon backbone lengthens. The ferricenium/ferrocene (Fc+/Fc) redox couple was used in much of the alkane SAM work, and valence photoelectron spectra have been measured for this archetypal organometallic compound. The vertical ionization energy of Fc is 6.88 eV,56 but this is not the quantity of interest. Since the electronic coupling matrix element in eq. 1 corresponds to the transition-state nuclear configuration, the adiabatic ionization energy (~6.65 eV) is more appropriate (Supporting Information). Consequently, the gas-phase energy gaps for Fc+/Fc hole tunneling across alkane spacers (n-CjH2j+2 j = 5–11) range from 3.6 to 2.9 eV.

Figure 4.

Figure 4

Distance dependence of Arrhenius prefactors for electron transfer reactions between a Au electrode and redox couples attached to the termini of oligomethylene (directly linked Fc, ●; ester-linked Fc, ○; Ru(pyridine)(NH3)52+, ▽) and oligovinylene (×) spacers. For distances >12 Å (1.2 nm), oligomethylene rates are described by an exponential distance decay of 10.6 nm−1 (solid line). The dotted line shows the prefactor expected for reactions limited by solvent dyanmics. (Reprinted from ref. 51 with permission from the American Chemical Society, copyright 2003.)

Figure 5.

Figure 5

Gas-phase vertical (○) and adiabatic (●) ionization energies for normal saturated hydrocarbons (refs. 54, 55). The dashed line corresponds to the adiabatic ionization energy of ferrocene (ref. 56).

In condensed phases, the energy gaps are likely to shift somewhat, owing to polarization of the surrounding medium. Photoconductivity measurements indicate that ionization thresholds of saturated hydrocarbons decrease by about 1.5 eV upon moving from gas to liquid phases.57 The binding energy of the tunneling electron for the ferricenium/ferrocene redox couple (E° = 0.4 V vs. NHE)58 is near 4.9 eV, suggesting that Δε is in the range of 3.9-3.1 eV for condensed-phase, normal alkane bridges.

Estimation of energy gaps for electron tunneling is more problematic. A naïve approach involves estimation of the LUMO energy of a molecular bridge on the basis of its absorption and ionization spectra. The onset of far UV (FUV) absorption in gaseous and liquid normal alkanes (n-CjH2j+2 j = 5–14) is near 8 eV.5963 The maxima found in liquids between 8.45 and 8.18 eV, and the shoulders near 7.7 eV have been assigned to electronic excitations of σ-bonding electrons into Rydberg-type orbitals (3p and 3s, respectively).63 Taking 7.7 eV for the HOMO-LUMO energy gap, along with the gas-phase ionization energies of saturated alkanes, place LUMO energies 2.6-1.9 eV below the vacuum level.

The diabatic states that would mediate coupling for electron transfer, however, do not correlate directly with those observed in valence-shell or Rydberg absorption spectra. The appropriate states for electron tunneling are anion states of the bridging molecule.64 In an m-electron molecule, the electron promoted to the LUMO in a valence-shell excited state sees an effective potential produced by m−1 electrons. The effective potential seen by the excess electron in an anion created from an m-electron parent, however, is produced by m electrons. The consequence is that the extra electrons in anions are very weakly bound, or not even bound at all. Indeed, negative electron affinities are extracted from resonances in electron transmission spectra (ETS) of many organic molecules.65,66 Only very broad (~4–5 eV) ETS resonances, indicative of extremely short lived anion states, have been detected in the 7–9 eV range for saturated alkanes.67 States so far above the vacuum level seem unlikely to assist long-range electronic coupling between donors and acceptors separated by alkane spacers.

Ab initio calculations of gas-phase electronic couplings across saturated alkane spacers provide interesting comparisons to the experimental quantities.6870 In a Natural Bond Orbital (NBO) basis,71,72 intrabridge coupling elements (hbb) between C-C σ-bonding orbitals in trans-n-alkane spacers are estimated to be ~2.7 eV.68,69 The energy gaps depend on the redox partner chosen for the calculations. For alkane-bridged methylene cation and anion radicals ([H2C-(CH2)j-CH2]±), Δε values of ~8 eV emerged from the calculations for both hole tunneling in the cations and electron tunneling in the anions.68,69 Experimental data suggest a somewhat smaller gap for hole tunneling: the vertical ionization energy of the ethyl radical (H3C–CH2) is 8.1 eV; its electron affinity is −0.26 eV.7375 Substituting the theoretical values in eq. 3 would suggest β ~ 14 nm−1, but the full calculation gave β ~ 5–7 nm−1 for transfer in [H2C-(CH2)j-CH2]+.69 Clearly, the McConnell model does not capture all contributions to the coupling matrix element; a principal source of the discrepancy lies in the inclusion of only nearest-neighbor interactions. Ratner demonstrated that the McConnell model could be generalized to give HAB as a sum of the contributions from all pathways.76 Since the coupling is a signed quantity, this extended McConnell model admitted the possibility of constructive and destructive interference from competing coupling routes. Ab initio calculations of coupling along trans-n-alkane spacers revealed that non-nearest-neighbor coupling pathways make substantial constructive contributions to the total coupling between donors and acceptors.6870 Moreover, pathways involving antibonding orbitals of the alkane contributed to the calculated couplings for the cations; HAB was neither exclusively hole nor electron mediated. These studies indicated that although nearest-neighbor McConnell pathways did not lead to accurate estimates of long-range couplings, more coarsely-grained effective pathways based on larger repeat units could be represented by a McConnell-type model.69

The energy gaps to hole and electron states of saturated alkane bridges are extremely large for most conventional redox reagents. The same cannot be said for many unsaturated hydrocarbon bridges. Moreover, the decrease in energy gap with increasing bridge length complicates analyses of distance dependences. When the energy gaps become small, incoherent hopping through real redox intermediates begins to compete with coherent single-step long-range tunneling.7779 Wasielewski and coworkers demonstrated that ET across oligo-p-phenylenevinylene bridges (βobsd = 0.4 nm−1) is a case in point.77,78 Analysis of the temperature dependences of these kinetics suggested that hopping is gated by torsional motions involving the donor and the bridge. A similarly shallow distance dependence (βobsd = 0. 6 nm−1) was reported for tunneling from a gold electrode to the Fc+/Fc couple across SAMs composed of oligo-p-phenylenevinylene bridges. In this instance, estimated energy gaps (>1 eV) are larger than observed activation energies (~0.2 eV) and incoherent hopping was ruled out.53 Instead, the weak distance dependence was attributed to dynamically limited, adiabatic ET. It is apparent that the empirical β values for electron transfer across oligo-p-phenylenevinylene bridges in both the small and large energy gap regimes are too small to be consistent with superexchange-mediated tunneling. The surprising finding is that two different mechanisms appear to be responsible for virtually distance-independent transport across this bridge.

Biology

Understanding electron transfer in biological systems has challenged chemists for over half a century. Szent-Györgyi, in attempting to rationalize electron transport in respiratory chains, suggested that electrons move among enzymes in energy bands, analogous to transport in semiconductors.80 This proposal met considerable opposition,8183 although no suitable alternative appeared for more than 25 years. In 1966, De Vault and Chance reported that rates of cytochrome oxidation in flash-irradiated suspensions of photosynthetic bacteria reached a limiting value (τ ~ 2 ms) as the temperature decreased below 100 K; and they suggested that quantum mechanical tunneling was the explanation.84 Without structural information and a precise understanding of the ET reaction, little more could be concluded. Eight years later, Hopfield developed a thermally activated tunneling model to describe the De Vault and Chance data.85 He postulated a 2-eV barrier height, leading to a 14.4-nm−1 distance decay constant, and a predicted 0.8-nm tunneling distance.

Definitive evidence for long-range electron tunneling through proteins emerged in 1982 from our work on cytochrome c modified with a RuIII(NH3)5 moiety coordinated to His33 on the protein surface (Ru(His33)-Fe-cyt c).86 In a kinetics study, flash photochemical electron injection generated transient RuII(His33)-FeIII-cyt c that relaxed to the RuIII-FeII thermodynamic product with a time constant of 30 ms (−ΔG° = 0.2 eV). Structural models placed the electron transfer distance at 1.8 nm; tunneling was the only plausible explanation. Irrefutable evidence of long-range tunneling was provided by measurements of intramolecular ET reactions in protein crystals.8789 The advent of site-directed mutagenesis and several experimental refinements developed over the ensuing years ultimately produced an experimentally validated timetable for long-range electron tunneling through proteins (Figure 6).9092 We have measured the kinetics of high-driving-force ET in more than 30 Ru-labeled proteins: donor-acceptor distances vary from 1.2 to 2.6 nm and specific rates span seven orders of magnitude (109 to 102 s−1). Driving-force-optimized rate constants are dispersed around an exponential distance decay of 11 nm−1, but the substantial scatter reflects important features of the protein medium.9094

Figure 6.

Figure 6

Distance dependence of driving-force-optimized ET rate constants for Ru-modified proteins: azurin (blue); cytochrome c (red); myoglobin (magenta); cytochrome b562 (green); high-potential iron protein (cyan) (ref. 90).

A comparison between the distance dependence of ET through n-alkane spacers embedded in SAMs and that of Ru-proteins is illuminating. Arrhenius prefactors (roughly equivalent to driving-force-optimized homogeneous rate constants) for 10 ET rate measurements across n-alkanes in SAMs vary over six orders of magnitude (109 to 103 s−1) in the 1.2–2.5 nm distance range with a nearly perfect exponential distance dependence (β = 10.6 nm−1).53 The standard deviation for SAM data is less than a factor of two (1.8), whereas that for the Ru-protein data is a factor of 8. Clearly, the n-alkane spacers embedded in SAMs are extremely well-ordered structures that create a uniform barrier to long-range tunneling. Within the Ru-protein data set are examples where rate constants differ by a factor of 103 at the same donor-acceptor distance, and virtually identical rates are found for distances differing by 0.5 nm.9092 The inescapable conclusion to be drawn from the protein data is that folded polypeptide matrices do not create a uniform barrier to electron tunneling. This conclusion is entirely consistent with investigations of electron tunneling through solvent glasses. Long-range coupling efficiencies are sensitive functions of the chemical composition of the glass (βtoluene < βH2SO4 ~ β2-MTHF), and covalent linkages are superior to van der Waals contacts (βoligo-xylenetoluene).39

The sidechains of the twenty amino acids have widely varying molecular and electronic structures, and polypeptide folds create a heterogeneous array of bonded and nonbonded contacts between electron donors and acceptors. When redox partners are oriented along an extended polypeptide, as they are in a β-sheet protein, Ru-azurin, ET rates exhibit a simple exponential distance dependence.9092 But, donor-acceptor couplings mediated by sidechain atoms, hydrogen bonds, and van der Waals contacts will not depend solely on the separation distance; the structure and composition of the intervening medium will play a defining role. Understanding the long-range coupling in a protein, then, is a challenging quantum chemical problem involving a very small energy splitting between reactant and product states (HAB < 10 cm−1) composed of hundreds or thousands of atoms, with multiple coupling modes, interferences, conformational dynamics, and potential breakdown of the Born-Oppenheimer and Condon approximations.95105 Nevertheless, ab initio electronic structure methods combined with molecular dynamics simulations have produced impressive strides in calculations of absolute ET rates in Ru-modified azurins.99,106 A great deal of fundamental information is subsumed in the calculation of protein ET rates. A decomposition of the calculated rates into contributions from electron- and hole-tunneling, and identification of the pathways contributing to the overall coupling, would be especially illuminating.13,107

Two general principles that emerge from studies of ET in glasses can provide insights into the factors that control long-range biological ET reactions: aromatics are better than alkanes and covalent bonds are superior to van der Waals contacts. As efficient long-range electron transfer in DNA (β < 10 nm−1) is facilitated by the high concentration of aromatic bases stacked in the double helix,108110 we anticipate that aromatic amino acids will provide smaller tunneling energy gaps than aliphatic residues in proteins. In support of this view, the ionization energies of aliphatic amino acids (~9.6 eV) are greater than those of aromatic amino acids (Phe, 9.4(1) eV; Tyr, 8.5(1); Trp, 7.8(1)).111113 Vertical electron attachment energies of Phe (0.87 eV) and Trp (0.68 eV) are about 1 eV less than those of Ala and Gly (1.80, 1.93 eV, respectively).114 Assessing the biological implications of the second principle is a difficult prospect, because it requires knowledge of individual protein structures and, in the case of interprotein ET, encounter-complex structures.

With the ready accessibility of protein-sequence databases, it is possible to investigate whether biological ET reactions exploit the presumed greater coupling efficiency of aromatic amino acids. The four aromatic amino acids are among the least frequently occurring residues in the the UniProtKB/Swiss-Prot protein sequence database115 (Phe, 3.90% of all residues, rank = 14; Tyr, 3.00%, 16; His, 2.36%, 18; Trp, 1.13%, 20) and have long been believed to stabilize folded structures, with additional roles in protein-protein recognition and ligand binding.116119 Histidine has additional functional importance, owing to its basicity and preference for metal binding and, for the purposes of the subsequent discussion, is not included in the aromatic class. The average amino-acid frequencies of occurrence in proteins from the six enzyme classes (oxidoreductases, 37,408 sequences; transferases, 89,489; hydrolases, 61,743; lyases, 23,052; isomerases, 14,067; ligases, 30,513) defined by the Enzyme Data Bank of the Swiss Institute of Bioinformatics are illustrated in Figure 7. The striking feature in this comparison is that only among the oxidoreductases do aromatic residues appear more frequently than the database average. With the exception of Tyr in the ligases, aromatic amino acids occur substantially less frequently than database averages in the other five enzyme classes. Analyses of transmembrane protein structures reveal that aromatic amino acids are found preferentially in membrane interface regions; this trend is believed to enhance stability.120122 Separate comparisons of amino acid frequencies in transmembrane and soluble proteins still exhibit higher frequencies of aromatics among the oxidoreductases, although the remaining five enzyme classes show some interesting variations (see Supporting Information). An obvious explanation for the higher frequencies of aromatic amino acids in oxidoreductases is their superior capability to mediate long-range electron transfer. Testing this hypothesis is a challenging prospect; folded polypeptide structures will not tolerate wholesale exchange of aromatic and aliphatic residues. Analyses of the structures and ET properties of proteins with particularly high and low aromatic frequencies might provide some insight into this question. The cytochromes P450 are a case in point (Figure 8): the average Phe occurrence frequency in the P450 family is 45% greater than in the database as a whole; Trp frequencies are higher by 22%. Enhanced superexchange coupling between redox partners and the heme is one rationale for the prevalence of aromatics in this enzyme family.

Figure 7.

Figure 7

Amino-acid occurrence frequencies in the primary sequences of six enzyme classes (oxidoreductases, 37,408 sequences; transferases, 89,489; hydrolases, 61,743; lyases, 23,052; isomerases, 14,067; ligases, 30,513) relative to the average frequencies in the Enzyme Data Bank of the Swiss Institute of Bioinformatics (ref. 115). All bar graphs have identical vertical axis limits

Figure 8.

Figure 8

Amino-acid occurrence frequencies in the primary sequences of the cytochrome P450 family of enzymes (975 sequences) relative to the average frequencies in the Enzyme Data Bank of the Swiss Institute of Bioinformatics (ref. 115).

The exigencies of biological function typically require that electrons be transferred in milliseconds over distances of 5 nm or more, yet it is clear from Figure 6 that single-step ET reactions across more than 2.5 nm cannot keep up with this pace. The solution to the problem is multistep tunneling (hopping): redox centers spaced at ~1.5-nm intervals with formal potentials near those of the terminal donors and acceptors.94,123,124 Indeed, it is likely that the 2-μs cytochrome oxidation in Chromatium vinosum studied by De Vault and Chance in 1966, and analyzed theoretically by Hopfield in 1974, was a two-step tunneling reaction.125 The structure of the photosynthetic reaction center in Chromatium has not been determined, but the Blastochloris viridis (formerly Rhodopseudomonas viridis) enzyme has an analogous string of four cytochromes126,127 (c554, E°(FeIII/II) = –0.07 V; vs. NHE; c556, E° = 0.32(1) V; c552, E° = 0.02(1) V; c559, E° = 0.38(1) V) that deliver electrons to the oxidized bacteriochlorophyll special pair (P+, E°(P+/0) = 0.5 V).125,128,129 The kinetics of P+ reduction in two-electron reduced (FeII-c556, FeII-c559) B. viridis reaction centers are biphasic: a 200 ns phase has been assigned to FeII-c559 → P+ ET and a 2 μs process is attributed to FeII-c556 → FeIII-c559 ET.125,130 The Fe-Fe distance between c556 and c559 is 2.78 nm (PDB #2I5N),131 too far for a 2-μs single-step ET reaction. Cytochrome c552 lies between c556 and c559 with Fe-Fe distances of 1.65 (c556 - c552) and 1.39 nm (c552 - c559). EPR measurements indicate that the FeIII hemes in c554, c556, and c552 are strongly coupled. Owing to electrostatic interactions among the cytochromes, it is difficult to determine precisely the driving forces for FeII-c556 → FeIII-c552 and FeII-c552 → FeIII-c559 ET reactions but, on the basis of formal potentials extracted from redox titrations, it is likely that the 2-step transfer from FeII-c556 to FeIII-c559 involves an endergonic first step and a spontaneous second step.128,129 Redox chains that facilitate charge separation across biological membranes have been identified in several components of the photosynthetic and respiratory machinery.94,128,132

Multistep biological electron tunneling need not always depend on redox-active metallo-cofactors. Perhaps the best-known example is the Class I ribonucleotide reductase in which a hole resides on a stable Tyr122 radical in the resting state of the E. coli enzyme.133142 A chain of Tyr and Trp residues is believed to mediate electron transfer from an active site Cys439 residue to Tyr122 over a distance of more than 3.5 nm. Multistep ET reactions via Trp and Tyr have been identified in several other natural systems: photosystem II, 143146 DNA photolyase, 147155 MauG156159 and the cytochrome c/cytochrome c peroxidase pair160,161.

The natural hopping systems are not as amenable to systematic variations as are sensitizer-modifed proteins. We examined the fundamental principles of multistep tunneling in a Re-modified azurin mutant engineered to have a Trp directly between Re and Cu centers separated by 1.9 nm. CuI oxidation by electronically excited ReI was accelerated by a factor of more than 100 in this mutant; replacement of Trp by Tyr or Phe inhibited CuI oxidation.162 Hopping maps based on semiclassical ET theory have been used to identify potential locations for redox intermediates (Int) in Ru-modified azurins.163 The greatest hopping advantage is predicted for azurins in which the Int-RuIII distance is up to 0.5 nm shorter than that for Int-CuI. The hopping advantage increases as systems orient nearer a “straight-line” between the donor and acceptor, a consequence of minimizing intermediate tunneling distances. The smallest predicted hopping advantage occurs when the Ru-Cu distance is less than 2 nm. Analyses of ET kinetics measurements in three CuI-Int-RuIII azurins (Int = nitrotyrosinate) revealed that hopping via NO2-TyrO accelerates CuI oxidation by factors of ~10–50, results that are fully consistent with the predictions of semiclassical theory.163

Generation of oxidized Trp and Tyr radicals requires high potential oxidants (E° > 1 V vs. NHE), so that they are likely to participate only in a relatively small subset of enzymatic transformations. The enzymatic reactions in which oxygen serves as an electron acceptor typically involve high-potential intermediates. Examination of the amino-acid occurrence frequencies in O2- and H2O2-reactive oxidoreductases (5961 sequences) reveals that Trp and Tyr are found much more often than the database average (Figure 9) (see Supporting Information for additional comparisons). The involvement of Trp and Tyr radicals in ET reactions is one explanation for the prevalence of these residues in this class of enzymes. We speculate that, in addition to participation in on-pathway ET chains, Trp and Tyr radicals also might play protective roles in O2-reactive oxidoreductases. If these enzymes do not operate with high fidelity or if xenobiotics inhibit natural function, the high-potential intermediates generated during turnover can produce reactive species that damage and inactivate enzymes.164166 Appropriately placed Tyr and/or Trp residues could prevent this damage by reducing the intermediates and directing the oxidizing hole to less harmful sites or out of the protein altogether. Devising methods to identify and detect protective biochemical mechanisms of this sort is an ongoing research challenge in biological electron transfer.167

Figure 9.

Figure 9

Amino-acid occurrence frequencies in the primary sequences of O2- and H2O2-reactive oxidoreductases (7149 sequences) relative to the average frequencies in the Enzyme Data Bank of the Swiss Institute of Bioinformatics (ref. 115).

How far can they go?

Tremendous advances in theory and experiment during the past half-century have produced a rigorous foundation for understanding long-range electron transfers in chemistry and biology. Yet, many fundamental problems remain to be solved. Superexchange is generally agreed to be the dominant, but not exclusive, coupling mechanism for long-range ET, although the mediating states and energy gaps are rarely identified,13,107,168 nor are they correlated with the spectroscopic and thermodynamic properties of the bridging medium. Indeed, the uncertainty about energy gaps often leads to confusion about competition between coherent tunneling and incoherent hopping.

Empirical studies of long-range electron transport continue to challenge the current paradigm. A particularly interesting example is provided by bacterial nanowires. Groups of microbes are known that transfer electrons to extracellular FeIII oxides.169 Many of these bacteria contact the oxides via micron-long hairlike appendages known as pili. Some pili are coated with multiheme c-type cytochromes that have been suggested to serve as hopping intermediates in micron-distance electron transport processes.170 Alternative interpretations, however, suggest that the pilus itself has metal-like conductive properties in the absence of the cytochromes.171 Beratan and coworkers have pointed out that superexchange tunneling theories impose severe constraints on these hyper-long-range ET processes.172 New insights into the ET properties of pili continue to emerge, but it remains to be clearly determined how this remarkable transport of electrons is accomplished.

Supplementary Material

Supporting Information

Acknowledgments

Our electron transfer research is supported by the National Institutes of Health (DK-019038), the National Science Foundation (CHE-1305124), the Gordon and Betty Moore Foundation, and the Arnold and Mabel Beckman Foundation.

Footnotes

Supporting Information

Estimation of the gas-phase Fc+/Fc electron exchange tunneling energy and additional comparisons of amino-acid occurrence frequencies. This material is available free of charge via the Internet at http://pubs.acs.org.

Contributor Information

Jay R. Winkler, Email: winklerj@caltech.edu.

Harry B. Gray, Email: hbgray@caltech.edu.

References

  • 1.Oppenheimer JR. Phys Rev. 1928;31:66–81. [Google Scholar]
  • 2.Fowler RH, Nordheim L. Proc R Soc Lond A. 1928;119:173–81. [Google Scholar]
  • 3.Gurney RW, Condon EU. Nature. 1928;122:439. [Google Scholar]
  • 4.Gamow G. Nature. 1928;122:805–6. [Google Scholar]
  • 5.Zener C. Proc R Soc Lond A. 1934;145:523–9. [Google Scholar]
  • 6.It was later discovered that the breakdown properties of these devices arose, not from field induced tunneling but from avalanche breakdown. Diodes operating according to Zener’s model were developed later (Morton DL, Gabriel J. Electronics: The Life Story of a Technology. Johns Hopkins University Press; 2007. ).
  • 7.Esaki L. Phys Rev. 1958;109:603–4. [Google Scholar]
  • 8.Shirakawa H. Angew Chem, Int Ed Eng. 2001;40:2575–80. [Google Scholar]
  • 9.MacDiarmid AG. Angew Chem, Int Ed Eng. 2001;40:2581–90. doi: 10.1002/1521-3773(20010716)40:14<2581::AID-ANIE2581>3.0.CO;2-2. [DOI] [PubMed] [Google Scholar]
  • 10.Heeger AJ. Angew Chem, Int Ed Eng. 2001;40:2591–611. [PubMed] [Google Scholar]
  • 11.Hutchison GR, Ratner MA, Marks TJ. J Phys Chem B. 2005;109:3126–38. doi: 10.1021/jp046579v. [DOI] [PubMed] [Google Scholar]
  • 12.Weiss EA, Wasielewski MR, Ratner MA. In: Molecular Wires: From Design to Properties. DeCola L, editor. Vol. 257. 2005. pp. 103–33. [Google Scholar]
  • 13.Solomon GC, Bergfield JP, Stafford CA, Ratner MA. Beilstein J Nanotechnol. 2011;2:862–71. doi: 10.3762/bjnano.2.95. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 14.Ratner M. Nature Nanotechnology. 2013;8:378–81. doi: 10.1038/nnano.2013.110. [DOI] [PubMed] [Google Scholar]
  • 15.Renaud N, Hliwa M, Joachim C. Unimolecular and Supramolecular Electronics II: Chemistry and Physics Meet at Metal-Molecule Interfaces. 2012;313:217–68. [Google Scholar]
  • 16.Li C, Mishchenko A, Wandlowski T. Unimolecular and Supramolecular Electronics II: Chemistry and Physics Meet at Metal-Molecule Interfaces. 2012;313:121–88. doi: 10.1007/128_2011_238. [DOI] [PubMed] [Google Scholar]
  • 17.Marcus RA. J Chem Phys. 1956;24:966–78. [Google Scholar]
  • 18.Marcus RA, Sutin N. Biochim Biophys Acta. 1985;811:265–322. [Google Scholar]
  • 19.Levich VG, Dogonadze RR. Doklady Akademii Nauk SSSR. 1959;124:123–6. [Google Scholar]
  • 20.Volk M, Aumeier G, Langenbacher T, Feick R, Ogrodnik A, Michel-Beyerle ME. J Phys Chem B. 1998;102:735–51. [Google Scholar]
  • 21.Bixon M, Jortner J. J Phys Chem. 1991;95:1941–4. [Google Scholar]
  • 22.Marcus RA. J Chem Phys. 1965;43:2654–7. [Google Scholar]
  • 23.Rehm D, Weller A. Isr J Chem. 1970;8:259–71. [Google Scholar]
  • 24.Gould IR, Ege D, Mattes SL, Farid S. J Am Chem Soc. 1987;109:3794–6. [Google Scholar]
  • 25.McCleskey TM, Winkler JR, Gray HB. J Am Chem Soc. 1992;114:6935–7. [Google Scholar]
  • 26.Closs GL, Calcaterra LT, Green NJ, Penfield KW, Miller JR. J Phys Chem. 1986;90:3673–83. [Google Scholar]
  • 27.Fox LS, Kozik M, Winkler JR, Gray HB. Science. 1990;247:1069–71. doi: 10.1126/science.247.4946.1069. [DOI] [PubMed] [Google Scholar]
  • 28.Jortner J. J Chem Phys. 1976;64:4860–7. [Google Scholar]
  • 29.Dogonadze RR, Kuznetsov AM, Vorotyntsev MA. Phys Status Solidi B. 1972;54:125–34. [Google Scholar]
  • 30.Dogonadze RR, Kuznetsov AM, Vorotyntsev MA. Phys Status Solidi B. 1972;54:425–33. [Google Scholar]
  • 31.Ulstrup J, Jortner J. J Chem Phys. 1975;63:4358–68. [Google Scholar]
  • 32.Brunschwig BS, Sutin N. Comments Inorg Chem. 1987;6:209–35. [Google Scholar]
  • 33.Miller JR. Science. 1975;189:221–2. doi: 10.1126/science.189.4198.221. [DOI] [PubMed] [Google Scholar]
  • 34.Miller JR, Hartman KW, Abrash S. J Am Chem Soc. 1982;104:4296–8. [Google Scholar]
  • 35.Strauch S, McLendon G, McGuire M, Guarr T. J Phys Chem. 1983;87:3579–81. [Google Scholar]
  • 36.Dorfman RC, Lin Y, Fayer MD. J Phys Chem. 1989;93:6388–96. [Google Scholar]
  • 37.Lin Y, Dorfman RC, Fayer MD. J Chem Phys. 1989;90:159–70. [Google Scholar]
  • 38.Ponce A, Gray HB, Winkler JR. J Am Chem Soc. 2000;122:8187–91. [Google Scholar]
  • 39.Wenger OS, Leigh BS, Villahermosa RM, Gray HB, Winkler JR. Science. 2005;307:99–102. doi: 10.1126/science.1103818. [DOI] [PubMed] [Google Scholar]
  • 40.Inokuti M, Hirayama F. J Chem Phys. 1965;43:1978–89. [Google Scholar]
  • 41.Tachiya M, Mozumder A. Chem Phys Lett. 1974;28:87–9. [Google Scholar]
  • 42.Blumen A. J Chem Phys. 1980;72:2632–40. [Google Scholar]
  • 43.Gurney RW, Condon EU. Phys Rev. 1929;33:127–40. [Google Scholar]
  • 44.Kramers HA. Physica. 1934;1:182–92. [Google Scholar]
  • 45.Anderson PW. Phys Rev. 1950;79:350–6. [Google Scholar]
  • 46.Halpern J, Orgel LE. Disc Faraday Soc. 1960:32–41. [Google Scholar]
  • 47.McConnell HM. J Chem Phys. 1961;35:508–15. [Google Scholar]
  • 48.Oevering H, Paddon-Row MN, Heppener M, Oliver AM, Cotsaris E, Verhoeven JW, Hush NS. J Am Chem Soc. 1987;109:3258–69. [Google Scholar]
  • 49.Beebe JM, Engelkes VB, Liu JQ, Gooding J, Eggers PK, Jun Y, Zhu XY, Paddon-Row MN, Frisbie CD. J Phys Chem B. 2005;109:5207–15. doi: 10.1021/jp044630p. [DOI] [PubMed] [Google Scholar]
  • 50.Wold DJ, Frisbie CD. J Am Chem Soc. 2001;123:5549–56. doi: 10.1021/ja0101532. [DOI] [PubMed] [Google Scholar]
  • 51.Smalley JF, Finklea HO, Chidsey CED, Linford MR, Creager SE, Ferraris JP, Chalfant K, Zawodzinsk T, Feldberg SW, Newton MD. J Am Chem Soc. 2003;125:2004–13. doi: 10.1021/ja028458j. [DOI] [PubMed] [Google Scholar]
  • 52.Smalley JF, Feldberg SW, Chidsey CED, Linford MR, Newton MD, Liu YP. J Phys Chem. 1995;99:13141–9. [Google Scholar]
  • 53.Newton MD, Smalley JF. Phys Chem Chem Phys. 2007;9:555–72. doi: 10.1039/b611448b. [DOI] [PubMed] [Google Scholar]
  • 54.Lias SG, Bartmess JE, Liebman JF, Holmes JL, Levin RD, Mallard WG. J Phys Chem Ref Data. 1988;17:1–861. [Google Scholar]
  • 55.Bieri G, Burger F, Heilbronner E, Maier JP. Helv Chim Acta. 1977;60:2213–33. [Google Scholar]
  • 56.Evans S, Green MLH, Orchard AF, Jewitt B, Pygall CF. J Chem Soc, Faraday Trans II. 1972;68:1847–65. [Google Scholar]
  • 57.Casanovas J, Grob R, Delacroix D, Guelfucci JP, Blanc D. J Chem Phys. 1981;75:4661–8. [Google Scholar]
  • 58.Bard AJ, Parsons R, Jordan J, editors. Standard Potentials in Aqueous Solution. Marcel Dekker, Inc; New York: 1985. [Google Scholar]
  • 59.Raymonda JW, Simpson WT. J Chem Phys. 1967;47:430–48. [Google Scholar]
  • 60.Au JW, Cooper G, Burton GR, Olney TN, Brion CE. Chem Phys. 1993;173:209–39. [Google Scholar]
  • 61.Costner EA, Long BK, Navar C, Jockusch S, Lei X, Zimmerman P, Campion A, Turro NJ, Willson CG. J Phys Chem A. 2009;113:9337–47. doi: 10.1021/jp903435c. [DOI] [PubMed] [Google Scholar]
  • 62.Tachibana S, Morisawa Y, Ikehata A, Sato H, Higashi N, Ozaki Y. Appl Spectrosc. 2011;65:221–6. [Google Scholar]
  • 63.Morisawa Y, Tachibana S, Ehara M, Ozaki Y. J Phys Chem A. 2012;116:11957–64. doi: 10.1021/jp307634m. [DOI] [PubMed] [Google Scholar]
  • 64.Simons J. J Phys Chem A. 2008;112:6401–511. doi: 10.1021/jp711490b. [DOI] [PubMed] [Google Scholar]
  • 65.Jordan KD, Burrow PD. Acc Chem Res. 1978;11:341–8. [Google Scholar]
  • 66.Jordan KD, Burrow PD. Chem Rev. 1987;87:557–88. [Google Scholar]
  • 67.Allan M, Andric L. J Chem Phys. 1996;105:3559–68. [Google Scholar]
  • 68.Liang C, Newton MD. J Phys Chem. 1992;96:2855–66. [Google Scholar]
  • 69.Liang C, Newton MD. J Phys Chem. 1993;97:3199–211. [Google Scholar]
  • 70.Shephard MJ, Paddon-Row MN, Jordan KD. Chem Phys. 1993;176:289–304. [Google Scholar]
  • 71.Reed AE, Curtiss LA, Weinhold F. Chem Rev. 1988;88:899–926. [Google Scholar]
  • 72.Weinhold F. J Comp Chem. 2012;33:2363–79. doi: 10.1002/jcc.23060. [DOI] [PubMed] [Google Scholar]
  • 73.Dyke JM, Ellis AR, Keddar N, Morris A. J Phys Chem. 1984;88:2565–9. [Google Scholar]
  • 74.DePuy CH, Gronert S, Barlow SE, Bierbaum VM, Damrauer R. J Am Chem Soc. 1989;111:1968–73. [Google Scholar]
  • 75.Ruscic B, Berkowitz J, Curtiss LA, Pople JA. J Chem Phys. 1989;91:114–21. [Google Scholar]
  • 76.Ratner MA. J Phys Chem. 1990;94:4877–83. [Google Scholar]
  • 77.Davis WB, Ratner MA, Wasielewski MR. Chem Phys. 2002;281:333–46. [Google Scholar]
  • 78.Davis WB, Svec WA, Ratner MA, Wasielewski MR. Nature. 1998;396:60–3. [Google Scholar]
  • 79.Eng MP, Albinsson B. Chem Phys. 2009;357:132–9. [Google Scholar]
  • 80.Szent-Györgyi A. Science. 1941;93:609–11. doi: 10.1126/science.93.2426.609. [DOI] [PubMed] [Google Scholar]
  • 81.Evans MG, Gergely J. Biochim Biophys Acta. 1949;3:188–97. [Google Scholar]
  • 82.Kasha M. Rev Mod Phys. 1959;31:162–9. [Google Scholar]
  • 83.Chance B, Williams GR. Adv Enzymol. 1956;17:65–134. doi: 10.1002/9780470122624.ch2. [DOI] [PubMed] [Google Scholar]
  • 84.De Vault D, Chance B. Biophys J. 1966;6:825–47. doi: 10.1016/s0006-3495(66)86698-5. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 85.Hopfield JJ. Proc Natl Acad Sci USA. 1974;71:3640–4. doi: 10.1073/pnas.71.9.3640. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 86.Winkler JR, Nocera DG, Yocom KM, Bordignon E, Gray HB. J Am Chem Soc. 1982;104:5798–800. [Google Scholar]
  • 87.Crane BR, Di Bilio AJ, Winkler JR, Gray HB. J Am Chem Soc. 2001;123:11623–31. doi: 10.1021/ja0115870. [DOI] [PubMed] [Google Scholar]
  • 88.Tezcan FA, Crane BR, Winkler JR, Gray HB. Proc Natl Acad Sci USA. 2001;98:5002–6. doi: 10.1073/pnas.081072898. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 89.Axelrod HL, Abresch EC, Okamura MY, Yeh AP, Rees DC, Feher G. J Mol Biol. 2002;319:501–15. doi: 10.1016/S0022-2836(02)00168-7. [DOI] [PubMed] [Google Scholar]
  • 90.Gray HB, Winkler JR. Quart Rev Biophys. 2003;36:341–72. doi: 10.1017/s0033583503003913. [DOI] [PubMed] [Google Scholar]
  • 91.Gray HB, Winkler JR. Biochim Biophys Acta - Bioenerg. 2010;1797:1563–72. doi: 10.1016/j.bbabio.2010.05.001. [DOI] [PubMed] [Google Scholar]
  • 92.Winkler JR, Gray HB. Chem Rev. 2013 [Google Scholar]
  • 93.Moser CC, Keske JM, Warncke K, Farid RS, Dutton PL. Nature. 1992;355:796–802. doi: 10.1038/355796a0. [DOI] [PubMed] [Google Scholar]
  • 94.Page CC, Moser CC, Chen X, Dutton PL. Nature. 1999;402:47–52. doi: 10.1038/46972. [DOI] [PubMed] [Google Scholar]
  • 95.Beratan DN, Onuchic JN, Hopfield JJ. J Chem Phys. 1987;86:4488–98. [Google Scholar]
  • 96.Onuchic JN, Beratan DN. J Chem Phys. 1990;92:722–33. [Google Scholar]
  • 97.Beratan DN, Onuchic JN, Winkler JR, Gray HB. Science. 1992;258:1740–1. doi: 10.1126/science.1334572. [DOI] [PubMed] [Google Scholar]
  • 98.Skourtis SS, Balabin I, Kawatsu T, Beratan DN. Proc Natl Acad Sci USA. 2005;102:3552–7. doi: 10.1073/pnas.0409047102. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 99.Prytkova TR, Kurnikov IV, Beratan DN. Science. 2007;315:622–5. doi: 10.1126/science.1134862. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 100.Balabin IA, Beratan DN, Skourtis SS. Phys Rev Lett. 2008:101. doi: 10.1103/PhysRevLett.101.158102. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 101.Gehlen JN, Daizadeh I, Stuchebrukhov AA, Marcus RA. Inorg Chim Acta. 1996;243:271–82. [Google Scholar]
  • 102.Stuchebrukhov AA. J Chem Phys. 1996;105:10819–29. [Google Scholar]
  • 103.Stuchebrukhov AA. J Chem Phys. 1996;104:8424–32. [Google Scholar]
  • 104.Stuchebrukhov AA. Adv Chem Phys. 2001;118:1–44. [Google Scholar]
  • 105.Medvedev ES, Stuchebrukhov AA. Chem Phys. 2004;296:181–92. [Google Scholar]
  • 106.Prytkova TR, Kurnikov IV, Beratan DN. J Phys Chem B. 2005;109:1618–25. doi: 10.1021/jp0457491. [DOI] [PubMed] [Google Scholar]
  • 107.Wohlthat S, Solomon GC, Hush NS, Reimers JR. Theor Chem Acc. 2011;130:815–28. [Google Scholar]
  • 108.Lewis FD, Wasielewski MR. Top Cur Chem. 2004;236:45–65. [Google Scholar]
  • 109.Lewis FD. Isr J Chem. 2013;53:350–65. [Google Scholar]
  • 110.Barton JK, Olmon ED, Sontz PA. Coord Chem Rev. 2011;255:619–34. doi: 10.1016/j.ccr.2010.09.002. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 111.Klasinc L. J Electron Spectrosc Relat Phenom. 1976;8:161–4. [Google Scholar]
  • 112.Plekan O, Feyer V, Richter R, Coreno M, Prince KC. Mol Phys. 2008;106:1143–53. [Google Scholar]
  • 113.Cannington PH, Ham NS. J Electron Spectrosc Relat Phenom. 1983;32:139–51. [Google Scholar]
  • 114.Aflatooni K, Hitt B, Gallup GA, Burrow PD. J Chem Phys. 2001;115:6489–94. [Google Scholar]
  • 115.http://www.uniprot.org/.
  • 116.Burley SK, Petsko GA. Science. 1985;229:23–8. doi: 10.1126/science.3892686. [DOI] [PubMed] [Google Scholar]
  • 117.Karlin S, Zhu ZY, Baud F. Proc Natl Acad Sci USA. 1999;96:12500–5. doi: 10.1073/pnas.96.22.12500. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 118.Thomas A, Meurisse R, Charloteaux B, Brasseur R. Proteins - Struct Func Gen. 2002;48:628–34. doi: 10.1002/prot.10190. [DOI] [PubMed] [Google Scholar]
  • 119.Lanzarotti E, Biekofsky RR, Estrin DA, Marti MA, Turjanski AG. J Chem Inf Model. 2011;51:1623–33. doi: 10.1021/ci200062e. [DOI] [PubMed] [Google Scholar]
  • 120.Yau WM, Wimley WC, Gawrisch K, White SH. Biochemistry. 1998;37:14713–8. doi: 10.1021/bi980809c. [DOI] [PubMed] [Google Scholar]
  • 121.Hong HD, Park S, Jimenez RHF, Rinehart D, Tamm LK. J Am Chem Soc. 2007;129:8320–7. doi: 10.1021/ja068849o. [DOI] [PubMed] [Google Scholar]
  • 122.Ulmschneider MB, Sansom MSP. Biochim Biophys Acta-Biomembr. 2001;1512:1–14. doi: 10.1016/s0005-2736(01)00299-1. [DOI] [PubMed] [Google Scholar]
  • 123.Shih C. PhD Thesis. California Institute of Technology; 2008. [Google Scholar]
  • 124.Warren JJ, Ener ME, Vlček A, Winkler JR, Gray HB. Coord Chem Rev. 2012;256:2478–87. doi: 10.1016/j.ccr.2012.03.032. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 125.Ortega JM, Mathis P. Biochemistry. 1993;32:1141–51. doi: 10.1021/bi00055a020. [DOI] [PubMed] [Google Scholar]
  • 126.Deisenhofer J, Epp O, Miki K, Huber R, Michel H. Nature. 1985;318:618–24. doi: 10.1038/318618a0. [DOI] [PubMed] [Google Scholar]
  • 127.Deisenhofer J, Epp O, Sinning I, Michel H. J Mol Biol. 1995;246:429–57. doi: 10.1006/jmbi.1994.0097. [DOI] [PubMed] [Google Scholar]
  • 128.Alric J, Lavergne J, Rappaport F, Verméglio A, Matsuura K, Shimada K, Nagashima KVP. J Am Chem Soc. 2006;128:4136–45. doi: 10.1021/ja058131t. [DOI] [PubMed] [Google Scholar]
  • 129.Voigt P, Knapp EW. J Biol Chem. 2003;278:51993–2001. doi: 10.1074/jbc.M307560200. [DOI] [PubMed] [Google Scholar]
  • 130.Chen IP, Pathis P, Koepke J, Michel H. Biochemistry. 2000;39:3592–602. doi: 10.1021/bi992443p. [DOI] [PubMed] [Google Scholar]
  • 131.Li L, Mustafi D, Fu Q, Tereshko V, Chen DL, Tice JD, Ismagilov RF. Proc Natl Acad Sci USA. 2006;103:19243–8. doi: 10.1073/pnas.0607502103. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 132.Roessler MM, King MS, Robinson AJ, Armstrong FA, Harmer J, Hirst J. Proc Natl Acad Sci USA. 2010;107:1930–5. doi: 10.1073/pnas.0908050107. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 133.Stubbe J, Nocera DG, Yee CS, Chang MCY. Chem Rev. 2003;103:2167–201. doi: 10.1021/cr020421u. [DOI] [PubMed] [Google Scholar]
  • 134.Sjöberg BM. Struct Bonding. 1997;88:139–73. [Google Scholar]
  • 135.Stubbe J, van der Donk WA. Chem Rev. 1998;98:705–62. doi: 10.1021/cr9400875. [DOI] [PubMed] [Google Scholar]
  • 136.Argirevic T, Riplinger C, Stubbe J, Neese F, Bennati M. J Am Chem Soc. 2012;134:17661–70. doi: 10.1021/ja3071682. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 137.Holder PG, Pizano AA, Anderson BL, Stubbe J, Nocera DG. J Am Chem Soc. 2012;134:1172–80. doi: 10.1021/ja209016j. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 138.Offenbacher AR, Minnihan EC, Stubbe J, Barry BA. J Am Chem Soc. 2013;135:6380–3. doi: 10.1021/ja3032949. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 139.Worsdorfer B, Conner DA, Yokoyama K, Livada J, Seyedsayamdost M, Jiang W, Silakov A, Stubbe J, Bollinger JM, Krebs C. J Am Chem Soc. 2013;135:8585–93. doi: 10.1021/ja401342s. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 140.Yokoyama K, Smith AA, Corzilius B, Griffin RG, Stubbe J. J Am Chem Soc. 2011;133:18420–32. doi: 10.1021/ja207455k. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 141.Offenbacher AR, Burns LA, Sherrill CD, Barry BA. J Phys Chem B. 2013;117:8457–68. doi: 10.1021/jp404757r. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 142.Chang MCY, Yee CS, Nocera DG, Stubbe J. J Am Chem Soc. 2004;126:16702–3. doi: 10.1021/ja044124d. [DOI] [PubMed] [Google Scholar]
  • 143.Boussac A, Rappaport F, Brettel K, Sugiura M. J Phys Chem B. 2013;117:3308–14. doi: 10.1021/jp400337j. [DOI] [PubMed] [Google Scholar]
  • 144.Keough JM, Zuniga AN, Jenson DL, Barry BA. J Phys Chem B. 2013;117:1296–307. doi: 10.1021/jp3118314. [DOI] [PubMed] [Google Scholar]
  • 145.Sjoholm J, Styring S, Havelius KGV, Ho FM. Biochemistry. 2012;51:2054–64. doi: 10.1021/bi2015794. [DOI] [PubMed] [Google Scholar]
  • 146.Tommos C, Babcock GT. Biochim Biophys Acta - Bioenerg. 2000;1458:199–219. doi: 10.1016/s0005-2728(00)00069-4. [DOI] [PubMed] [Google Scholar]
  • 147.Sancar A. Chem Rev. 2003;103:2203–38. doi: 10.1021/cr0204348. [DOI] [PubMed] [Google Scholar]
  • 148.Taylor JS. Acc Chem Res. 1994;27:76–82. [Google Scholar]
  • 149.Li YF, Heelis PF, Sancar A. Biochemistry. 1991;30:6322–9. doi: 10.1021/bi00239a034. [DOI] [PubMed] [Google Scholar]
  • 150.Aubert C, Mathis P, Eker APM, Brettel K. Proc Natl Acad Sci USA. 1999;96:5423–7. doi: 10.1073/pnas.96.10.5423. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 151.Byrdin M, Eker APM, Vos MH, Brettel K. Proc Natl Acad Sci USA. 2003;100:8676–81. doi: 10.1073/pnas.1531645100. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 152.Kodali G, Siddiqui SU, Stanley RJ. J Am Chem Soc. 2009;131:4795–807. doi: 10.1021/ja809214r. [DOI] [PubMed] [Google Scholar]
  • 153.Lukacs A, Eker APM, Byrdin M, Villette S, Pan J, Brettel K, Vos MH. J Phys Chem B. 2006;110:15654–8. doi: 10.1021/jp063686b. [DOI] [PubMed] [Google Scholar]
  • 154.Woiczikowski PB, Steinbrecher T, Kubař T, Elstner M. J Phys Chem B. 2011;115:9846–63. doi: 10.1021/jp204696t. [DOI] [PubMed] [Google Scholar]
  • 155.Aubert C, Vos MH, Mathis P, Eker APM, Brettel K. Nature. 2000;405:586–90. doi: 10.1038/35014644. [DOI] [PubMed] [Google Scholar]
  • 156.Davidson VL, Liu AM. Biochim Biophys Acta - Proteins Proteomics. 2012;1824:1299–305. doi: 10.1016/j.bbapap.2012.01.008. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 157.Geng JF, Dornevil K, Davidson VL, Liu AM. Proc Natl Acad Sci USA. 2013;110:9639–44. doi: 10.1073/pnas.1301544110. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 158.Yukl ET, Liu FG, Krzystek J, Shin S, Jensen LMR, Davidson VL, Wilmot CM, Liu AM. Proc Natl Acad Sci USA. 2013;110:4569–73. doi: 10.1073/pnas.1215011110. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 159.Davidson VL, Wilmot CM. Annu Rev Biochem. 2013;82:531–50. doi: 10.1146/annurev-biochem-051110-133601. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 160.Jiang N, Kuznetsov A, Nocek JM, Hoffman BM, Crane BR, Hu XQ, Beratan DN. J Phys Chem B. 2013;117:9129–41. doi: 10.1021/jp401551t. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 161.Seifert JL, Pfister TD, Nocek JM, Lu Y, Hoffman BM. J Am Chem Soc. 2005;127:5750–1. doi: 10.1021/ja042459p. [DOI] [PubMed] [Google Scholar]
  • 162.Shih C, Museth AK, Abrahamsson M, Blanco-Rodriguez AM, Di Bilio AJ, Sudhamsu J, Crane BR, Ronayne KL, Towrie M, Vlcek A, Richards JH, Winkler JR, Gray HB. Science. 2008;320:1760–2. doi: 10.1126/science.1158241. [DOI] [PubMed] [Google Scholar]
  • 163.Warren JJ, Herrera N, Hill MG, Winkler JR, Gray HB. J Am Chem Soc. 2013;135:11151–8. doi: 10.1021/ja403734n. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 164.Yosca TH, Rittle J, Krest CM, Onderko EL, Silakov A, Calixto JC, Behan RK, Green MT. Science. 2013;342:825–9. doi: 10.1126/science.1244373. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 165.Schünemann V, Lendzian F, Jung C, Contzen J, Barra AL, Sligar SG, Trautwein AX. J Biol Chem. 2004;279:10919–30. doi: 10.1074/jbc.M307884200. [DOI] [PubMed] [Google Scholar]
  • 166.Jung C, Schünemann V, Lendzian F. Biochem Biophys Res Commun. 2005;338:355–64. doi: 10.1016/j.bbrc.2005.08.166. [DOI] [PubMed] [Google Scholar]
  • 167.Rutherford AW, Osyczka A, Rappaport F. FEBS Lett. 2012;586:603–16. doi: 10.1016/j.febslet.2011.12.039. [DOI] [PubMed] [Google Scholar]
  • 168.Dance ZEX, Ahrens MJ, Vega AM, Ricks AB, McCamant DW, Ratner MA, Wasielewski MR. J Am Chem Soc. 2008;130:830–2. doi: 10.1021/ja077386z. [DOI] [PubMed] [Google Scholar]
  • 169.Nealson KH, Saffarini D. Annu Rev Microbiol. 1994;48:311–43. doi: 10.1146/annurev.mi.48.100194.001523. [DOI] [PubMed] [Google Scholar]
  • 170.Gorby YA, Yanina S, McLean JS, Rosso KM, Moyles D, Dohnalkova A, Beveridge TJ, Chang IS, Kim BH, Kim KS, Culley DE, Reed SB, Romine MF, Saffarini DA, Hill EA, Shi L, Elias DA, Kennedy DW, Pinchuk G, Watanabe K, Ishii Si, Logan B, Nealson KH, Fredrickson JK. Proc Natl Acad Sci USA. 2006;103:11358–63. doi: 10.1073/pnas.0604517103. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 171.Malvankar NS, Vargas M, Nevin KP, Franks AE, Leang C, Kim BC, Inoue K, Mester T, Covalla SF, Johnson JP, Rotello VM, Tuominen MT, Lovley DR. Nature Nanotechnology. 2011;6:573–9. doi: 10.1038/nnano.2011.119. [DOI] [PubMed] [Google Scholar]
  • 172.Polizzi NF, Skourtis SS, Beratan DN. Faraday Discuss. 2012;155:43–62. doi: 10.1039/c1fd00098e. [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

Supporting Information

RESOURCES