Oxidative phosphorylation

Oxidative phosphorylation (UK /ɒkˈsɪd.ə.tɪv/, US /ˈɑːk.sɪˌdeɪ.tɪv/ [1] or electron transport-linked phosphorylation or terminal oxidation) is the metabolic pathway in which cells use enzymes to oxidize nutrients, thereby releasing the chemical energy stored within in order to produce adenosine triphosphate (ATP). In most eukaryotes, this takes place inside mitochondria. Almost all aerobic organisms carry out oxidative phosphorylation. This pathway is so pervasive because it releases more energy than alternative fermentation processes such as anaerobic glycolysis.[2]

The electron transport chain in the cell is the site of oxidative phosphorylation. The NADH and succinate generated in the citric acid cycle are oxidized, releasing the energy of O2 to power the ATP synthase.

During oxidative phosphorylation, electrons are transferred from electron donors to electron acceptors such as oxygen in redox reactions. These redox reactions release the energy stored in the relatively weak double bond of O2, which is used to form ATP. In eukaryotes, these redox reactions are catalyzed by a series of protein complexes within the inner membrane of the cell's mitochondria, whereas, in prokaryotes, these proteins are located in the cell's outer membrane. These linked sets of proteins are called electron transport chains. In eukaryotes, five main protein complexes are involved, whereas in prokaryotes many different enzymes are present, using a variety of electron donors and acceptors.

The energy transferred by electrons flowing through this electron transport chain is used to transport protons across the inner mitochondrial membrane, in a process called electron transport. This generates potential energy in the form of a pH gradient and an electrical potential across this membrane. This store of energy is tapped when protons flow back across the membrane and down the potential energy gradient, through a large enzyme called ATP synthase; this process is known as chemiosmosis. The ATP synthase uses the energy to transform adenosine diphosphate (ADP) into adenosine triphosphate, in a phosphorylation reaction. The reaction is driven by the proton flow, which forces the rotation of a part of the enzyme; the ATP synthase is a rotary mechanical motor.

Although oxidative phosphorylation is a vital part of metabolism, it produces reactive oxygen species such as superoxide and hydrogen peroxide, which lead to propagation of free radicals, damaging cells and contributing to disease and, possibly, aging (senescence). The enzymes carrying out this metabolic pathway are also the target of many drugs and poisons that inhibit their activities.

Chemiosmosis
Further information: Chemiosmosis and Bioenergetics

Oxidative phosphorylation works by using energy-releasing chemical reactions to drive energy-requiring reactions: The two sets of reactions are said to be coupled. This means one cannot occur without the other. The chain of redox reactions driving the flow of electrons through the electron transport chain, from electron donors such as NADH to electron acceptors such as oxygen and hydrogen (protons),[2] is an exergonic process – it releases energy, whereas the synthesis of ATP is an endergonic process, which requires an input of energy. Both the electron transport chain and the ATP synthase are embedded in a membrane, and energy is transferred from the electron transport chain to the ATP synthase by movements of protons across this membrane, in a process called chemiosmosis.[3] A current of protons is driven from the negative N-side of the membrane to the positive P-side through the proton-pumping enzymes of the electron transport chain. The movement of protons creates an electrochemical gradient across the membrane, which is often called the proton-motive force. It has two components: a difference in proton concentration (a H+ gradient, ΔpH) and a difference in electric potential, with the N-side having a negative charge.[4]

ATP synthase releases this stored energy by completing the circuit and allowing protons to flow down the electrochemical gradient, back to the N-side of the membrane.[5] The electrochemical gradient drives the rotation of part of the enzyme's structure and couples this motion to the synthesis of ATP.

The two components of the proton-motive force are thermodynamically equivalent: In mitochondria, the largest part of energy is provided by the potential; in alkaliphile bacteria the electrical energy even has to compensate for a counteracting inverse pH difference. Inversely, chloroplasts operate mainly on ΔpH. However, they also require a small membrane potential for the kinetics of ATP synthesis. In the case of the fusobacterium Propionigenium modestum it drives the counter-rotation of subunits a and c of the FO motor of ATP synthase.[4]

The amount of energy released by oxidative phosphorylation is high, compared with the amount produced by anaerobic fermentation, due to the high energy of O2.[2] Glycolysis produces only 2 ATP molecules, but somewhere between 30 and 36 ATPs are produced by the oxidative phosphorylation of the 10 NADH and 2 succinate molecules made by converting one molecule of glucose to carbon dioxide and water,[6] while each cycle of beta oxidation of a fatty acid yields about 14 ATPs. These ATP yields are theoretical maximum values; in practice, some protons leak across the membrane, lowering the yield of ATP.[7]

Electron and proton transfer molecules
Further information: Coenzyme and Cofactor (biochemistry)
Reduction of coenzyme Q from its ubiquinone form (Q) to the reduced ubiquinol form (QH2).

The electron transport chain carries both protons and electrons, passing electrons from donors to acceptors, and transporting protons across a membrane. These processes use both soluble and protein-bound transfer molecules. In mitochondria, electrons are transferred within the intermembrane space by the water-soluble electron transfer protein cytochrome c.[8] This carries only electrons, and these are transferred by the reduction and oxidation of an iron atom that the protein holds within a heme group in its structure. Cytochrome c is also found in some bacteria, where it is located within the periplasmic space.[9]

Within the inner mitochondrial membrane, the lipid-soluble electron carrier coenzyme Q10 (Q) carries both electrons and protons by a redox cycle.[10] This small benzoquinone molecule is very hydrophobic, so it diffuses freely within the membrane. When Q accepts two electrons and two protons, it becomes reduced to the ubiquinol form (QH2); when QH2 releases two electrons and two protons, it becomes oxidized back to the ubiquinone (Q) form. As a result, if two enzymes are arranged so that Q is reduced on one side of the membrane and QH2 oxidized on the other, ubiquinone will couple these reactions and shuttle protons across the membrane.[11] Some bacterial electron transport chains use different quinones, such as menaquinone, in addition to ubiquinone.[12]

Within proteins, electrons are transferred between flavin cofactors,[5][13] iron–sulfur clusters, and cytochromes. There are several types of iron–sulfur cluster. The simplest kind found in the electron transfer chain consists of two iron atoms joined by two atoms of inorganic sulfur; these are called [2Fe–2S] clusters. The second kind, called [4Fe–4S], contains a cube of four iron atoms and four sulfur atoms. Each iron atom in these clusters is coordinated by an additional amino acid, usually by the sulfur atom of cysteine. Metal ion cofactors undergo redox reactions without binding or releasing protons, so in the electron transport chain they serve solely to transport electrons through proteins. Electrons move quite long distances through proteins by hopping along chains of these cofactors.[14] This occurs by quantum tunnelling, which is rapid over distances of less than 1.4×10−9 m.[15]

Eukaryotic electron transport chains
Further information: Electron transport chain and Chemiosmosis

Many catabolic biochemical processes, such as glycolysis, the citric acid cycle, and beta oxidation, produce the reduced coenzyme NADH. This coenzyme contains electrons that have a high transfer potential; in other words, they will release a large amount of energy upon oxidation. However, the cell does not release this energy all at once, as this would be an uncontrollable reaction. Instead, the electrons are removed from NADH and passed to oxygen through a series of enzymes that each release a small amount of the energy. This set of enzymes, consisting of complexes I through IV, is called the electron transport chain and is found in the inner membrane of the mitochondrion. Succinate is also oxidized by the electron transport chain, but feeds into the pathway at a different point.

In eukaryotes, the enzymes in this electron transport system use the energy released from O2 by NADH to pump protons across the inner membrane of the mitochondrion. This causes protons to build up in the intermembrane space, and generates an electrochemical gradient across the membrane. The energy stored in this potential is then used by ATP synthase to produce ATP. Oxidative phosphorylation in the eukaryotic mitochondrion is the best-understood example of this process. The mitochondrion is present in almost all eukaryotes, with the exception of anaerobic protozoa such as Trichomonas vaginalis that instead reduce protons to hydrogen in a remnant mitochondrion called a hydrogenosome.[16]

Typical respiratory enzymes and substrates in eukaryotes.
Respiratory enzyme Redox pair Midpoint potential 

(Volts)

NADH dehydrogenase NAD+ / NADH −0.32[17]
Succinate dehydrogenase FMN or FAD / FMNH2 or FADH2 −0.20[17]
Cytochrome bc1 complex Coenzyme Q10ox / Coenzyme Q10red +0.06[17]
Cytochrome bc1 complex Cytochrome box / Cytochrome bred +0.12[17]
Complex IV Cytochrome cox / Cytochrome cred +0.22[17]
Complex IV Cytochrome aox / Cytochrome ared +0.29[17]
Complex IV O2 / HO− +0.82[17]
Conditions: pH = 7[17]

NADH-coenzyme Q oxidoreductase (complex I)
Complex I or NADH-Q oxidoreductase. The abbreviations are discussed in the text. In all diagrams of respiratory complexes in this article, the matrix is at the bottom, with the intermembrane space above.

NADH-coenzyme Q oxidoreductase, also known as NADH dehydrogenase or complex I, is the first protein in the electron transport chain.[18] Complex I is a giant enzyme with the mammalian complex I having 46 subunits and a molecular mass of about 1,000 kilodaltons (kDa).[19] The structure is known in detail only from a bacterium;[20][21] in most organisms the complex resembles a boot with a large "ball" poking out from the membrane into the mitochondrion.[22][23] The genes that encode the individual proteins are contained in both the cell nucleus and the mitochondrial genome, as is the case for many enzymes present in the mitochondrion.

The reaction that is catalyzed by this enzyme is the two electron oxidation of NADH by coenzyme Q10 or ubiquinone (represented as Q in the equation below), a lipid-soluble quinone that is found in the mitochondrion membrane:

 

 

 

 

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The start of the reaction, and indeed of the entire electron chain, is the binding of a NADH molecule to complex I and the donation of two electrons. The electrons enter complex I via a prosthetic group attached to the complex, flavin mononucleotide (FMN). The addition of electrons to FMN converts it to its reduced form, FMNH2. The electrons are then transferred through a series of iron–sulfur clusters: the second kind of prosthetic group present in the complex.[20] There are both [2Fe–2S] and [4Fe–4S] iron–sulfur clusters in complex I.

As the electrons pass through this complex, four protons are pumped from the matrix into the intermembrane space. Exactly how this occurs is unclear, but it seems to involve conformational changes in complex I that cause the protein to bind protons on the N-side of the membrane and release them on the P-side of the membrane.[24] Finally, the electrons are transferred from the chain of iron–sulfur clusters to a ubiquinone molecule in the membrane.[18] Reduction of ubiquinone also contributes to the generation of a proton gradient, as two protons are taken up from the matrix as it is reduced to ubiquinol (QH2).

Succinate-Q oxidoreductase (complex II)
Complex II: Succinate-Q oxidoreductase.

Succinate-Q oxidoreductase, also known as complex II or succinate dehydrogenase, is a second entry point to the electron transport chain.[25] It is unusual because it is the only enzyme that is part of both the citric acid cycle and the electron transport chain. Complex II consists of four protein subunits and contains a bound flavin adenine dinucleotide (FAD) cofactor, iron–sulfur clusters, and a heme group that does not participate in electron transfer to coenzyme Q, but is believed to be important in decreasing production of reactive oxygen species.[26][27] It oxidizes succinate to fumarate and reduces ubiquinone. As this reaction releases less energy than the oxidation of NADH, complex II does not transport protons across the membrane and does not contribute to the proton gradient.

 

 

 

 

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In some eukaryotes, such as the parasitic worm Ascaris suum, an enzyme similar to complex II, fumarate reductase (menaquinol:fumarate oxidoreductase, or QFR), operates in reverse to oxidize ubiquinol and reduce fumarate. This allows the worm to survive in the anaerobic environment of the large intestine, carrying out anaerobic oxidative phosphorylation with fumarate as the electron acceptor.[28] Another unconventional function of complex II is seen in the malaria parasite Plasmodium falciparum. Here, the reversed action of complex II as an oxidase is important in regenerating ubiquinol, which the parasite uses in an unusual form of pyrimidine biosynthesis.[29]

Electron transfer flavoprotein-Q oxidoreductase

Electron transfer flavoprotein-ubiquinone oxidoreductase (ETF-Q oxidoreductase), also known as electron transferring-flavoprotein dehydrogenase, is a third entry point to the electron transport chain. It is an enzyme that accepts electrons from electron-transferring flavoprotein in the mitochondrial matrix, and uses these electrons to reduce ubiquinone.[30] This enzyme contains a flavin and a [4Fe–4S] cluster, but, unlike the other respiratory complexes, it attaches to the surface of the membrane and does not cross the lipid bilayer.[31]

 

 

 

 

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In mammals, this metabolic pathway is important in beta oxidation of fatty acids and catabolism of amino acids and choline, as it accepts electrons from multiple acetyl-CoA dehydrogenases.[32][33] In plants, ETF-Q oxidoreductase is also important in the metabolic responses that allow survival in extended periods of darkness.[34]

Q-cytochrome c oxidoreductase (complex III)
The two electron transfer steps in complex III: Q-cytochrome c oxidoreductase. After each step, Q (in the upper part of the figure) leaves the enzyme.

Q-cytochrome c oxidoreductase is also known as cytochrome c reductase, cytochrome bc1 complex, or simply complex III.[35][36] In mammals, this enzyme is a dimer, with each subunit complex containing 11 protein subunits, an [2Fe-2S] iron–sulfur cluster and three cytochromes: one cytochrome c1 and two b cytochromes.[37] A cytochrome is a kind of electron-transferring protein that contains at least one heme group. The iron atoms inside complex III's heme groups alternate between a reduced ferrous (+2) and oxidized ferric (+3) state as the electrons are transferred through the protein.

The reaction catalyzed by complex III is the oxidation of one molecule of ubiquinol and the reduction of two molecules of cytochrome c, a heme protein loosely associated with the mitochondrion. Unlike coenzyme Q, which carries two electrons, cytochrome c carries only one electron.

 

 

 

 

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As only one of the electrons can be transferred from the QH2 donor to a cytochrome c acceptor at a time, the reaction mechanism of complex III is more elaborate than those of the other respiratory complexes, and occurs in two steps called the Q cycle.[38] In the first step, the enzyme binds three substrates, first, QH2, which is then oxidized, with one electron being passed to the second substrate, cytochrome c. The two protons released from QH2 pass into the intermembrane space. The third substrate is Q, which accepts the second electron from the QH2 and is reduced to Q.−, which is the ubisemiquinone free radical. The first two substrates are released, but this ubisemiquinone intermediate remains bound. In the second step, a second molecule of QH2 is bound and again passes its first electron to a cytochrome c acceptor. The second electron is passed to the bound ubisemiquinone, reducing it to QH2 as it gains two protons from the mitochondrial matrix. This QH2 is then released from the enzyme.[39]

As coenzyme Q is reduced to ubiquinol on the inner side of the membrane and oxidized to ubiquinone on the other, a net transfer of protons across the membrane occurs, adding to the proton gradient.[5] The rather complex two-step mechanism by which this occurs is important, as it increases the efficiency of proton transfer. If, instead of the Q cycle, one molecule of QH2 were used to directly reduce two molecules of cytochrome c, the efficiency would be halved, with only one proton transferred per cytochrome c reduced.[5]

Cytochrome c oxidase (complex IV)
Further information: cytochrome c oxidase
Complex IV: cytochrome c oxidase.

Cytochrome c oxidase, also known as complex IV, is the final protein complex in the electron transport chain.[40] The mammalian enzyme has an extremely complicated structure and contains 13 subunits, two heme groups, as well as multiple metal ion cofactors – in all, three atoms of copper, one of magnesium and one of zinc.[41]

This enzyme mediates the final reaction in the electron transport chain and transfers electrons to oxygen and hydrogen (protons),[2] while pumping protons across the membrane.[42] The final electron acceptor oxygen, which provides most of the energy released in the electron transfer chain and is also called the terminal electron acceptor, is reduced to water in this step, which releases half of all the energy in aerobic respiration.[2] Both the direct pumping of protons and the consumption of matrix protons in the reduction of oxygen contribute to the proton gradient. The reaction catalyzed is the oxidation of cytochrome c and the reduction of oxygen:

 

 

 

 

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Alternative reductases and oxidases

Many eukaryotic organisms have electron transport chains that differ from the much-studied mammalian enzymes described above. For example, plants have alternative NADH oxidases, which oxidize NADH in the cytosol rather than in the mitochondrial matrix, and pass these electrons to the ubiquinone pool.[43] These enzymes do not transport protons, and, therefore, reduce ubiquinone without altering the electrochemical gradient across the inner membrane.[44]

Another example of a divergent electron transport chain is the alternative oxidase, which is found in plants, as well as some fungi, protists, and possibly some animals.[45][46] This enzyme transfers electrons directly from ubiquinol to oxygen.[47]

The electron transport pathways produced by these alternative NADH and ubiquinone oxidases have lower ATP yields than the full pathway. The advantages produced by a shortened pathway are not entirely clear. However, the alternative oxidase is produced in response to stresses such as cold, reactive oxygen species, and infection by pathogens, as well as other factors that inhibit the full electron transport chain.[48][49] Alternative pathways might, therefore, enhance an organisms' resistance to injury, by reducing oxidative stress.[50]

Organization of complexes

The original model for how the respiratory chain complexes are organized was that they diffuse freely and independently in the mitochondrial membrane.[51] However, recent data suggest that the complexes might form higher-order structures called supercomplexes or "respirasomes".[52] In this model, the various complexes exist as organized sets of interacting enzymes.[53] These associations might allow channeling of substrates between the various enzyme complexes, increasing the rate and efficiency of electron transfer.[54] Within such mammalian supercomplexes, some components would be present in higher amounts than others, with some data suggesting a ratio between complexes I/II/III/IV and the ATP synthase of approximately 1:1:3:7:4.[55] However, the debate over this supercomplex hypothesis is not completely resolved, as some data do not appear to fit with this model.[19][56]

Prokaryotic electron transport chains
Further information: Microbial metabolism

In contrast to the general similarity in structure and function of the electron transport chains in eukaryotes, bacteria and archaea possess a large variety of electron-transfer enzymes. These use an equally wide set of chemicals as substrates.[57] In common with eukaryotes, prokaryotic electron transport uses the energy released from the oxidation of a substrate to pump ions across a membrane and generate an electrochemical gradient. In the bacteria, oxidative phosphorylation in Escherichia coli is understood in most detail, while archaeal systems are at present poorly understood.[58]

The main difference between eukaryotic and prokaryotic oxidative phosphorylation is that bacteria and archaea use many different substances to donate or accept electrons. This allows prokaryotes to grow under a wide variety of environmental conditions.[59] In E. coli, for example, oxidative phosphorylation can be driven by a large number of pairs of reducing agents and oxidizing agents, which are listed below. The midpoint potential of a chemical measures how much energy is released when it is oxidized or reduced, with reducing agents having negative potentials and oxidizing agents positive potentials.

Respiratory enzymes and substrates in E. coli.[60]
Respiratory enzyme Redox pair Midpoint potential 

(Volts)

Formate dehydrogenase Bicarbonate / Formate −0.43
Hydrogenase Proton / Hydrogen −0.42
NADH dehydrogenase NAD+ / NADH −0.32
Glycerol-3-phosphate dehydrogenase DHAP / Gly-3-P −0.19
Pyruvate oxidase Acetate + Carbon dioxide / Pyruvate ?
Lactate dehydrogenase Pyruvate / Lactate −0.19
D-amino acid dehydrogenase 2-oxoacid + ammonia / D-amino acid ?
Glucose dehydrogenase Gluconate / Glucose −0.14
Succinate dehydrogenase Fumarate / Succinate +0.03
Ubiquinol oxidase Oxygen / Water +0.82
Nitrate reductase Nitrate / Nitrite +0.42
Nitrite reductase Nitrite / Ammonia +0.36
Dimethyl sulfoxide reductase DMSO / DMS +0.16
Trimethylamine N-oxide reductase TMAO / TMA +0.13
Fumarate reductase Fumarate / Succinate +0.03

As shown above, E. coli can grow with reducing agents such as formate, hydrogen, or lactate as electron donors, and nitrate, DMSO, or oxygen as acceptors.[59] The larger the difference in midpoint potential between an oxidizing and reducing agent, the more energy is released when they react. Out of these compounds, the succinate/fumarate pair is unusual, as its midpoint potential is close to zero. Succinate can therefore be oxidized to fumarate if a strong oxidizing agent such as oxygen is available, or fumarate can be reduced to succinate using a strong reducing agent such as formate. These alternative reactions are catalyzed by succinate dehydrogenase and fumarate reductase, respectively.[61]

Some prokaryotes use redox pairs that have only a small difference in midpoint potential. For example, nitrifying bacteria such as Nitrobacter oxidize nitrite to nitrate, donating the electrons to oxygen. The small amount of energy released in this reaction is enough to pump protons and generate ATP, but not enough to produce NADH or NADPH directly for use in anabolism.[62] This problem is solved by using a nitrite oxidoreductase to produce enough proton-motive force to run part of the electron transport chain in reverse, causing complex I to generate NADH.[63][64]

Prokaryotes control their use of these electron donors and acceptors by varying which enzymes are produced, in response to environmental conditions.[65] This flexibility is possible because different oxidases and reductases use the same ubiquinone pool. This allows many combinations of enzymes to function together, linked by the common ubiquinol intermediate.[60] These respiratory chains therefore have a modular design, with easily interchangeable sets of enzyme systems.

In addition to this metabolic diversity, prokaryotes also possess a range of isozymes – different enzymes that catalyze the same reaction. For example, in E. coli, there are two different types of ubiquinol oxidase using oxygen as an electron acceptor. Under highly aerobic conditions, the cell uses an oxidase with a low affinity for oxygen that can transport two protons per electron. However, if levels of oxygen fall, they switch to an oxidase that transfers only one proton per electron, but has a high affinity for oxygen.[66]

ATP synthase (complex V)
Further information: ATP synthase

ATP synthase, also called complex V, is the final enzyme in the oxidative phosphorylation pathway. This enzyme is found in all forms of life and functions in the same way in both prokaryotes and eukaryotes.[67] The enzyme uses the energy stored in a proton gradient across a membrane to drive the synthesis of ATP from ADP and phosphate (Pi). Estimates of the number of protons required to synthesize one ATP have ranged from three to four,[68][69] with some suggesting cells can vary this ratio, to suit different conditions.[70]

 

 

 

 

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This phosphorylation reaction is an equilibrium, which can be shifted by altering the proton-motive force. In the absence of a proton-motive force, the ATP synthase reaction will run from right to left, hydrolyzing ATP and pumping protons out of the matrix across the membrane. However, when the proton-motive force is high, the reaction is forced to run in the opposite direction; it proceeds from left to right, allowing protons to flow down their concentration gradient and turning ADP into ATP.[67] Indeed, in the closely related vacuolar type H+-ATPases, the hydrolysis reaction is used to acidify cellular compartments, by pumping protons and hydrolysing ATP.[71]

ATP synthase is a massive protein complex with a mushroom-like shape. The mammalian enzyme complex contains 16 subunits and has a mass of approximately 600 kilodaltons.[72] The portion embedded within the membrane is called FO and contains a ring of c subunits and the proton channel. The stalk and the ball-shaped headpiece is called F1 and is the site of ATP synthesis. The ball-shaped complex at the end of the F1 portion contains six proteins of two different kinds (three α subunits and three β subunits), whereas the "stalk" consists of one protein: the γ subunit, with the tip of the stalk extending into the ball of α and β subunits.[73] Both the α and β subunits bind nucleotides, but only the β subunits catalyze the ATP synthesis reaction. Reaching along the side of the F1 portion and back into the membrane is a long rod-like subunit that anchors the α and β subunits into the base of the enzyme.

As protons cross the membrane through the channel in the base of ATP synthase, the FO proton-driven motor rotates.[74] Rotation might be caused by changes in the ionization of amino acids in the ring of c subunits causing electrostatic interactions that propel the ring of c subunits past the proton channel.[75] This rotating ring in turn drives the rotation of the central axle (the γ subunit stalk) within the α and β subunits. The α and β subunits are prevented from rotating themselves by the side-arm, which acts as a stator. This movement of the tip of the γ subunit within the ball of α and β subunits provides the energy for the active sites in the β subunits to undergo a cycle of movements that produces and then releases ATP.[76]

Mechanism of ATP synthase. ATP is shown in red, ADP and phosphate in pink and the rotating γ subunit in black.

This ATP synthesis reaction is called the binding change mechanism and involves the active site of a β subunit cycling between three states.[77] In the "open" state, ADP and phosphate enter the active site (shown in brown in the diagram). The protein then closes up around the molecules and binds them loosely – the "loose" state (shown in red). The enzyme then changes shape again and forces these molecules together, with the active site in the resulting "tight" state (shown in pink) binding the newly produced ATP molecule with very high affinity. Finally, the active site cycles back to the open state, releasing ATP and binding more ADP and phosphate, ready for the next cycle.

In some bacteria and archaea, ATP synthesis is driven by the movement of sodium ions through the cell membrane, rather than the movement of protons.[78][79] Archaea such as Methanococcus also contain the A1Ao synthase, a form of the enzyme that contains additional proteins with little similarity in sequence to other bacterial and eukaryotic ATP synthase subunits. It is possible that, in some species, the A1Ao form of the enzyme is a specialized sodium-driven ATP synthase,[80] but this might not be true in all cases.[79]

Oxidative phosphorylation - energetics

The energy released in oxidative phosphorylation can mostly be attributed to O2 with its relatively weak double bond.[2] The transport of electrons from redox pair NAD+/ NADH to the final redox pair 1/2 O2/ H2O can be summarized as

1/2 O2 + NADH + H+ → H2O + NAD+

The potential difference between these two redox pairs is 1.14 volt, which is equivalent to -52 kcal/mol or -2600 kJ per 6 mol of O2.

When one NADH is oxidized through the electron transfer chain, three ATPs are produced, which is equivalent to 7.3 kcal/mol x 3 = 21.9 kcal/mol.

The conservation of the energy can be calculated by the following formula

Efficiency = (21.9 x 100%) / 52 = 42%

So we can conclude that when NADH is oxidized, about 42% of energy is conserved in the form of three ATPs and the remaining (58%) energy is lost as heat (unless the chemical energy of ATP under physiological conditions was underestimated).

Reactive oxygen species
Further information: Oxidative stress and Antioxidant

Molecular oxygen is an ideal terminal electron acceptor because it is a strong oxidizing agent. The reduction of oxygen does involve potentially harmful intermediates.[81] Although the transfer of four electrons and four protons reduces oxygen to water, which is harmless, transfer of one or two electrons produces superoxide or peroxide anions, which are dangerously reactive.

 

 

 

 

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These reactive oxygen species and their reaction products, such as the hydroxyl radical, are very harmful to cells, as they oxidize proteins and cause mutations in DNA. This cellular damage might contribute to disease and is proposed as one cause of aging.[82][83]

The cytochrome c oxidase complex is highly efficient at reducing oxygen to water, and it releases very few partly reduced intermediates; however small amounts of superoxide anion and peroxide are produced by the electron transport chain.[84] Particularly important is the reduction of coenzyme Q in complex III, as a highly reactive ubisemiquinone free radical is formed as an intermediate in the Q cycle. This unstable species can lead to electron "leakage" when electrons transfer directly to oxygen, forming superoxide.[85] As the production of reactive oxygen species by these proton-pumping complexes is greatest at high membrane potentials, it has been proposed that mitochondria regulate their activity to maintain the membrane potential within a narrow range that balances ATP production against oxidant generation.[86] For instance, oxidants can activate uncoupling proteins that reduce membrane potential.[87]

To counteract these reactive oxygen species, cells contain numerous antioxidant systems, including antioxidant vitamins such as vitamin C and vitamin E, and antioxidant enzymes such as superoxide dismutase, catalase, and peroxidases,[81] which detoxify the reactive species, limiting damage to the cell.

Oxidative phosphorylation in hypoxic conditions

As oxygen is fundamental for oxidative phosphorylation, a shortage in O2 level likely alters ATP production rates. However, proton motive force and ATP production can be maintained by intracellular acidosis.[88] Cytosolic protons that have accumulated with ATP hydrolysis and lactic acidosis can freely diffuse across the mitochondrial outer-membrane and acidify the inter-membrane space, hence directly contributing to the proton motive force and ATP production.

Inhibitors

There are several well-known drugs and toxins that inhibit oxidative phosphorylation. Although any one of these toxins inhibits only one enzyme in the electron transport chain, inhibition of any step in this process will halt the rest of the process. For example, if oligomycin inhibits ATP synthase, protons cannot pass back into the mitochondrion.[89] As a result, the proton pumps are unable to operate, as the gradient becomes too strong for them to overcome. NADH is then no longer oxidized and the citric acid cycle ceases to operate because the concentration of NAD+ falls below the concentration that these enzymes can use.

Many site-specific inhibitors of the electron transport chain have contributed to the present knowledge of mitochondrial respiration. Synthesis of ATP is also dependent on the electron transport chain, so all site-specific inhibitors also inhibit ATP formation. The fish poison rotenone, the barbiturate drug amytal, and the antibiotic piericidin A inhibit NADH and coenzyme Q.[90]

Carbon monoxide, cyanide, hydrogen sulphide and azide effectively inhibit cytochrome oxidase. Carbon monoxide reacts with the reduced form of the cytochrome while cyanide and azide react with the oxidised form. An antibiotic, antimycin A, and British anti-Lewisite, an antidote used against chemical weapons, are the two important inhibitors of the site between cytochrome B and C1.[90]

Compounds Use Site of action Effect on oxidative phosphorylation
Cyanide
Carbon monoxide
Azide
Hydrogen sulfide		 Poisons Complex IV Inhibit the electron transport chain by binding more strongly than oxygen to the Fe–Cu center in cytochrome c oxidase, preventing the reduction of oxygen.[91]
Oligomycin Antibiotic Complex V Inhibits ATP synthase by blocking the flow of protons through the Fo subunit.[89]
CCCP
2,4-Dinitrophenol		 Poisons, weight-loss[N 1] Inner membrane Ionophores that disrupt the proton gradient by carrying protons across a membrane. This ionophore uncouples proton pumping from ATP synthesis because it carries protons across the inner mitochondrial membrane.[92]
Rotenone Pesticide Complex I Prevents the transfer of electrons from complex I to ubiquinone by blocking the ubiquinone-binding site.[93]
Malonate and oxaloacetate Poisons Complex II Competitive inhibitors of succinate dehydrogenase (complex II).[94]
Antimycin A Piscicide Complex III Binds to the Qi site of cytochrome c reductase, thereby inhibiting the oxidation of ubiquinol.

Not all inhibitors of oxidative phosphorylation are toxins. In brown adipose tissue, regulated proton channels called uncoupling proteins can uncouple respiration from ATP synthesis.[95] This rapid respiration produces heat, and is particularly important as a way of maintaining body temperature for hibernating animals, although these proteins may also have a more general function in cells' responses to stress.[96]

History
Further information: History of biochemistry and History of molecular biology

The field of oxidative phosphorylation began with the report in 1906 by Arthur Harden of a vital role for phosphate in cellular fermentation, but initially only sugar phosphates were known to be involved.[97] However, in the early 1940s, the link between the oxidation of sugars and the generation of ATP was firmly established by Herman Kalckar,[98] confirming the central role of ATP in energy transfer that had been proposed by Fritz Albert Lipmann in 1941.[99] Later, in 1949, Morris Friedkin and Albert L. Lehninger proved that the coenzyme NADH linked metabolic pathways such as the citric acid cycle and the synthesis of ATP.[100] The term oxidative phosphorylation was coined by Volodymyr Belitser in 1939.[101][102]

For another twenty years, the mechanism by which ATP is generated remained mysterious, with scientists searching for an elusive "high-energy intermediate" that would link oxidation and phosphorylation reactions.[103] This puzzle was solved by Peter D. Mitchell with the publication of the chemiosmotic theory in 1961.[104] At first, this proposal was highly controversial, but it was slowly accepted and Mitchell was awarded a Nobel prize in 1978.[105][106] Subsequent research concentrated on purifying and characterizing the enzymes involved, with major contributions being made by David E. Green on the complexes of the electron-transport chain, as well as Efraim Racker on the ATP synthase.[107] A critical step towards solving the mechanism of the ATP synthase was provided by Paul D. Boyer, by his development in 1973 of the "binding change" mechanism, followed by his radical proposal of rotational catalysis in 1982.[77][108] More recent work has included structural studies on the enzymes involved in oxidative phosphorylation by John E. Walker, with Walker and Boyer being awarded a Nobel Prize in 1997.[109]

See also

Notes
  1. DNP was extensively used as an anti-obesity medication in the 1930s but was ultimately discontinued due to its dangerous side effects. However, illicit use of the drug for this purpose continues today. See 2,4-Dinitrophenol#Dieting aid for more information.

References
  1. "oxidative Meaning in the Cambridge English Dictionary". dictionary.cambridge.org. Archived from the original on 24 January 2018. Retrieved 28 April 2018.
  2. Schmidt-Rohr K (2020). "Oxygen Is the High-Energy Molecule Powering Complex Multicellular Life: Fundamental Corrections to Traditional Bioenergetics". ACS Omega. 5 (5): 2221–2233. doi:10.1021/acsomega.9b03352. PMC 7016920. PMID 32064383.
  3. Mitchell P, Moyle J (1967). "Chemiosmotic hypothesis of oxidative phosphorylation". Nature. 213 (5072): 137–9. Bibcode:1967Natur.213..137M. doi:10.1038/213137a0. PMID 4291593. S2CID 4149605.
  4. Dimroth P, Kaim G, Matthey U (1 January 2000). "Crucial role of the membrane potential for ATP synthesis by F(1)F(o) ATP synthases". J. Exp. Biol. 203 (Pt 1): 51–9. PMID 10600673. Archived from the original on 30 September 2007.
  5. Schultz BE, Chan SI (2001). "Structures and proton-pumping strategies of mitochondrial respiratory enzymes" (PDF). Annu Rev Biophys Biomol Struct. 30: 23–65. doi:10.1146/annurev.biophys.30.1.23. PMID 11340051.
  6. Rich PR (2003). "The molecular machinery of Keilin's respiratory chain". Biochem. Soc. Trans. 31 (Pt 6): 1095–105. doi:10.1042/bst0311095. PMID 14641005.
  7. Porter RK, Brand MD (1995). "Mitochondrial proton conductance and H+/O ratio are independent of electron transport rate in isolated hepatocytes". Biochem. J. 310 (Pt 2): 379–82. doi:10.1042/bj3100379. PMC 1135905. PMID 7654171.
  8. Mathews FS (1985). "The structure, function and evolution of cytochromes". Prog. Biophys. Mol. Biol. 45 (1): 1–56. doi:10.1016/0079-6107(85)90004-5. PMID 3881803.
  9. Wood PM (1983). "Why do c-type cytochromes exist?". FEBS Lett. 164 (2): 223–6. doi:10.1016/0014-5793(83)80289-0. PMID 6317447. S2CID 7685958.
  10. Crane FL (1 December 2001). "Biochemical functions of coenzyme Q10". J Am Coll Nutr. 20 (6): 591–8. doi:10.1080/07315724.2001.10719063. PMID 11771674. S2CID 28013583.
  11. Mitchell P (1979). "Keilin's respiratory chain concept and its chemiosmotic consequences". Science. 206 (4423): 1148–59. Bibcode:1979Sci...206.1148M. doi:10.1126/science.388618. PMID 388618.
  12. Søballe B, Poole RK (1999). "Microbial ubiquinones: multiple roles in respiration, gene regulation and oxidative stress management" (PDF). Microbiology. 145 (8): 1817–30. doi:10.1099/13500872-145-8-1817. PMID 10463148. Archived (PDF) from the original on 2008-05-29.
  13. Johnson DC, Dean DR, Smith AD, Johnson MK (2005). "Structure, function, and formation of biological iron-sulfur clusters". Annu. Rev. Biochem. 74: 247–81. doi:10.1146/annurev.biochem.74.082803.133518. PMID 15952888.
  14. Page CC, Moser CC, Chen X, Dutton PL (1999). "Natural engineering principles of electron tunnelling in biological oxidation-reduction". Nature. 402 (6757): 47–52. Bibcode:1999Natur.402...47P. doi:10.1038/46972. PMID 10573417. S2CID 4431405.
  15. Leys D, Scrutton NS (2004). "Electrical circuitry in biology: emerging principles from protein structure". Curr. Opin. Struct. Biol. 14 (6): 642–7. doi:10.1016/j.sbi.2004.10.002. PMID 15582386.
  16. Boxma B, de Graaf RM, van der Staay GW, van Alen TA, Ricard G, Gabaldón T, van Hoek AH, Moon-van der Staay SY, Koopman WJ, van Hellemond JJ, Tielens AG, Friedrich T, Veenhuis M, Huynen MA, Hackstein JH (2005). "An anaerobic mitochondrion that produces hydrogen" (PDF). Nature. 434 (7029): 74–9. Bibcode:2005Natur.434...74B. doi:10.1038/nature03343. PMID 15744302. S2CID 4401178.
  17. Medical CHEMISTRY Compendium. By Anders Overgaard Pedersen and Henning Nielsen. Aarhus University. 2008
  18. Hirst J (2005). "Energy transduction by respiratory complex I--an evaluation of current knowledge". Biochem. Soc. Trans. 33 (Pt 3): 525–9. doi:10.1042/BST0330525. PMID 15916556.
  19. Lenaz G, Fato R, Genova ML, Bergamini C, Bianchi C, Biondi A (2006). "Mitochondrial Complex I: structural and functional aspects". Biochim. Biophys. Acta. 1757 (9–10): 1406–20. doi:10.1016/j.bbabio.2006.05.007. PMID 16828051.
  20. Sazanov LA, Hinchliffe P (2006). "Structure of the hydrophilic domain of respiratory complex I from Thermus thermophilus". Science. 311 (5766): 1430–6. Bibcode:2006Sci...311.1430S. doi:10.1126/science.1123809. PMID 16469879. S2CID 1892332.
  21. Efremov, RG; Baradaran, R; Sazanov, LA (2010). "The architecture of respiratory complex I". Nature. 465 (7297): 441–5. doi:10.1038/nature09066. PMID 20505720. S2CID 4372778.
  22. Baranova EA, Holt PJ, Sazanov LA (2007). "Projection structure of the membrane domain of Escherichia coli respiratory complex I at 8 A resolution". J. Mol. Biol. 366 (1): 140–54. doi:10.1016/j.jmb.2006.11.026. PMID 17157874.
  23. Friedrich T, Böttcher B (2004). "The gross structure of the respiratory complex I: a Lego System". Biochim. Biophys. Acta. 1608 (1): 1–9. doi:10.1016/j.bbabio.2003.10.002. PMID 14741580.
  24. Hirst J (January 2010). "Towards the molecular mechanism of respiratory complex I". Biochem. J. 425 (2): 327–39. doi:10.1042/BJ20091382. PMID 20025615.
  25. Cecchini G (2003). "Function and structure of complex II of the respiratory chain". Annu. Rev. Biochem. 72: 77–109. doi:10.1146/annurev.biochem.72.121801.161700. PMID 14527321.
  26. Yankovskaya V, Horsefield R, Törnroth S, Luna-Chavez C, Miyoshi H, Léger C, Byrne B, Cecchini G, Iwata S, et al. (2003). "Architecture of succinate dehydrogenase and reactive oxygen species generation". Science. 299 (5607): 700–4. Bibcode:2003Sci...299..700Y. doi:10.1126/science.1079605. PMID 12560550. S2CID 29222766.
  27. Horsefield R, Iwata S, Byrne B (2004). "Complex II from a structural perspective". Curr. Protein Pept. Sci. 5 (2): 107–18. doi:10.2174/1389203043486847. PMID 15078221.
  28. Kita K, Hirawake H, Miyadera H, Amino H, Takeo S (2002). "Role of complex II in anaerobic respiration of the parasite mitochondria from Ascaris suum and Plasmodium falciparum". Biochim. Biophys. Acta. 1553 (1–2): 123–39. doi:10.1016/S0005-2728(01)00237-7. PMID 11803022.
  29. Painter HJ, Morrisey JM, Mather MW, Vaidya AB (2007). "Specific role of mitochondrial electron transport in blood-stage Plasmodium falciparum". Nature. 446 (7131): 88–91. Bibcode:2007Natur.446...88P. doi:10.1038/nature05572. PMID 17330044. S2CID 4421676.
  30. Ramsay RR, Steenkamp DJ, Husain M (1987). "Reactions of electron-transfer flavoprotein and electron-transfer flavoprotein: ubiquinone oxidoreductase". Biochem. J. 241 (3): 883–92. doi:10.1042/bj2410883. PMC 1147643. PMID 3593226.
  31. Zhang J, Frerman FE, Kim JJ (2006). "Structure of electron transfer flavoprotein-ubiquinone oxidoreductase and electron transfer to the mitochondrial ubiquinone pool". Proc. Natl. Acad. Sci. U.S.A. 103 (44): 16212–7. Bibcode:2006PNAS..10316212Z. doi:10.1073/pnas.0604567103. PMC 1637562. PMID 17050691.
  32. Ikeda Y, Dabrowski C, Tanaka K (25 January 1983). "Separation and properties of five distinct acyl-CoA dehydrogenases from rat liver mitochondria. Identification of a new 2-methyl branched chain acyl-CoA dehydrogenase". J. Biol. Chem. 258 (2): 1066–76. PMID 6401712. Archived from the original on 29 September 2007.
  33. Ruzicka FJ, Beinert H (1977). "A new iron-sulfur flavoprotein of the respiratory chain. A component of the fatty acid beta oxidation pathway" (PDF). J. Biol. Chem. 252 (23): 8440–5. PMID 925004. Archived (PDF) from the original on 2007-09-27.
  34. Ishizaki K, Larson TR, Schauer N, Fernie AR, Graham IA, Leaver CJ (2005). "The critical role of Arabidopsis electron-transfer flavoprotein:ubiquinone oxidoreductase during dark-induced starvation". Plant Cell. 17 (9): 2587–600. doi:10.1105/tpc.105.035162. PMC 1197437. PMID 16055629.
  35. Berry EA, Guergova-Kuras M, Huang LS, Crofts AR (2000). "Structure and function of cytochrome bc complexes" (PDF). Annu. Rev. Biochem. 69: 1005–75. CiteSeerX 10.1.1.319.5709. doi:10.1146/annurev.biochem.69.1.1005. PMID 10966481. Archived (PDF) from the original on 2015-12-28.
  36. Crofts AR (2004). "The cytochrome bc1 complex: function in the context of structure". Annu. Rev. Physiol. 66: 689–733. doi:10.1146/annurev.physiol.66.032102.150251. PMID 14977419.
  37. Iwata S, Lee JW, Okada K, Lee JK, Iwata M, Rasmussen B, Link TA, Ramaswamy S, Jap BK (1998). "Complete structure of the 11-subunit bovine mitochondrial cytochrome bc1 complex". Science. 281 (5373): 64–71. Bibcode:1998Sci...281...64I. doi:10.1126/science.281.5373.64. PMID 9651245.
  38. Trumpower BL (1990). "The protonmotive Q cycle. Energy transduction by coupling of proton translocation to electron transfer by the cytochrome bc1 complex" (PDF). J. Biol. Chem. 265 (20): 11409–12. PMID 2164001. Archived (PDF) from the original on 2007-09-27.
  39. Hunte C, Palsdottir H, Trumpower BL (2003). "Protonmotive pathways and mechanisms in the cytochrome bc1 complex". FEBS Lett. 545 (1): 39–46. doi:10.1016/S0014-5793(03)00391-0. PMID 12788490. S2CID 13942619.
  40. Calhoun MW, Thomas JW, Gennis RB (1994). "The cytochrome oxidase superfamily of redox-driven proton pumps". Trends Biochem. Sci. 19 (8): 325–30. doi:10.1016/0968-0004(94)90071-X. PMID 7940677.
  41. Tsukihara T, Aoyama H, Yamashita E, Tomizaki T, Yamaguchi H, Shinzawa-Itoh K, Nakashima R, Yaono R, Yoshikawa S (1996). "The whole structure of the 13-subunit oxidized cytochrome c oxidase at 2.8 A". Science. 272 (5265): 1136–44. Bibcode:1996Sci...272.1136T. doi:10.1126/science.272.5265.1136. PMID 8638158. S2CID 20860573.
  42. Yoshikawa S, Muramoto K, Shinzawa-Itoh K, Aoyama H, Tsukihara T, Shimokata K, Katayama Y, Shimada H (2006). "Proton pumping mechanism of bovine heart cytochrome c oxidase". Biochim. Biophys. Acta. 1757 (9–10): 1110–6. doi:10.1016/j.bbabio.2006.06.004. PMID 16904626.
  43. Rasmusson AG, Soole KL, Elthon TE (2004). "Alternative NAD(P)H dehydrogenases of plant mitochondria". Annu Rev Plant Biol. 55: 23–39. doi:10.1146/annurev.arplant.55.031903.141720. PMID 15725055.
  44. Menz RI, Day DA (1996). "Purification and characterization of a 43-kDa rotenone-insensitive NADH dehydrogenase from plant mitochondria". J. Biol. Chem. 271 (38): 23117–20. doi:10.1074/jbc.271.38.23117. PMID 8798503. S2CID 893754.
  45. McDonald A, Vanlerberghe G (2004). "Branched mitochondrial electron transport in the Animalia: presence of alternative oxidase in several animal phyla". IUBMB Life. 56 (6): 333–41. doi:10.1080/1521-6540400000876. PMID 15370881.
  46. Sluse FE, Jarmuszkiewicz W (1998). "Alternative oxidase in the branched mitochondrial respiratory network: an overview on structure, function, regulation, and role". Braz. J. Med. Biol. Res. 31 (6): 733–47. doi:10.1590/S0100-879X1998000600003. PMID 9698817.
  47. Moore AL, Siedow JN (1991). "The regulation and nature of the cyanide-resistant alternative oxidase of plant mitochondria". Biochim. Biophys. Acta. 1059 (2): 121–40. doi:10.1016/S0005-2728(05)80197-5. PMID 1883834.
  48. Vanlerberghe GC, McIntosh L (1997). "ALTERNATIVE OXIDASE: From Gene to Function". Annu. Rev. Plant Physiol. Plant Mol. Biol. 48: 703–734. doi:10.1146/annurev.arplant.48.1.703. PMID 15012279.
  49. Ito Y, Saisho D, Nakazono M, Tsutsumi N, Hirai A (1997). "Transcript levels of tandem-arranged alternative oxidase genes in rice are increased by low temperature". Gene. 203 (2): 121–9. doi:10.1016/S0378-1119(97)00502-7. PMID 9426242.
  50. Maxwell DP, Wang Y, McIntosh L (1999). "The alternative oxidase lowers mitochondrial reactive oxygen production in plant cells". Proc. Natl. Acad. Sci. U.S.A. 96 (14): 8271–6. Bibcode:1999PNAS...96.8271M. doi:10.1073/pnas.96.14.8271. PMC 22224. PMID 10393984.
  51. Lenaz G (2001). "A critical appraisal of the mitochondrial coenzyme Q pool". FEBS Lett. 509 (2): 151–5. doi:10.1016/S0014-5793(01)03172-6. PMID 11741580. S2CID 46138989.
  52. Heinemeyer J, Braun HP, Boekema EJ, Kouril R (2007). "A structural model of the cytochrome C reductase/oxidase supercomplex from yeast mitochondria". J. Biol. Chem. 282 (16): 12240–8. doi:10.1074/jbc.M610545200. PMID 17322303. S2CID 18123642.
  53. Schägger H, Pfeiffer K (2000). "Supercomplexes in the respiratory chains of yeast and mammalian mitochondria". EMBO J. 19 (8): 1777–83. doi:10.1093/emboj/19.8.1777. PMC 302020. PMID 10775262.
  54. Schägger H (2002). "Respiratory chain supercomplexes of mitochondria and bacteria". Biochim. Biophys. Acta. 1555 (1–3): 154–9. doi:10.1016/S0005-2728(02)00271-2. PMID 12206908.
  55. Schägger H, Pfeiffer K (2001). "The ratio of oxidative phosphorylation complexes I-V in bovine heart mitochondria and the composition of respiratory chain supercomplexes". J. Biol. Chem. 276 (41): 37861–7. doi:10.1074/jbc.M106474200. PMID 11483615. Archived from the original on 2007-09-29.
  56. Gupte S, Wu ES, Hoechli L, Hoechli M, Jacobson K, Sowers AE, Hackenbrock CR (1984). "Relationship between lateral diffusion, collision frequency, and electron transfer of mitochondrial inner membrane oxidation-reduction components". Proc. Natl. Acad. Sci. U.S.A. 81 (9): 2606–10. Bibcode:1984PNAS...81.2606G. doi:10.1073/pnas.81.9.2606. PMC 345118. PMID 6326133.
  57. Nealson KH (1999). "Post-Viking microbiology: new approaches, new data, new insights". Orig Life Evol Biosph. 29 (1): 73–93. Bibcode:1999OLEB...29...73N. doi:10.1023/A:1006515817767. PMID 11536899. S2CID 12289639.
  58. Schäfer G, Engelhard M, Müller V (1999). "Bioenergetics of the Archaea". Microbiol. Mol. Biol. Rev. 63 (3): 570–620. doi:10.1128/MMBR.63.3.570-620.1999. PMC 103747. PMID 10477309.
  59. Ingledew WJ, Poole RK (1984). "The respiratory chains of Escherichia coli". Microbiol. Rev. 48 (3): 222–71. doi:10.1128/mmbr.48.3.222-271.1984. PMC 373010. PMID 6387427.
  60. Unden G, Bongaerts J (1997). "Alternative respiratory pathways of Escherichia coli: energetics and transcriptional regulation in response to electron acceptors". Biochim. Biophys. Acta. 1320 (3): 217–34. doi:10.1016/S0005-2728(97)00034-0. PMID 9230919.
  61. Cecchini G, Schröder I, Gunsalus RP, Maklashina E (2002). "Succinate dehydrogenase and fumarate reductase from Escherichia coli". Biochim. Biophys. Acta. 1553 (1–2): 140–57. doi:10.1016/S0005-2728(01)00238-9. PMID 11803023.
  62. Freitag A, Bock E; Bock (1990). "Energy conservation in Nitrobacter". FEMS Microbiology Letters. 66 (1–3): 157–62. doi:10.1111/j.1574-6968.1990.tb03989.x.
  63. Starkenburg SR, Chain PS, Sayavedra-Soto LA, Hauser L, Land ML, Larimer FW, Malfatti SA, Klotz MG, Bottomley PJ, Arp DJ, Hickey WJ (2006). "Genome sequence of the chemolithoautotrophic nitrite-oxidizing bacterium Nitrobacter winogradskyi Nb-255". Appl. Environ. Microbiol. 72 (3): 2050–63. doi:10.1128/AEM.72.3.2050-2063.2006. PMC 1393235. PMID 16517654.
  64. Yamanaka T, Fukumori Y (1988). "The nitrite oxidizing system of Nitrobacter winogradskyi". FEMS Microbiol. Rev. 54 (4): 259–70. doi:10.1111/j.1574-6968.1988.tb02746.x. PMID 2856189.
  65. Iuchi S, Lin EC (1993). "Adaptation of Escherichia coli to redox environments by gene expression". Mol. Microbiol. 9 (1): 9–15. doi:10.1111/j.1365-2958.1993.tb01664.x. PMID 8412675.
  66. Calhoun MW, Oden KL, Gennis RB, de Mattos MJ, Neijssel OM (1993). "Energetic efficiency of Escherichia coli: effects of mutations in components of the aerobic respiratory chain" (PDF). J. Bacteriol. 175 (10): 3020–5. doi:10.1128/jb.175.10.3020-3025.1993. PMC 204621. PMID 8491720. Archived (PDF) from the original on 2007-09-27.
  67. Boyer PD (1997). "The ATP synthase--a splendid molecular machine". Annu. Rev. Biochem. 66: 717–49. doi:10.1146/annurev.biochem.66.1.717. PMID 9242922.
  68. Van Walraven HS, Strotmann H, Schwarz O, Rumberg B (1996). "The H+/ATP coupling ratio of the ATP synthase from thiol-modulated chloroplasts and two cyanobacterial strains is four". FEBS Lett. 379 (3): 309–13. doi:10.1016/0014-5793(95)01536-1. PMID 8603713. S2CID 35989618.
  69. Yoshida M, Muneyuki E, Hisabori T (2001). "ATP synthase--a marvellous rotary engine of the cell". Nat. Rev. Mol. Cell Biol. 2 (9): 669–77. doi:10.1038/35089509. PMID 11533724. S2CID 3926411.
  70. Schemidt RA, Qu J, Williams JR, Brusilow WS (1998). "Effects of carbon source on expression of F0 genes and on the stoichiometry of the c subunit in the F1F0 ATPase of Escherichia coli". J. Bacteriol. 180 (12): 3205–8. doi:10.1128/jb.180.12.3205-3208.1998. PMC 107823. PMID 9620972.
  71. Nelson N, Perzov N, Cohen A, Hagai K, Padler V, Nelson H (1 January 2000). "The cellular biology of proton-motive force generation by V-ATPases". J. Exp. Biol. 203 (Pt 1): 89–95. PMID 10600677. Archived from the original on 30 September 2007.
  72. Rubinstein JL, Walker JE, Henderson R (2003). "Structure of the mitochondrial ATP synthase by electron cryomicroscopy". EMBO J. 22 (23): 6182–92. doi:10.1093/emboj/cdg608. PMC 291849. PMID 14633978.
  73. Leslie AG, Walker JE (2000). "Structural model of F1-ATPase and the implications for rotary catalysis". Philos. Trans. R. Soc. Lond. B Biol. Sci. 355 (1396): 465–71. doi:10.1098/rstb.2000.0588. PMC 1692760. PMID 10836500.
  74. Noji H, Yoshida M (2001). "The rotary machine in the cell, ATP synthase". J. Biol. Chem. 276 (3): 1665–8. doi:10.1074/jbc.R000021200. PMID 11080505. S2CID 30953216.
  75. Capaldi RA, Aggeler R (2002). "Mechanism of the F(1)F(0)-type ATP synthase, a biological rotary motor". Trends Biochem. Sci. 27 (3): 154–60. doi:10.1016/S0968-0004(01)02051-5. PMID 11893513.
  76. Dimroth P, von Ballmoos C, Meier T (2006). "Catalytic and mechanical cycles in F-ATP synthases. Fourth in the Cycles Review Series". EMBO Rep. 7 (3): 276–82. doi:10.1038/sj.embor.7400646. PMC 1456893. PMID 16607397.
  77. Gresser MJ, Myers JA, Boyer PD (25 October 1982). "Catalytic site cooperativity of beef heart mitochondrial F1 adenosine triphosphatase. Correlations of initial velocity, bound intermediate, and oxygen exchange measurements with an alternating three-site model". J. Biol. Chem. 257 (20): 12030–8. PMID 6214554. Archived from the original on 29 September 2007.
  78. Dimroth P (1994). "Bacterial sodium ion-coupled energetics". Antonie van Leeuwenhoek. 65 (4): 381–95. doi:10.1007/BF00872221. PMID 7832594. S2CID 23763996.
  79. Becher B, Müller V (1994). "Delta mu Na+ drives the synthesis of ATP via an delta mu Na(+)-translocating F1F0-ATP synthase in membrane vesicles of the archaeon Methanosarcina mazei Gö1". J. Bacteriol. 176 (9): 2543–50. doi:10.1128/jb.176.9.2543-2550.1994. PMC 205391. PMID 8169202.
  80. Müller V (2004). "An exceptional variability in the motor of archael A1A0 ATPases: from multimeric to monomeric rotors comprising 6-13 ion binding sites". J. Bioenerg. Biomembr. 36 (1): 115–25. doi:10.1023/B:JOBB.0000019603.68282.04. PMID 15168615. S2CID 24887884.
  81. Davies KJ (1995). "Oxidative stress: the paradox of aerobic life". Biochem. Soc. Symp. 61: 1–31. doi:10.1042/bss0610001. PMID 8660387.
  82. Rattan SI (2006). "Theories of biological aging: genes, proteins, and free radicals" (PDF). Free Radic. Res. 40 (12): 1230–8. CiteSeerX 10.1.1.476.9259. doi:10.1080/10715760600911303. PMID 17090411. S2CID 11125090. Archived from the original (PDF) on 2014-06-14. Retrieved 2017-10-27.
  83. Valko M, Leibfritz D, Moncol J, Cronin MT, Mazur M, Telser J (2007). "Free radicals and antioxidants in normal physiological functions and human disease". Int. J. Biochem. Cell Biol. 39 (1): 44–84. doi:10.1016/j.biocel.2006.07.001. PMID 16978905.
  84. Raha S, Robinson BH (2000). "Mitochondria, oxygen free radicals, disease and ageing". Trends Biochem. Sci. 25 (10): 502–8. doi:10.1016/S0968-0004(00)01674-1. PMID 11050436.
  85. Finkel T, Holbrook NJ (2000). "Oxidants, oxidative stress and the biology of ageing". Nature. 408 (6809): 239–47. Bibcode:2000Natur.408..239F. doi:10.1038/35041687. PMID 11089981. S2CID 2502238.
  86. Kadenbach B, Ramzan R, Wen L, Vogt S (March 2010). "New extension of the Mitchell Theory for oxidative phosphorylation in mitochondria of living organisms". Biochim. Biophys. Acta. 1800 (3): 205–12. doi:10.1016/j.bbagen.2009.04.019. PMID 19409964.
  87. Echtay KS, Roussel D, St-Pierre J, Jekabsons MB, Cadenas S, Stuart JA, Harper JA, Roebuck SJ, Morrison A, Pickering S, Clapham JC, Brand MD (January 2002). "Superoxide activates mitochondrial uncoupling proteins". Nature. 415 (6867): 96–9. Bibcode:2002Natur.415...96E. doi:10.1038/415096a. PMID 11780125. S2CID 4349744.
  88. Devaux, JBL; Hedges, CP; Hickey, AJR (January 2019). "Acidosis Maintains the Function of Brain Mitochondria in Hypoxia-Tolerant Triplefin Fish: A Strategy to Survive Acute Hypoxic Exposure?". Front Physiol. 9, 1914: 1941. doi:10.3389/fphys.2018.01941. PMC 6346031. PMID 30713504.
  89. Joshi S, Huang YG (1991). "ATP synthase complex from bovine heart mitochondria: the oligomycin sensitivity conferring protein is essential for dicyclohexyl carbodiimide-sensitive ATPase". Biochim. Biophys. Acta. 1067 (2): 255–8. doi:10.1016/0005-2736(91)90051-9. PMID 1831660.
  90. Satyanarayana, U. (2002). Biochemistry (2nd ed.). Kolkata, India: Books and Allied. ISBN 8187134801. OCLC 71209231.
  91. Tsubaki M (1993). "Fourier-transform infrared study of cyanide binding to the Fea3-CuB binuclear site of bovine heart cytochrome c oxidase: implication of the redox-linked conformational change at the binuclear site". Biochemistry. 32 (1): 164–73. doi:10.1021/bi00052a022. PMID 8380331.
  92. Heytler PG (1979). "Uncouplers of oxidative phosphorylation". Meth. Enzymol. Methods in Enzymology. 55: 462–42. doi:10.1016/0076-6879(79)55060-5. ISBN 978-0-12-181955-2. PMID 156853.
  93. Lambert AJ, Brand MD (2004). "Inhibitors of the quinone-binding site allow rapid superoxide production from mitochondrial NADH:ubiquinone oxidoreductase (complex I)". J. Biol. Chem. 279 (38): 39414–20. doi:10.1074/jbc.M406576200. PMID 15262965. S2CID 26620903.
  94. Dervartanian DV, Veeger C (November 1964). "Studies on succinate dehydrogenase: I. Spectral properties of the purified enzyme and formation of enzyme-competitive inhibitor complexes". Biochim. Biophys. Acta. 92 (2): 233–47. doi:10.1016/0926-6569(64)90182-8. PMID 14249115.
  95. Ricquier D, Bouillaud F (2000). "The uncoupling protein homologues: UCP1, UCP2, UCP3, StUCP and AtUCP". Biochem. J. 345 (2): 161–79. doi:10.1042/0264-6021:3450161. PMC 1220743. PMID 10620491.
  96. Borecký J, Vercesi AE (2005). "Plant uncoupling mitochondrial protein and alternative oxidase: energy metabolism and stress". Biosci. Rep. 25 (3–4): 271–86. doi:10.1007/s10540-005-2889-2. PMID 16283557. S2CID 18598358.
  97. Harden A, Young WJ.; Young (1906). "The alcoholic ferment of yeast-juice". Proceedings of the Royal Society. B (77): 405–20. doi:10.1098/rspb.1906.0029.
  98. Kalckar HM (1974). "Origins of the concept oxidative phosphorylation". Mol. Cell. Biochem. 5 (1–2): 55–63. doi:10.1007/BF01874172. PMID 4279328. S2CID 26999163.
  99. Lipmann F (1941). "Metabolic generation and utilization of phosphate bond energy". Adv Enzymol. 1: 99–162. doi:10.4159/harvard.9780674366701.c141. ISBN 9780674366701.
  100. Friedkin M, Lehninger AL (1 April 1949). "Esterification of inorganic phosphate coupled to electron transport between dihydrodiphosphopyridine nucleotide and oxygen". J. Biol. Chem. 178 (2): 611–44. PMID 18116985. Archived from the original on 16 December 2008.
  101. Kalckar, H. M. (1991). "50 years of biological research--from oxidative phosphorylation to energy requiring transport regulation". Annual Review of Biochemistry. 60: 1–37. doi:10.1146/annurev.bi.60.070191.000245. PMID 1883194.
  102. Belitser, V. A.; Tsibakova, E. T. (1939). "About phosphorilation mechanism coupled with respiration". Biokhimiya. 4: 516–534.
  103. Slater EC (1953). "Mechanism of phosphorylation in the respiratory chain". Nature. 172 (4387): 975–8. Bibcode:1953Natur.172..975S. doi:10.1038/172975a0. PMID 13111237. S2CID 4153659.
  104. Mitchell P (1961). "Coupling of phosphorylation to electron and hydrogen transfer by a chemi-osmotic type of mechanism". Nature. 191 (4784): 144–8. Bibcode:1961Natur.191..144M. doi:10.1038/191144a0. PMID 13771349. S2CID 1784050.
  105. Milton H. Saier Jr. Peter Mitchell and the Vital Force. OCLC 55202414.
  106. Mitchell, Peter (1978). "David Keilin's Respiratory Chain Concept and Its Chemiosmotic Consequences" (PDF). Nobel lecture. Nobel Foundation. Archived (PDF) from the original on 2007-09-27. Retrieved 2007-07-21.
  107. Pullman ME, Penefsky HS, Datta A, Racker E (1 November 1960). "Partial resolution of the enzymes catalyzing oxidative phosphorylation. I. Purification and properties of soluble dinitrophenol-stimulated adenosine triphosphatase". J. Biol. Chem. 235 (11): 3322–9. PMID 13738472. Archived from the original on 29 September 2007.
  108. Boyer PD, Cross RL, Momsen W (1973). "A new concept for energy coupling in oxidative phosphorylation based on a molecular explanation of the oxygen exchange reactions". Proc. Natl. Acad. Sci. U.S.A. 70 (10): 2837–9. Bibcode:1973PNAS...70.2837B. doi:10.1073/pnas.70.10.2837. PMC 427120. PMID 4517936.
  109. "The Nobel Prize in Chemistry 1997". Nobel Foundation. Archived from the original on 2017-03-25. Retrieved 2007-07-21.

Further reading

Introductory
  • Nelson DL; Cox MM (2004). Lehninger Principles of Biochemistry (4th ed.). W. H. Freeman. ISBN 0-7167-4339-6.
  • Schneider ED; Sagan D (2006). Into the Cool: Energy Flow, Thermodynamics and Life (1st ed.). University of Chicago Press. ISBN 0-226-73937-6.
  • Lane N (2006). Power, Sex, Suicide: Mitochondria and the Meaning of Life (1st ed.). Oxford University Press, USA. ISBN 0-19-920564-7.

Advanced
  • Nicholls DG; Ferguson SJ (2002). Bioenergetics 3 (1st ed.). Academic Press. ISBN 0-12-518121-3.
  • Haynie D (2001). Biological Thermodynamics (1st ed.). Cambridge University Press. ISBN 0-521-79549-4.
  • Rajan SS (2003). Introduction to Bioenergetics (1st ed.). Anmol. ISBN 81-261-1364-2.
  • Wikstrom M (Ed) (2005). Biophysical and Structural Aspects of Bioenergetics (1st ed.). Royal Society of Chemistry. ISBN 0-85404-346-2.CS1 maint: extra text: authors list (link)

General resources

Structural resources

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