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Electron transport chain

The electron transport chain (ETC), also known as the respiratory chain, is a series of membrane-bound protein complexes and mobile electron carriers that transfer high-energy electrons derived from NADH and FADH₂ to molecular oxygen (O₂), the terminal electron acceptor, while simultaneously pumping protons across the inner mitochondrial membrane to establish an electrochemical gradient essential for ATP production via oxidative phosphorylation.^[1] This process occurs primarily in the mitochondria of eukaryotic cells and represents the final stage of aerobic cellular respiration, efficiently converting the energy from nutrient breakdown into usable ATP, with approximately 30–32 molecules of ATP generated per glucose molecule oxidized.^[1] In prokaryotes, a similar ETC operates in the plasma membrane, and analogous systems exist in chloroplasts for photosynthesis. The ETC comprises four large protein complexes (I–IV), along with the lipid-soluble carrier ubiquinone (coenzyme Q) and the water-soluble cytochrome c, all embedded in or associated with the inner mitochondrial membrane. Complex I (NADH dehydrogenase) initiates the chain by accepting electrons from NADH (produced in the citric acid cycle and glycolysis), passing them through iron-sulfur clusters and flavin mononucleotide (FMN) to reduce ubiquinone while translocating four protons per two electrons.^[1] Complex II (succinate dehydrogenase), the only complex not pumping protons directly, feeds electrons from FADH₂ (generated in the citric acid cycle) into ubiquinone without contributing to the initial proton gradient.^[1] Electrons then move via reduced ubiquinone to Complex III (cytochrome bc₁ complex), which uses the Q-cycle mechanism to transfer them to cytochrome c while pumping four additional protons. Finally, Complex IV (cytochrome c oxidase) accepts electrons from cytochrome c, reduces O₂ to water, and pumps two more protons, completing the chain and preventing electron leakage that could generate harmful reactive oxygen species (ROS).^[1] Beyond ATP synthesis, the ETC plays critical roles in cellular homeostasis, including ROS production as a byproduct (primarily at Complexes I and III), which serves as signaling molecules but can contribute to oxidative stress, aging, and diseases like Parkinson's when dysregulated. Recent structural studies, including cryo-electron microscopy of supercomplexes (e.g., I₁III₂IV₁), have revealed how these assemblies enhance electron transfer efficiency through substrate channeling and stabilization by cardiolipin lipids, underscoring the ETC's evolutionary optimization for energy conservation. Disruptions in ETC function, such as mutations in complex subunits, are implicated in mitochondrial disorders, highlighting its indispensability for aerobic life.^[1]

Introduction

Definition and biological role

The electron transport chain (ETC) is a series of multi-protein complexes embedded in cellular membranes that catalyze sequential redox reactions, transferring electrons from donor molecules to acceptor molecules while coupling this process to proton translocation across the membrane.^[1] In eukaryotic cells, the ETC resides in the inner mitochondrial membrane; in prokaryotes, it is located in the plasma membrane; and in photosynthetic organisms, it occurs in the thylakoid membrane of chloroplasts.^[2] This conserved mechanism underpins oxidative phosphorylation in respiration and photophosphorylation in photosynthesis, enabling efficient energy conversion across diverse life forms.^[3] The primary biological role of the ETC is to generate a proton motive force—an electrochemical gradient (Δp) across the membrane—through proton pumping driven by exergonic electron transfers, which powers ATP synthesis via ATP synthase.^[1] In aerobic respiration, electrons derived from NADH and FADH₂ (produced in glycolysis, the citric acid cycle, and fatty acid oxidation) flow through the chain to oxygen as the terminal acceptor, yielding water and facilitating the production of approximately 30–32 ATP molecules per glucose molecule oxidized.^[4] The overall reaction for the mitochondrial ETC can be summarized as:
\ce{NADH + 1/2 O2 + H+ -> NAD+ + H2O}
(with associated proton pumping omitted for simplicity).^[1] In photosynthesis, electrons originate from water (split by light energy) and are transferred via photosystems to NADP⁺, producing NADPH and oxygen, while the proton gradient drives ATP formation essential for carbon fixation.^[5] This universal process is vital for cellular energy homeostasis, as disruptions in the ETC can impair ATP production and lead to metabolic disorders, underscoring its evolutionary conservation from bacteria to higher eukaryotes.^[6]

Historical background

The discovery of the electron transport chain (ETC) emerged from early 20th-century studies on cellular respiration. In the 1920s, Otto Warburg investigated oxygen consumption in living cells using manometric techniques, revealing that respiration involves an iron-containing enzyme that facilitates atmospheric oxygen reduction, for which he received the 1931 Nobel Prize in Physiology or Medicine.^[7] Concurrently, David Keilin identified cytochromes as key respiratory pigments in 1925, observing their characteristic absorption bands in yeast, insects, and vertebrates, establishing them as ubiquitous components of aerobic respiration.^[8] In the 1940s and 1950s, advances in mitochondrial isolation enabled fractionation and component identification. David E. Green and colleagues developed methods to disrupt mitochondria into functional assemblies, isolating the "cyclophorase" system in 1951 that integrated the citric acid cycle with oxidative phosphorylation.^[9] Britton Chance applied rapid-mixing spectroscopy to elucidate cytochrome kinetics, demonstrating sequential redox reactions in the respiratory chain during the 1950s. The role of quinones was clarified with the 1957 discovery of ubiquinone (coenzyme Q) by Frederick L. Crane, David E. Green, and associates, who isolated it from beef heart mitochondria as a lipid-soluble electron carrier essential for NADH and succinate oxidation.^[10] Efraim Racker's group isolated the F1 portion of ATP synthase from mitochondria in 1960, reconstituting it into vesicles to confirm its role in ATP synthesis.^[11] Peter Mitchell proposed the chemiosmotic hypothesis in 1961, positing that ETC-driven proton translocation across the inner mitochondrial membrane generates an electrochemical gradient powering ATP synthesis, a concept validated over the next decade and awarded the 1978 Nobel Prize in Chemistry.^[12] The 1970s and 1980s saw structural insights through spectroscopy and early crystallography; for instance, spectroscopic studies in the 1970s and 1980s mapped electron pathways in Complex I (NADH:ubiquinone oxidoreductase). Recent decades have benefited from cryo-electron microscopy (cryo-EM) for high-resolution structures. Judy Hirst's laboratory determined the near-atomic structure of mammalian Complex I in 2016, revealing its L-shaped architecture and proton-pumping mechanism. In the 2020s, single-molecule techniques have provided dynamic views; for example, tracking of bacterial outer-membrane cytochromes in 2021 illuminated redox protein diffusion and electron transfer rates in respiratory chains. These milestones continue to refine our understanding of ETC assembly and function.

General principles

Redox carriers and electron transfer

The electron transport chain (ETC) relies on a series of redox carriers that facilitate the transfer of electrons from high-energy donors like NADH to the terminal acceptor oxygen. These carriers are prosthetic groups embedded within membrane-bound protein complexes or mobile within the lipid bilayer. Key types include flavins such as flavin mononucleotide (FMN) and flavin adenine dinucleotide (FAD), which accept two electrons and two protons from substrates like NADH or succinate, forming semiquinone intermediates before passing electrons singly. Iron-sulfur (Fe-S) clusters, consisting of 2Fe-2S or 4Fe-4S configurations, serve as one-electron carriers with variable redox potentials tuned to sequential steps in the chain. Heme groups in cytochromes (b, c, a types) coordinate iron atoms that cycle between Fe³⁺ and Fe²⁺ states, enabling one-electron transfers, while copper centers in the terminal oxidase handle electron delivery to O₂. Quinones, particularly ubiquinone (coenzyme Q), act as lipid-soluble mobile carriers that shuttle two electrons and protons between complexes, cycling between oxidized ubiquinone and reduced ubiquinol forms.^[2]^[13] Electron transfer in the ETC proceeds sequentially through these carriers in a downhill redox potential gradient, ensuring exergonic flow. NADH donates two electrons to FMN in Complex I via a one-electron semiquinone step, followed by transfers to Fe-S clusters and then to ubiquinone, which accepts two electrons to form ubiquinol. Ubiquinol diffuses to the next complex, where it donates electrons—one via an Fe-S cluster to a cytochrome c heme, and the other through a bifurcated path involving additional hemes. Cytochrome c, another mobile one-electron carrier, relays electrons to copper centers and hemes in the terminal oxidase, reducing O₂ to H₂O. This process involves both one- and two-electron steps, with carriers insulated by protein scaffolds to direct flow and prevent leakage, often via quantum tunneling across short distances up to 2 nm. The overall gradient spans from the low potential of NADH/NAD⁺ (E°' ≈ -320 mV) to the high potential of O₂/H₂O (E°' ≈ +820 mV), driving irreversible electron flow.^[2]^[14]^[2] The redox potential difference (ΔE) between electron acceptor and donor dictates the feasibility and energy yield of each transfer, calculated as ΔE = E°'_acceptor - E°'_donor. For the full NADH to O₂ span, ΔE ≈ 1.14 V, making the reaction highly favorable. The associated standard free energy change is given by ΔG°' = -nFΔE, where n is the number of electrons transferred (typically 2 for NADH), and F is the Faraday constant (96.485 kJ/mol/V). This yields ΔG°' ≈ -220 kJ/mol for NADH oxidation, releasing energy in discrete steps to avoid dissipation as heat. In mitochondrial systems, this energy couples to proton translocation, with approximately 10 protons pumped across the membrane per NADH oxidized—4 at Complex I, 4 at Complex III, and 2 at Complex IV—establishing the proton motive force.^[15]^[2]^[1] A specialized mechanism amplifying proton translocation occurs in Complex III via the Q-cycle, a two-step process of quinone oxidation and reduction. In the first step, ubiquinol at the Qo site donates one electron to the Rieske Fe-S center (leading to cytochrome c) and the other to a low-potential heme b, releasing two protons to the intermembrane space. The second electron reduces another ubiquinone at the Qi site, taking up two protons from the matrix to form semiquinol, which in a subsequent cycle fully reduces to ubiquinol. This bifurcation effectively translocates 4 H⁺ per 2 electrons transferred (beyond scalar protons), doubling the proton/electron stoichiometry compared to linear transfer. The Q-cycle thus enhances bioenergetic efficiency without additional energy input.^[14]^[2]

Proton translocation and chemiosmosis

Proton translocation in the electron transport chain occurs through two primary mechanisms: vectorial transport driven by conformational changes in membrane-bound complexes and redox-linked scalar proton release or uptake associated with quinone chemistry. In complexes such as Complex I, electron transfer induces long-range conformational changes that propagate across the protein, facilitating the active pumping of protons from the matrix to the intermembrane space via dedicated proton channels.^[16] This vectorial mechanism ensures that proton movement is tightly coupled to the redox reactions without direct scalar release. In contrast, redox-linked translocation, exemplified by the Q-cycle in Complex III, involves the scalar protons liberated or consumed during the reduction and oxidation of ubiquinone at the quinone-binding sites, contributing to net proton displacement across the membrane.^[2] The primary sites of proton pumping in the mitochondrial electron transport chain are Complexes I, III, and IV, where electron transfer from NADH ultimately results in the translocation of 10 protons per two electrons (H⁺/2e⁻) into the intermembrane space.^[17] This collective pumping establishes an electrochemical gradient that stores the energy derived from electron flow. Complex II does not contribute to proton pumping, as its role is limited to electron transfer without associated translocation. The chemiosmotic theory, proposed by Peter Mitchell, posits that the proton gradient generated by these translocation events forms a proton motive force (Δp) comprising a membrane potential (Δψ) and a pH gradient (ΔpH), which drives ATP synthesis through indirect osmotic coupling rather than direct chemical intermediates. This delocalized mechanism allows the gradient to power processes across the membrane without requiring physical linkage between electron transport and phosphorylation sites. The proton motive force is quantitatively expressed as:

\Delta p = \Delta \psi - 2.303 \frac{RT}{F} \Delta \mathrm{pH}

where Δp and Δψ are in millivolts, R is the gas constant, T is temperature in Kelvin, F is the Faraday constant, and ΔpH is the difference between internal and external pH (positive when the matrix is more alkaline).^[12] In mitochondria, the membrane potential component (Δψ) typically ranges from 150 to 200 mV, negative inside relative to the intermembrane space, reflecting the high energetic barrier protons must overcome to re-enter the matrix.^[18] In prokaryotes, this gradient also maintains cytoplasmic pH homeostasis by counteracting environmental acidity through proton influx.

Mitochondrial electron transport chain

Complex I: NADH:ubiquinone oxidoreductase

Complex I, also known as NADH:ubiquinone oxidoreductase, serves as the entry point for electrons from NADH into the mitochondrial electron transport chain, linking catabolic pathways like the tricarboxylic acid cycle to oxidative phosphorylation. It catalyzes the transfer of two electrons from NADH to ubiquinone while translocating protons across the inner mitochondrial membrane, thereby contributing to the electrochemical gradient essential for ATP synthesis.^[19] The enzyme exhibits an L-shaped architecture, with a hydrophilic peripheral arm projecting into the mitochondrial matrix and a hydrophobic membrane arm integrated into the lipid bilayer. In mammalian mitochondria, Complex I consists of 45 subunits totaling approximately 1 MDa, including 14 conserved core subunits critical for electron transfer and proton pumping—seven of which (ND1–ND6 and ND4L) are encoded by mitochondrial DNA, while the remainder are nuclear-encoded. The peripheral arm, primarily composed of nuclear-encoded subunits, accommodates the NADH oxidation site, a flavin mononucleotide (FMN) cofactor, and eight iron-sulfur (Fe-S) clusters arranged in a linear chain. The membrane arm, dominated by mitochondrially encoded subunits, harbors the ubiquinone (Q) binding pocket and four putative proton channels formed by antiporter-like structures in ND2, ND4, and ND5. High-resolution cryo-electron microscopy structures have elucidated these features, revealing intricate subunit interfaces and cofactor positions.^[19]^[20]^[21] Complex I oxidizes NADH to NAD⁺ in the matrix, reducing ubiquinone to ubiquinol (QH₂) at the membrane domain and pumping four protons (4 H⁺/2 e⁻) from the matrix to the intermembrane space. This process establishes a proton motive force without net consumption of matrix protons beyond the reaction stoichiometry. The balanced equation is:

\text{NADH} + \text{[Q](/page/Q)} + 5\text{H}^+_\text{matrix} \to \text{NAD}^+ + \text{QH}_2 + 4\text{H}^+_\text{intermembrane}

Electrons flow sequentially from NADH to FMN, through the eight Fe-S clusters (seven participating in transfer, one structural), and finally to Q, with midpoint redox potentials increasing from approximately −320 mV (NADH/NAD⁺) to +90 mV (Q/QH₂) to drive the exergonic transfer.^[19]^[22] Proton pumping is coupled to Q reduction via a mechanism involving conformational rearrangements that propagate as an electrostatic "wave" across the membrane arm. Reduction of Q induces loop movements in the Q-binding cavity, tilting transmembrane helices in ND1 and rotating the ND6 subunit, which in turn facilitates proton release through coordinated water networks and charged residues in the antiporter subunits. This indirect coupling avoids short-circuiting the redox reaction while ensuring efficient energy transduction.^[23]^[24] Beyond the core subunits, approximately 31 accessory proteins provide structural stability, facilitate biogenesis via dedicated assembly factors, and modulate activity under physiological stress. Mutations in Complex I genes, particularly in core subunits like NDUFS1 or mtDNA-encoded ND genes, disrupt assembly or function and are implicated in mitochondrial diseases, including neurodegenerative conditions such as Leigh syndrome.^[19]^[25]

Complex II: Succinate:ubiquinone oxidoreductase

Complex II, also known as succinate:ubiquinone oxidoreductase or succinate dehydrogenase, is a heterotetrameric enzyme complex embedded in the inner mitochondrial membrane, consisting of four nuclear-encoded subunits: SDHA, SDHB, SDHC, and SDHD.^[26] The SDHA subunit, a flavoprotein, binds flavin adenine dinucleotide (FAD) at its active site and catalyzes the oxidation of succinate to fumarate, while SDHB serves as the iron-sulfur protein subunit containing three iron-sulfur clusters ([2Fe-2S], [4Fe-4S], and [3Fe-4S]) that facilitate electron transfer.^[26] The membrane-anchoring subunits SDHC and SDHD form a heterodimer that harbors the ubiquinone-binding site at their interface, but unlike other respiratory complexes, Complex II lacks proton-translocating channels or membrane-spanning helices dedicated to pumping.^[27] In its primary function, Complex II links the tricarboxylic acid (TCA) cycle to the electron transport chain by oxidizing succinate to fumarate in the TCA cycle while reducing ubiquinone (Q) to ubiquinol (QH₂) in the respiratory chain, serving as a dual-role enzyme without net proton translocation across the membrane.01789-1/fulltext) The overall reaction is:

\text{Succinate} + \text{Q} \rightarrow \text{Fumarate} + \text{QH}_2

This process bypasses Complex I, delivering electrons directly to the ubiquinone pool and subsequently to Complex III, resulting in a lower ATP yield of approximately 1.5 ATP per pair of electrons compared to 2.5 ATP from NADH oxidation via Complex I, due to fewer protons pumped downstream.^[1] The redox potentials are tuned for efficient electron transfer, with the succinate/fumarate couple at E°' = +30 mV and the ubiquinone/ubiquinol couple at approximately +90 mV, ensuring thermodynamically favorable reduction of Q.^[28]^[29] A unique aspect of Complex II is its exclusive position as the only TCA cycle enzyme that directly participates in the electron transport chain, integrating carbon metabolism with respiration.01789-1/fulltext) Germline mutations in the SDH subunit genes (SDHA, SDHB, SDHC, SDHD) are associated with hereditary paraganglioma-pheochromocytoma syndromes, where impaired Complex II activity disrupts succinate metabolism and stabilizes hypoxia-inducible factors, promoting tumorigenesis.^[30]

Complex III: Ubiquinol:cytochrome c oxidoreductase

Complex III, also known as ubiquinol:cytochrome c oxidoreductase or the cytochrome bc1 complex, is a dimeric integral membrane protein embedded in the inner mitochondrial membrane.^[31] Each monomer consists of 11 subunits in mammalian mitochondria, including three core redox-active subunits: cytochrome b (encoded by mtDNA), cytochrome c1, and the Rieske iron-sulfur protein (RISP), along with eight additional nuclear-encoded subunits that provide structural stability.^[32] The dimer formation, with each monomer featuring four metal centers—hemes b_H and b_L in cytochrome b, heme c1 in cytochrome c1, and a [2Fe-2S] cluster in RISP—facilitates efficient electron transfer and is essential for the enzyme's stability and function within respiratory supercomplexes.^[33] The primary function of Complex III is to oxidize ubiquinol (QH₂) at the Qo site on the intermembrane space side and transfer electrons to cytochrome c, while simultaneously translocating protons across the membrane to contribute to the proton motive force.^[32] This process involves bifurcating the two electrons from QH₂: one follows the high-potential chain through the RISP [2Fe-2S] cluster to heme c1 and then to cytochrome c, while the other traverses the low-potential chain via hemes b_L and b_H to reduce ubiquinone (Q) at the Qi site on the matrix side.^[31] Through this mechanism, Complex III achieves a proton-to-electron stoichiometry of 4 H⁺ translocated per 2 electrons transferred, amplifying the electrochemical gradient essential for ATP synthesis.^[34] The Q-cycle is the hallmark mechanism of Complex III, enabling proton amplification by coupling quinol oxidation and quinone reduction in a cyclic manner. At the Qo site, the first QH₂ molecule binds and undergoes oxidation: one electron is transferred to the RISP [2Fe-2S] cluster (the rate-limiting step, with a timescale of approximately 770 µs), reducing it and leading to the formation of a transient, unstable semiquinone anion (SQ⁻, with low steady-state occupancy around 0.01); this electron then passes to heme c1 and cytochrome c, releasing two protons into the intermembrane space.^[31] The second electron from the semiquinone reduces heme b_L, which relays it to heme b_H and ultimately to a ubiquinone at the Qi site, forming a semiquinone intermediate. A second QH₂ oxidation at Qo repeats the process, providing the second electron to fully reduce the Qi semiquinone to QH₂, taking up two protons from the matrix. This bifurcation and recycling ensure that two cytochrome c molecules are reduced per net QH₂ oxidized, without net consumption at Qi.^[33]^[32] The net reaction catalyzed by Complex III, encompassing one full Q-cycle, is:

\mathrm{QH_2 + 2\ cyt\ c^{3+} + 2\ H^+_{matrix} \to Q + 2\ cyt\ c^{2+} + 4\ H^+_{intermembrane}}

This equation reflects the overall electron transfer from ubiquinol to two molecules of oxidized cytochrome c, with enhanced proton release due to the Q-cycle.^[31]^[32] Unique aspects of Complex III include its two distinct quinone-binding sites: the Qo site, which accommodates stigmatellin binding to inhibit quinol oxidation near the RISP cluster, and the Qi site, targeted by antimycin to block electron transfer from heme b_H.^[33] The dimeric architecture not only supports intra-monomer electron transfer (with edge-to-edge distances of about 7-10 Å between hemes) but is also crucial for assembly into supercomplexes with Complexes I and IV, which stabilize the respiratory chain and optimize electron flux while minimizing reactive oxygen species production.^[32] The mobility of the RISP extrinsic domain further enables conformational changes essential for Qo site access and efficient bifurcation during the Q-cycle.^[31]

Complex IV: Cytochrome c oxidase

Complex IV, also known as cytochrome c oxidase, is the terminal enzyme of the mitochondrial electron transport chain in eukaryotic cells, consisting of 13 to 14 subunits in mammalian forms, with a catalytic core formed by three mitochondrially encoded subunits (MT-CO1, MT-CO2, and MT-CO3) and the rest as nuclear-encoded supernumerary subunits that stabilize the structure and regulate activity.^[35] The MT-CO1 subunit houses heme a and the binuclear center (heme a₃ coordinated to Cu_B), while MT-CO2 contains the Cu_A binuclear copper center, and assembly requires specific chaperones for insertion of these metal cofactors into the membrane-embedded complex.^[36] These supernumerary subunits, such as COX4 and COX5, form a supramolecular assembly that positions the enzyme for efficient electron transfer from cytochrome c and proton translocation.^[35] The primary function of cytochrome c oxidase is to catalyze the four-electron reduction of molecular oxygen to two molecules of water, utilizing electrons from four reduced cytochrome c molecules, while contributing to the proton motive force by translocating protons across the inner mitochondrial membrane.^[37] This reaction consumes four protons from the matrix for scalar chemistry and pumps an additional four protons to the intermembrane space per oxygen reduced, though the pumped proton stoichiometry per two electrons (2-4 H⁺/2e^-) has been debated, with experimental evidence supporting a total of four vectorial protons per O₂ alongside the scalar protons.^[37] The overall balanced equation is:

$4 \ \ce{cyt \ c^{2+}} + \ce{O2} + 8 \ce{H+_{matrix}} \rightarrow 4 \ \ce{cyt \ c^{3+}} + 2 \ce{H2O} + 4 \ce{H+_{intermembrane}}

This process ensures complete reduction of O₂ without releasing harmful intermediates and links exergonic electron transfer to energy conservation via the proton gradient.^[38] The catalytic mechanism involves sequential electron transfer from reduced cytochrome c docked at the extramembranous domain of subunit MT-CO2 to the Cu_A center, which relays electrons through heme a in MT-CO1 to the binuclear center (heme a₃-Cu_B), where O₂ binds to ferrous heme a₃ and undergoes four-electron reduction with concomitant cleavage of the O-O bond to form water.^[39] Proton loading sites and channels, including the D-pathway in MT-CO1, facilitate both chemical proton uptake for water formation and pumped proton ejection, with the redox-driven conformational changes at the binuclear center ensuring vectorial transport without back-leakage.^[37] This tightly coupled electron-proton transfer prevents reactive oxygen species formation during O₂ activation.^[39] Cytochrome c oxidase activity is allosterically regulated by the ATP/ADP ratio, where ATP binds to nuclear-encoded subunits like COX3 to inhibit electron transfer and respiration when cellular energy is high, while ADP relieves this inhibition to accelerate turnover.^[40] The enzyme is reversibly inhibited by nitric oxide (NO) at nanomolar concentrations, which competitively binds the binuclear center with O₂ to modulate mitochondrial respiration in response to signaling, and by carbon monoxide (CO), which similarly targets the reduced heme a₃ to suppress activity.^[41]^[42] In brown adipose tissue, cytochrome c oxidase supports non-shivering thermogenesis by maintaining high electron flux rates that, coupled with uncoupling protein 1, dissipate the proton gradient as heat rather than ATP synthesis.^[43]

Mobile electron carriers: Ubiquinone and cytochrome c

Ubiquinone, also known as coenzyme Q or CoQ, is a lipid-soluble molecule embedded in the inner mitochondrial membrane that serves as a mobile electron carrier in the electron transport chain (ETC).^[44] It consists of a redox-active benzoquinone ring attached to a polyisoprenoid tail, which in humans comprises 10 isoprene units (CoQ₁₀), conferring hydrophobicity and enabling diffusion within the membrane lipid bilayer.^[45] Ubiquinone cycles between its oxidized form (Q) and reduced form (QH₂, ubiquinol) as it accepts two electrons and two protons from upstream complexes, such as Complex I or II, and donates them to Complex III.^[46] This two-electron transfer is governed by the redox reaction:

\text{Q} + 2\text{H}^+ + 2\text{e}^- \rightleftharpoons \text{QH}_2

with a standard reduction potential (E°') of +90 mV at pH 7.^[47] The ubiquinone pool in the inner membrane maintains a high local concentration, approximately 10-fold greater than that of the respiratory complexes, ensuring rapid and efficient electron transfer without significant diffusion limitations during steady-state respiration.^[48] This large pool behaves as a homogeneous reservoir, allowing electrons from multiple dehydrogenases to converge and distribute to downstream acceptors.^[46] In rodents, the isoprenoid tail is typically shorter, with 9 units (CoQ₉), reflecting species-specific variations in biosynthesis that do not substantially alter its ETC function.^[49] Beyond electron shuttling between the Q-binding sites of Complexes I, II, and III, reduced ubiquinol (QH₂) exhibits antioxidant properties by donating electrons to neutralize reactive oxygen species, thereby protecting membrane lipids from peroxidation.^[44] Cytochrome c is a small, water-soluble heme protein that functions as a one-electron carrier in the mitochondrial ETC, diffusing freely within the intermembrane space to shuttle electrons from Complex III to Complex IV.^[50] It has a molecular weight of approximately 12 kDa and contains a covalently bound heme c group, where the iron atom cycles between Fe³⁺ (oxidized, ferricytochrome c) and Fe²⁺ (reduced, ferrocytochrome c) states, with a midpoint redox potential of about +250 mV.^[1] The protein's compact structure, featuring lysine-rich surfaces, facilitates electrostatic interactions with the membrane-associated complexes and anionic phospholipids like cardiolipin, optimizing docking and electron transfer rates.^[50] Maintaining a concentration of around 10 μM in the intermembrane space, cytochrome c ensures kinetic efficiency in electron delivery, supporting maximal respiratory flux under physiological conditions. In pathological contexts, such as apoptosis, cytochrome c is released from the intermembrane space into the cytosol, where it promotes caspase activation and programmed cell death.^[51]

Integration with oxidative phosphorylation

ATP synthase and proton motive force

The ATP synthase, also known as Complex V of the mitochondrial electron transport chain, is a rotary molecular machine embedded in the inner mitochondrial membrane that harnesses the proton motive force (PMF) to synthesize ATP from ADP and inorganic phosphate (Pi).^[52] The PMF, consisting of the electrochemical gradient (Δψ) and pH gradient (ΔpH) across the membrane, provides the energy for this process, with protons flowing back into the matrix through the enzyme driving rotation and catalysis.^[53] Structurally, ATP synthase comprises two main domains: the membrane-embedded F0 portion, which includes a proton-translocating c-ring channel formed by 8–15 c-subunits (8 in mammalian mitochondria), and the peripheral F1 portion in the matrix, featuring a catalytic hexameric head of three α and three β subunits arranged as (αβ)3 around a central γ rotor stalk.^[54]^[52] The mechanism of ATP synthesis, elucidated by Paul Boyer's binding change model and confirmed by structural studies from John Walker, involves proton-driven rotation of the c-ring coupled to conformational changes in the F1 head.^[53] Protons enter the F0 channel via an a-subunit half-channel from the intermembrane space, bind to aspartate or glutamate residues on c-subunits, and drive stepwise rotation of the c-ring (45° per proton in mammalian mitochondria, or 8 protons per full 360° turn).^[54] This rotation turns the γ stalk, which induces sequential conformational shifts in the β-subunits: from open (O, nucleotide release), to loose (L, ADP/Pi binding), to tight (T, ATP formation without energy input), releasing one ATP per 120° rotation and thus three ATP per full turn.^[53] The overall reaction is ADP + Pi + n H⁺_out → ATP + n H⁺_in, where n reflects the proton stoichiometry.^[52] Stoichiometry links PMF utilization to ATP yield: in mammalian mitochondria, a c-ring of 8 subunits translocates 8 protons per full rotation for 3 ATP synthesized at the synthase (mechanistic stoichiometry of ~2.67 H⁺/ATP). Accounting for additional protons required for ADP import and Pi uptake (~1 H⁺ each via translocators), the effective stoichiometry is ~4 H⁺/ATP overall. Combined with ~10 H⁺ pumped per NADH oxidized by the upstream complexes, this results in a P/O ratio of ~2.5 ATP per NADH (or ~1.5 per FADH₂, with 6 H⁺ pumped via Complexes II–IV).^[54] This efficiency ensures that the PMF, generated by electron transport, directly powers oxidative phosphorylation without net ATP hydrolysis under physiological conditions.^[52] Regulation of ATP synthase maintains cellular energy homeostasis and prevents wasteful ATP hydrolysis during low PMF states. The inhibitory factor 1 (IF1) binds to the F1 β-subunits in a pH- and Δp-dependent manner, stabilizing the enzyme in an inactive conformation to block hydrolysis while allowing synthesis when PMF is high.^[55] Oligomycin, a natural antibiotic, specifically inhibits proton translocation through the F0 c-ring by binding the a/c interface, halting both synthesis and hydrolysis.^[55] The enzyme's activity is thus finely tuned to the PMF magnitude, slowing rotation at low gradients.^[56] F-type ATP synthases exhibit remarkable evolutionary conservation across domains of life, with bacterial homologs like that in Escherichia coli (also featuring a 10-c-subunit ring) operating analogously to drive ATP synthesis using PMF from diverse respiratory chains.^[54] This conservation underscores their origin as ancient proton pumps adapted for energy conservation in membranes.^[52]

Reverse electron transport and ROS generation

Reverse electron transport (RET) refers to the backward flow of electrons within the mitochondrial electron transport chain, where reducing equivalents from ubiquinol (QH₂) are transferred to Complex I, reducing NAD⁺ to NADH against the typical redox gradient.^[57] This process is driven by a high proton motive force (Δp), which provides the energy to overcome the endergonic nature of the reaction, particularly when the ubiquinone pool is highly reduced and NAD⁺ levels are elevated.^[57] The key reaction can be represented as:

\ce{QH2 + NAD+ -> Q + NADH + H+}

This thermodynamically unfavorable transfer (negative ΔE) is favored under conditions of high membrane potential and a reduced CoQ/CoQH₂ ratio, such as during succinate accumulation via Complex II.^[58] RET prominently occurs in pathophysiological states like ischemia-reperfusion injury, where succinate buildup from reversed Complex II activity fuels electron donation to the CoQ pool, promoting backward flow to Complex I.^[57] In such scenarios, RET accounts for a substantial portion of reactive oxygen species (ROS) production, with superoxide (O₂⁻) generated primarily at the flavin mononucleotide (FMN) site of Complex I during reverse electron entry.^[58] Additional ROS sites include the FMN site in forward mode and the Q₀ site of Complex III, where semiquinone intermediates leak electrons to molecular oxygen; overall, approximately 1-2% of electrons in the chain divert to O₂ under physiological conditions, escalating during RET.^[58] Physiologically, RET-mediated ROS signaling supports adaptive responses, such as hypoxic sensing in carotid body cells and immune activation in macrophages, where controlled superoxide bursts modulate pathways like HIF-1α stabilization.^[57] However, excessive RET-driven ROS contributes to oxidative damage in pathologies, including ischemia-reperfusion, by peroxidizing lipids and proteins.^[57] Antioxidants like superoxide dismutase (SOD) mitigate this by converting superoxide to hydrogen peroxide, while targeted agents such as mitoQ accumulate in mitochondria to scavenge RET-derived ROS.^[57] Recent studies from the 2020s highlight RET's role in cancer metabolism, particularly in brain cancer stem cells of glioblastoma, where elevated RET at Complex I sustains oxidative phosphorylation, generates ROS for proliferation signaling, and maintains NAD⁺/NADH balance via sirtuin activation, rendering these cells vulnerable to RET inhibitors like CPTP.^[59]

Prokaryotic electron transport chains

Diversity of electron donors and dehydrogenases

In prokaryotic electron transport chains (ETCs), the entry of electrons occurs through a diverse array of dehydrogenases that oxidize various substrates, enabling adaptation to different environmental conditions and energy demands. Unlike the more conserved mitochondrial systems, bacterial ETCs feature modular components that allow flexible assembly of respiratory modules, facilitating efficient energy conservation under aerobic, microaerobic, or anaerobic growth. This modularity supports the integration of multiple electron donors into the quinone pool, enhancing metabolic versatility in diverse bacterial lineages. NADH serves as a primary electron donor in many bacteria, oxidized by two main types of NADH:quinone oxidoreductases. NDH-1, a complex I homolog, is a proton-pumping enzyme that translocates approximately 4 H⁺ per 2 electrons transferred from NADH to quinone, contributing to the proton motive force for ATP synthesis; it is prevalent in species like Escherichia coli. In contrast, NDH-2 is a simpler, non-pumping single-subunit enzyme that transfers electrons from NADH to quinone without generating a proton gradient, often serving as a backup or alternative pathway in organisms such as Bacillus subtilis and Shewanella oneidensis.^[60]^[61]^[62] Beyond NADH, alternative dehydrogenases oxidize a range of organic and inorganic substrates to feed electrons into the ETC. For instance, formate dehydrogenase (FDH) catalyzes the oxidation of formate to CO₂, transferring electrons to quinone, as exemplified by the reaction:

\text{HCOO}^- + \text{Q} \rightarrow \text{CO}_2 + \text{QH}_2

This process is crucial for anaerobic respiration in E. coli and other enteric bacteria, where FDH enables formate utilization as an energy source. Similarly, lactate dehydrogenase and other substrate-specific enzymes provide additional entry points for electrons from fermentation products.^[60] Specialized dehydrogenases further expand substrate diversity, including those for gases like H₂ and CO. Hydrogenases, such as [NiFe]- or [FeFe]-types, oxidize molecular hydrogen (H₂ → 2H⁺ + 2e⁻) and channel electrons into the quinone pool or other carriers, supporting lithoautotrophic growth in hydrogen-oxidizing bacteria like Ralstonia eutropha. Carbon monoxide dehydrogenase (CODH) oxidizes CO to CO₂, integrating this toxic gas as an energy source in carboxydotrophic prokaryotes such as Oligotropha carboxidovorans, thereby mitigating environmental CO toxicity while generating reducing equivalents.^[63]^[64]^[65] In certain marine and pathogenic bacteria, the Na⁺-translocating NADH:quinone reductase (Nqr) couples NADH oxidation to Na⁺ extrusion, pumping 2 Na⁺ per 2 electrons without proton translocation; this is prominent in Vibrio cholerae, where it establishes a sodium motive force for flagellar motility and solute transport under varying oxygen levels. Menaquinol-dependent dehydrogenases, often involved in anaerobic conditions, oxidize substrates using menaquinone as an intermediate, as seen in sulfate-reducing bacteria like Desulfovibrio vulgaris, allowing adaptation to low-potential environments. This diversity of dehydrogenases, through modular assembly, enables bacteria to thrive in microaerobic niches by optimizing electron flow and minimizing reactive oxygen species production.^[66]^[60]

Variations in quinones, cytochromes, and terminal oxidases

In prokaryotic electron transport chains (ETCs), quinones serve as mobile electron carriers that exhibit significant structural and functional variations to accommodate diverse environmental conditions. Ubiquinone (coenzyme Q), predominant in aerobic respiration, possesses a high midpoint redox potential (E°' ≈ +100 mV), facilitating efficient electron transfer to oxygen under oxic conditions. In contrast, menaquinone (vitamin K2) is the primary quinone in anaerobic or microaerobic environments, characterized by a lower redox potential (E°' ≈ -74 to -80 mV), which enables coupling to low-potential electron donors and acceptors such as fumarate or nitrate. Demethylmenaquinone, a structurally related variant, also features a low redox potential (E°' ≈ -36 mV) and participates in anaerobic branches of the ETC, particularly in bacteria like Escherichia coli, where all three quinones coexist and influence pathway branching by directing electrons to specific downstream complexes based on redox poise and oxygen availability. Cytochrome variations further diversify prokaryotic ETCs, with the bc₁ complex (analogous to mitochondrial complex III) oxidizing low-potential quinols like menaquinol and transferring electrons to higher-potential c-type cytochromes, thereby contributing to proton translocation via the Q-cycle mechanism. Alternative pathways bypass cytochrome c, utilizing bd-type quinol oxidases, which directly oxidize ubiquinol or menaquinol without an intervening cytochrome c and exhibit high affinity for oxygen (K_m ≈ 1-10 nM), allowing respiration under low-oxygen conditions. These bd oxidases, found exclusively in prokaryotes, are particularly vital in pathogenic bacteria for survival during oxidative stress or hypoxia. Terminal oxidases represent the most variable downstream components, adapting to oxygen levels, altitude, or alternative acceptors. The aa₃-type oxidase, resembling eukaryotic complex IV, couples quinol or cytochrome c oxidation to oxygen reduction while pumping protons (2 H⁺/2 e⁻).^[67] In contrast, the ba₃-type oxidase, prevalent in high-altitude or microaerophilic species such as Thermus thermophilus, operates with lower proton-pumping efficiency (≈1 H⁺/2 e⁻)^[68] but higher oxygen affinity, suited for low-oxygen niches. For denitrification in anaerobic bacteria like Pseudomonas stutzeri, nitric oxide reductases serve as terminal enzymes, reducing NO to N₂O as part of the respiratory chain, integrating with upstream quinone-dependent branches. A representative reaction for bd-type oxidases illustrates this adaptability: QH₂ + ½ O₂ → Q + H₂O, accompanied by proton translocation of 2 H⁺/2 e⁻ across the membrane via vectorial quinol oxidation, without active pumping.^[69] These variations enable branching in prokaryotic ETCs, as exemplified in E. coli, where cytochrome bo₃ (an aa₃-like quinol oxidase) handles high-oxygen aerobic respiration, while alternative bd oxidases or menaquinone-linked paths activate under low oxygen, optimizing energy yield and survival across redox gradients.

Examples from aerobic and anaerobic bacteria

In aerobic bacteria, Escherichia coli exemplifies a flexible electron transport chain adapted to varying oxygen levels, featuring two NADH dehydrogenases—NDH-1, a proton-pumping complex I homolog, and NDH-2, a non-proton-pumping enzyme—and two terminal quinol oxidases: cytochrome bo₃, which operates under high oxygen conditions with high proton-pumping efficiency, and cytochrome bd, which predominates in microaerobic environments for its lower oxygen affinity.^[70]^[71] This switching mechanism optimizes energy yield while protecting against oxidative stress, with NDH-1 and bo₃ contributing to higher ATP production under normoxia. Similarly, Paracoccus denitrificans possesses a mitochondrial-like respiratory chain, including a canonical complex I (NDH-1), ubiquinone, complex III, cytochrome c, and a terminal aa₃-type oxidase, enabling efficient aerobic respiration with a proton motive force comparable to eukaryotic mitochondria.^[73] This configuration supports high ATP yields through oxidative phosphorylation, and the bacterium's branched chain allows adaptation to alternative electron acceptors like nitrate under oxygen limitation, though aerobic conditions maximize efficiency.^[74] Facultative anaerobes like Bacillus subtilis demonstrate branched electron transport with multiple terminal oxidases for environmental versatility, including the quinol oxidase cytochrome aa₃, which pumps protons efficiently under aerobic conditions, and cyanide-resistant cytochrome bd, which sustains respiration in low-oxygen or toxin-exposed settings.^[75]^[76] The presence of a cytochrome c oxidase branch alongside quinol oxidases allows B. subtilis to balance energy production and stress tolerance, with aa₃ handling bulk oxygen reduction and bd providing a protective, alternative pathway.^[77] In strict anaerobes such as Desulfovibrio species, the electron transport chain couples hydrogen or formate oxidation to sulfate reduction via menaquinone (MK-6), involving transmembrane complexes like Qrc (quinone-reducing complex) and Dsr (dissimilatory sulfite reductase) without oxygen involvement, generating a modest proton motive force for ATP synthesis.^[78] This menaquinone-dependent pathway supports energy conservation in sulfate-rich, anoxic environments, though it yields fewer protons translocated per electron compared to aerobic chains.^[79] Methanogenic archaea, such as those in the genus Methanobacterium, employ a unique anaerobic electron transport system where reduced coenzyme F₄₂₀ (F₄₂₀H₂) donates electrons to heterodisulfide reductase (Hdr), forming a proton-translocating complex that reduces the CoM-S-S-CoB heterodisulfide to thiols during methanogenesis from CO₂ and H₂.^[80] This F₄₂₀H₂:Hdr pathway generates a proton gradient for ATP synthase but operates without quinones or cytochromes typical of bacterial respiration, highlighting archaeal divergence.^[81] Unique adaptations in prokaryotic chains include the role of cytochrome bd oxidases in respiratory protection, where they act as oxygen scavengers to shield nitrogenase or other O₂-sensitive enzymes in microaerophilic or transitioning bacteria, consuming trace oxygen without generating excessive reactive oxygen species.^[82]^[83] Recent metagenomic studies from the 2020s have uncovered uncultured prokaryotic diversity, revealing novel electron transport configurations in environmental microbiomes, such as expanded dehydrogenase variants in sediment communities that expand known respiratory plasticity.^[84] Efficiency varies markedly, with aerobic chains like those in E. coli and P. denitrificans yielding up to 30-38 ATP per glucose equivalent through extensive proton pumping, whereas anaerobic systems in Desulfovibrio and methanogens produce far less—typically 1-5 ATP per reduced substrate—prioritizing biosynthesis and survival in electron acceptor-limited niches over maximal energy harvest.^[85]^[86]

Photosynthetic electron transport chains

Oxygenic photosynthesis in chloroplasts

In oxygenic photosynthesis, the electron transport chain (ETC) in chloroplasts of plants, algae, and cyanobacteria converts light energy into chemical energy by driving non-cyclic electron flow from water to NADP⁺, producing oxygen as a byproduct. This process occurs within the thylakoid membranes and involves two photosystems linked by the cytochrome b₆f complex, forming the Z-scheme. The Z-scheme, first proposed in 1960, illustrates the sequential excitation of electrons at higher redox potentials in photosystem II (PSII) and photosystem I (PSI), enabling efficient energy capture despite the thermodynamic barrier between the two systems. The primary components include PSII, PSI, the mobile carrier plastoquinone (PQ), the cytochrome b₆f complex, and plastocyanin (PC). PSII, centered around the reaction core chlorophyll pair P680, contains the oxygen-evolving complex (OEC) with a Mn₄CaO₅ cluster that catalyzes water oxidation to extract electrons. Electrons from the OEC pass through a pheophytin-quinone (Q_A-Q_B) acceptor complex, where Q_B binds PQ to form plastoquinol (PQH₂). The cytochrome b₆f complex, homologous to complex III in respiration, features b-type hemes, a Rieske iron-sulfur protein, and cytochrome f, facilitating electron transfer from PQH₂ to PC via a Q-cycle mechanism. PSI, with its P700 reaction center chlorophyll pair, includes iron-sulfur (Fe-S) clusters (F_X, F_A, F_B) that relay electrons to soluble ferredoxin (Fd), which reduces NADP⁺ to NADPH via ferredoxin-NADP⁺ reductase.^[87]^[88]^[89] Linear electron flow follows the path: H₂O → PSII (P680) → PQ → cytochrome b₆f → PC → PSI (P700) → Fd → NADP⁺. Light absorption at PSII boosts electrons from P680 to pheophytin, creating P680⁺, which oxidizes the OEC to split water (2H₂O → O₂ + 4H⁺ + 4e⁻). These electrons reduce PQ to PQH₂, which diffuses to cytochrome b₆f. There, the Q-cycle bifurcates electrons: one to PC via the Rieske center and cytochrome f, and the other across the membrane to reduce another PQ molecule, amplifying proton translocation. PC then delivers electrons to P700⁺ in PSI, where light re-energizes them to reduce Fd and ultimately NADP⁺. A parallel cyclic electron flow around PSI returns electrons from Fd to cytochrome b₆f via ferredoxin-dependent pathways, enhancing ATP production without NADPH generation.^[90] Proton pumping builds a proton motive force (ΔpH) across the thylakoid membrane, essential for ATP synthesis. In PSII, water oxidation releases scalar protons (4H⁺ per O₂) into the lumen. The cytochrome b₆f Q-cycle translocates 4H⁺ per 2e⁻ (2 from PQH₂ scalar release in the lumen and 2 vectorial from the stromal to lumen side), contributing the majority of the gradient. This ΔpH, along with a minor membrane potential, drives ATP synthase to produce ATP from ADP and Pᵢ. The overall Z-scheme stoichiometry for linear flow is 2H₂O + 2NADP⁺ + ~8 photons → O₂ + 2NADPH + 2H⁺, balancing NADPH and ATP needs for the Calvin cycle, though cyclic flow adjusts the ATP/NADPH ratio.^[91] Unique to chloroplast thylakoids, the photosynthetic ETC enables dynamic regulation through state transitions and non-photochemical quenching (NPQ). State transitions involve reversible phosphorylation of light-harvesting complex II (LHCII) proteins, mediated by the redox state of PQ; in state 1 (oxidized PQ), LHCII associates with PSII, while in state 2 (reduced PQ), ~15% of LHCII migrates to PSI via actin-dependent mechanisms, balancing excitation between photosystems. NPQ dissipates excess light energy as heat in LHCII antennae, primarily through pH-dependent zeaxanthin formation and PsbS protein activation in PSII, preventing photodamage under high light. These mechanisms optimize electron flow and protect the chain in varying light conditions.^[92]^[93] Recent structural studies using cryo-electron microscopy have advanced understanding of the photosynthetic ETC's assembly and regulation. For instance, a 2024 study achieved a 1.7 Å resolution structure of PSII, revealing intricate water channels involved in substrate delivery to the OEC. In 2022, the PSI–NDH supercomplex was resolved at high resolution, elucidating cyclic electron flow mechanisms. Additionally, 2023 cryo-EM structures of LHCII in photo-active and photo-protecting states demonstrated allosteric regulation of energy dissipation. These findings highlight the dynamic supramolecular organization that optimizes efficiency under fluctuating light conditions.^[94]

Anoxygenic photosynthesis in bacteria

Anoxygenic photosynthesis in bacteria involves electron transport chains that utilize light energy to generate a proton motive force for ATP synthesis without producing oxygen, relying instead on alternative electron donors such as reduced sulfur compounds. These processes occur in diverse prokaryotes, primarily purple bacteria and green sulfur bacteria, each employing distinct reaction centers and carriers. Purple bacteria, such as those in the Rhodospirillaceae family, feature a Type II reaction center with a special pair P870 that absorbs light at approximately 870 nm, initiating electron transfer to a quinone (Q), followed by the bc1 complex, cytochrome c, and terminal oxidases like aa3 under aerobic conditions.^[95] In contrast, green sulfur bacteria utilize a Type I reaction center with P840, where light excitation drives electrons through iron-sulfur (Fe-S) centers to menaquinone, enabling sulfide oxidation without oxygen evolution.^[96] Electron donors in these systems include hydrogen sulfide (H₂S), molecular hydrogen (H₂), and organic compounds, but notably exclude water splitting, which limits the process to anoxic environments. For instance, purple sulfur bacteria like Chromatium oxidize thiosulfate or H₂S to elemental sulfur or sulfate via enzymes such as sulfide:quinone oxidoreductase (SQR), providing electrons to the quinone pool. Green sulfur bacteria similarly employ H₂S as a primary donor, oxidized by SQR to deposit sulfur granules outside the cell. The electron flow typically proceeds from the donor to the reaction center, then through quinones or cytochromes to terminal acceptors, often in a cyclic manner that returns electrons to the center or reduces NAD⁺ for carbon fixation, thereby establishing a proton gradient across the membrane for ATP production.^[97] A representative reaction in green sulfur bacteria is $2\mathrm{H_2S} + 2\mathrm{Q} \rightarrow \mathrm{S_0} + 2\mathrm{QH_2}, where quinone accepts electrons from sulfide oxidation.^[96] Unique structural and functional aspects enhance the efficiency of these chains, including intracytoplasmic membranes in purple bacteria that invaginate from the cytoplasmic membrane to house reaction centers and light-harvesting complexes, optimizing light capture under low-oxygen conditions. These bacteria, exemplified by Rhodobacter capsulatus, demonstrate remarkable versatility, seamlessly switching between photosynthetic electron transport and respiratory modes by sharing components like the bc1 complex and quinones when oxygen becomes available.^[98] This homology between bacterial Type I and II reaction centers and eukaryotic Photosystems I and II underscores their evolutionary conservation, though anoxygenic chains operate with a single photosystem.^[99]

Regulation, inhibitors, and pathology

Mechanisms of regulation

The electron transport chain (ETC) is regulated at multiple levels to fine-tune mitochondrial respiration according to cellular energy demands, preventing excessive reactive oxygen species (ROS) production and maintaining metabolic homeostasis. Allosteric mechanisms provide rapid, reversible control by sensing immediate metabolic states, while post-translational modifications allow dynamic adjustments to environmental cues like oxidative stress. Transcriptional regulation adapts the ETC composition over longer timescales in response to hypoxia or oxygen availability, and structural dynamics of supercomplexes influence electron flux efficiency. In both eukaryotic and prokaryotic systems, these layers integrate with ion signaling to coordinate overall bioenergetics. Allosteric regulation directly modulates ETC complex activities based on energy status. In mammalian mitochondria, cytochrome c oxidase (Complex IV) is inhibited by ATP binding to its matrix domain under high-energy conditions, reducing electron flux and preserving a low membrane potential to minimize ROS generation. This ATP-mediated inhibition is particularly pronounced in the phosphorylated, dimeric form of Complex IV, ensuring respiratory control without complete shutdown. Similarly, Complex I activity is allosterically inhibited by a high NADH/NAD⁺ ratio, which reflects substrate accumulation and prevents over-reduction of the chain, thereby linking upstream metabolic states to downstream electron transfer rates. Post-translational modifications offer precise, covalent control over ETC function, often in response to signaling pathways or stress. Phosphorylation of Complex I subunits by protein kinase A (PKA), activated via cAMP signaling, alters its assembly, catalytic activity, and supercomplex integration, thereby governing oxidative phosphorylation kinetics and oxygen consumption in response to hormonal or adrenergic stimuli. S-glutathionylation, a reversible thiol modification, protects ETC complexes from oxidative damage during ROS elevation; for instance, it targets Complex I and Complex II to attenuate superoxide production by blocking electron leakage, while also feeding back to adjust nutrient uptake and mitochondrial metabolism. These modifications enable the ETC to adapt swiftly to redox imbalances without requiring new protein synthesis. Transcriptional control reshapes the ETC proteome to match environmental conditions, particularly oxygen levels. In hypoxic mammalian cells, hypoxia-inducible factor 1 (HIF-1) suppresses mitochondrial biogenesis and promotes isoform switching in Complex IV, such as upregulating COX4-2 expression while downregulating COX4-1 via LON protease, optimizing respiratory efficiency and reducing oxygen consumption. In bacteria, the ArcA/ArcB two-component system senses quinone redox state to regulate oxidase genes; under low oxygen, phosphorylated ArcA activates transcription of cytochrome bd oxidase (cydAB) for microaerobic respiration while repressing aerobic cytochrome bo oxidase, ensuring adaptive electron transfer to available acceptors. Supercomplex dynamics further regulate ETC efficiency through assembly and disassembly, stabilizing electron channeling. In mitochondria, factors like COX7A2L (SCAF1) promote the association of Complexes I, III, and IV into respirasomes, enhancing proton pumping and reducing ROS by minimizing diffusible intermediate exposure; disruptions in these factors lead to disassembly and inefficient flux. Assembly of Complex IV itself relies on dedicated factors such as SCO1 and SURF1, which coordinate subunit incorporation and supercomplex integration to maintain structural integrity under varying metabolic loads. Calcium signaling provides an additional layer of regulation, particularly in mitochondria, where MICU1 acts as a gatekeeper for the mitochondrial calcium uniporter (MCU). By sensing cytosolic Ca²⁺ levels, MICU1 modulates Ca²⁺ influx to activate dehydrogenases like isocitrate dehydrogenase and α-ketoglutarate dehydrogenase, thereby stimulating ETC substrate supply and NADH production without overload. In bacteria, two-component systems beyond ArcA/B, such as RegB/RegA in photosynthetic species, sense redox or light cues to regulate ETC components, integrating environmental signals with respiratory adaptation. These mechanisms collectively ensure the ETC responds dynamically to physiological needs across organisms.

Inhibitors and experimental tools

Inhibitors of the electron transport chain (ETC) are valuable pharmacological and genetic tools that target specific complexes to dissect their functions, measure electron flux, and model mitochondrial dysfunction in research settings. These agents bind to distinct sites within the complexes, blocking electron transfer or proton translocation, and have been instrumental in elucidating the mechanistic details of oxidative phosphorylation. For instance, partial inhibition of Complex I by certain compounds can mimic physiological stress and inform therapeutic strategies.^[1] For Complex I (NADH:ubiquinone oxidoreductase), rotenone binds to the quinone-binding site (Q-site) in the membrane domain, preventing electron transfer from the iron-sulfur clusters to ubiquinone and halting NADH oxidation. Piericidin A similarly inhibits at the Q-site, competing with ubiquinone for binding and blocking the reduction step.47496-8/fulltext) Rotenone is extensively used in cellular and animal models of Parkinson's disease, where chronic exposure induces selective dopaminergic neuron loss by promoting mitochondrial reactive oxygen species (ROS) production and α-synuclein aggregation. Complex III (cytochrome bc1 complex) inhibitors target the Q-cycle, a bifurcated electron transfer pathway. Antimycin A binds to the Qi site on the distal side, inhibiting electron transfer from heme bH to ubiquinone and causing semiquinone accumulation at the Qo site, which facilitates ROS generation. Myxothiazol, in contrast, binds to the Qo site on the proximal side, blocking electron donation from the Rieske iron-sulfur protein to cytochrome c1 and preventing initial ubiquinol oxidation; this specificity has been crucial for experimentally isolating Q-cycle branches. Complex IV (cytochrome c oxidase) is inhibited by cyanide, which binds tightly to the heme a3 iron in the binuclear center, preventing oxygen binding and reduction to water. Azide targets the CuB site adjacent to heme a3, similarly disrupting the catalytic cycle by competing with oxygen.45888-5/fulltext) Carbon monoxide (CO) serves as a spectroscopic tool, reversibly binding to heme a3 to probe the enzyme's redox state and ligand interactions in low-temperature studies without permanent inactivation. Complex II (succinate:ubiquinone oxidoreductase) is targeted by thenoyltrifluoroacetone (TTFA), which binds to the ubiquinone reduction site in subunit C (Sdha), inhibiting succinate oxidation and flavin-mediated electron transfer to ubiquinone. For ATP synthase (Complex V), oligomycin occludes the FO proton channel, blocking proton flow through the c-ring and preventing ATP synthesis while allowing proton leak in some contexts. Genetic tools complement pharmacological inhibitors for ETC studies. RNA interference (RNAi) knockouts silence nuclear-encoded ETC genes, enabling assessment of complex assembly and compensatory responses in cell lines. Mitochondrial DNA (mtDNA)-deficient rho0 cells, generated by ethidium bromide treatment, lack mtDNA-encoded subunits and serve as models for ETC impairment, as they exhibit reduced respiration and reliance on glycolysis. Flux assays, such as those using the Seahorse XF analyzer, quantify oxygen consumption rate (OCR) to measure ETC activity; inhibitors like rotenone and oligomycin are applied sequentially to isolate contributions from individual complexes via changes in basal, ATP-linked, and maximal respiration. Therapeutically, metformin acts as a partial Complex I inhibitor by binding near the Q-site, modestly reducing NADH oxidation to activate AMP-activated protein kinase (AMPK) and improve insulin sensitivity in type 2 diabetes management. In the 2020s, proteolysis-targeting chimeras (PROTACs) have emerged as tools for targeted degradation of ETC complexes, such as Complex I subunits, by recruiting E3 ligases for ubiquitin-mediated proteolysis, offering spatiotemporal control in research beyond traditional small-molecule inhibition.

Role in diseases and cellular dysfunction

Dysfunction in the electron transport chain (ETC) is a hallmark of various mitochondrial diseases, primarily arising from mutations in nuclear or mitochondrial DNA that impair respiratory complexes. Leigh syndrome, a severe neurometabolic disorder, often results from defects in Complex I (NADH:ubiquinone oxidoreductase) or Complex IV (cytochrome c oxidase), leading to lactic acidosis due to disrupted oxidative phosphorylation and energy failure in high-demand tissues like the brain.^[100] These mutations, accounting for about one-third of childhood-onset cases, cause bilateral symmetric lesions in the basal ganglia and brainstem, manifesting as psychomotor regression, hypotonia, and seizures.^[101] Similarly, Leber's hereditary optic neuropathy (LHON) stems from primary mitochondrial DNA mutations in Complex I genes, such as MT-ND1, MT-ND4, and MT-ND6, resulting in acute or subacute vision loss from optic nerve degeneration.^[102] These point mutations disrupt electron transfer, reducing ATP production and triggering retinal ganglion cell apoptosis.^[103] In neurodegenerative disorders, ETC impairments contribute to selective neuronal vulnerability. Parkinson's disease features a specific Complex I deficiency in the substantia nigra pars compacta, where dopaminergic neurons degenerate, leading to motor symptoms like bradykinesia and rigidity.^[104] This defect, observed in postmortem tissue, reduces NADH oxidation and elevates reactive oxygen species (ROS), exacerbating α-synuclein aggregation and neuronal loss.^[105] In Alzheimer's disease, Complex IV activity declines in affected brain regions, partly due to amyloid-β peptide binding and inhibition of cytochrome c oxidase, which impairs energy metabolism and promotes oxidative stress.^[106] This bioenergetic failure correlates with amyloid plaque formation and cognitive decline, as amyloid-β oligomers further suppress mitochondrial respiration.^[107] Cancer cells exploit ETC alterations to favor proliferation, exemplified by the Warburg effect, where tumors suppress oxidative phosphorylation in favor of aerobic glycolysis, even in oxygen-rich environments, to generate biosynthetic intermediates.^[108] Mutations in succinate dehydrogenase (Complex II), such as in SDHB or SDHD genes, cause succinate accumulation, mimicking hypoxia (pseudohypoxia) by stabilizing HIF-1α and driving angiogenesis and metastasis in paragangliomas and pheochromocytomas.^[109] This oncometabolite inhibits α-ketoglutarate-dependent dioxygenases, leading to epigenetic changes that promote tumorigenesis.^[110] ETC dysfunction also drives ROS-mediated pathologies. In aging, somatic mitochondrial DNA mutations accumulate due to chronic ROS exposure from leaky electron transport, impairing respiratory efficiency and accelerating cellular senescence in post-mitotic tissues.^[111] This vicious cycle of mutagenesis and oxidative damage contributes to frailty and organ decline without necessarily increasing overall ROS levels.^[112] During ischemia-reperfusion injury, such as in stroke or myocardial infarction, reverse electron transport at Complex I generates a burst of ROS upon oxygen restoration, fueled by succinate oxidation, exacerbating tissue damage through lipid peroxidation and inflammation.^[113] Emerging therapies in the 2020s target these defects, including EPI-743, a redox-active quinone analog that bypasses CoQ10 deficiencies in ETC disorders by enhancing NADPH-dependent antioxidant defenses and stabilizing mitochondrial function in Leigh syndrome and related conditions.^[114] Gene editing approaches, such as base editors delivered via adeno-associated viruses, have corrected pathogenic mtDNA mutations in Complex I genes in patient-derived cells, restoring ETC activity and offering potential for treating LHON and Leigh syndrome.^[115] These interventions aim to mitigate lactic acidosis and neurodegeneration by directly repairing heteroplasmic mutations.^[116]

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The mitochondrial coenzyme Q junction and complex ... - FEBS Press
Aug 24, 2021 · The cycle starts at the quinol oxidation site (Qo), where the Fe-S cluster of RISP accepts the first electron from a quinol molecule, ...<|separator|>
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The Q Cycle of Cytochrome bc Complexes: a Structure Perspective
Structure-function problems discussed recently for the bc1 complex include the role of the monomer and dimer in the electron transport pathway associated with ...Iii. The Q Cycle · Quinone Binding In The Dimer... · V. Role Of The Dimer In...Missing: paper | Show results with:paper
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Electronic Connection Between the Quinone and Cytochrome c ...
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Structure of the intact 14-subunit human cytochrome c oxidase
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Biogenesis and Assembly of Eukaryotic Cytochrome c Oxidase ...
The COX catalytic core is formed by three mitochondrial DNA encoded subunits, Cox1, Cox2 and Cox3, conserved in the bacterial enzyme.
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Oxygen Activation and Energy Conservation by Cytochrome c Oxidase
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Proton pumping by cytochrome c oxidase – A 40 year anniversary
Cytochrome c oxidase transduces energy into a proton gradient. The proton pump mechanism involves loading a site, proton transfer, and ejection, creating a ...Missing: O2 | Show results with:O2
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Electron Transfer Pathways in Cytochrome c Oxidase - PMC - NIH
The electron transfer pathway in Cytochrome c Oxidase follows the sequence CuA → heme a → heme a3, with arginines 481 and 482 playing a crucial role.
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Cytochrome c Oxidase at Full Thrust: Regulation and Biological ...
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Coenzyme Q10 | Linus Pauling Institute | Oregon State University
Mitochondrial ATP synthesis As part of the mitochondrial electron transport chain, coenzyme Q10 accepts electrons from reducing equivalents generated during ...
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Ubiquinone - an overview | ScienceDirect Topics
Ubiquinones exist in various chain lengths, with ubiquinone-9 being predominant in rats, while ubiquinone-10 is predominant in humans. 3.3.1 Measurement of ...
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Redox-State Dynamics of Ubiquinone-10 Imply Cooperative ... - NIH
First, for RegB, the standard redox potential of the ... The culture redox potential was calculated for pH 7 from the measured electrode potential.
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Review Mobility and function of Coenzyme Q (ubiquinone) in the ...
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The effect of different ubiquinones on lifespan in Caenorhabditis ...
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The multiple functions of cytochrome c and their regulation in life ...
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Press release: The 1997 Nobel Prize in Chemistry - NobelPrize.org
In 1960 the American scientist Efraim Racker and co-workers isolated, from mitochondria, the enzyme “F o F 1 ATPase” which we now call ATP synthase. The ...
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ATP synthase: From sequence to ring size to the P/O ratio - PMC - NIH
Sep 28, 2010 · The P/O ratio for NADH would be 10/(3.3 + 1) = 10/4.3 ≈ 2.3, thus moving below the range of values directly determined.
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An overview of ATP synthase, inhibitors, and their toxicity - PMC
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Regulation of Mitochondrial Structure and Function by the F1Fo ...
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Role of Mitochondrial Reverse Electron Transport in ROS Signaling
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Mitochondrial electron transport chain, ROS generation and ...
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Regulation of Reverse Electron Transfer at Mitochondrial Complex I ...
Here we show that reverse electron transfer (RET) through respiratory chain complex I (RC-I) is particularly active in brain cancer stem cells (CSC).
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Microbial electron transport and energy conservation
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New Insights into Type II NAD(P)H:Quinone Oxidoreductases - PMC
The main reducing equivalent synthesized by the cell central metabolism is NADH, making it the principal electron donor to respiratory chains. In prokaryotes, ...
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Purification and Characterization of NDH-2 Protein and Elucidating ...
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A Bacterial Electron-bifurcating Hydrogenase - PMC - NIH
Here, we describe an electron-bifurcating hydrogenase that apparently couples the reverse reaction, exergonic downhill flux of two electrons to NAD+ that then ...
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Structural basis for bacterial energy extraction from atmospheric ...
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Carbon Monoxide and Prokaryotic Energy Metabolism - PMC - NIH
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Cryo-EM structures of Na+-pumping NADH-ubiquinone ... - Nature
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Aerobic respiratory chain of Escherichia coli is not allowed ... - PNAS
Oct 18, 2011 · NDH-I and. NDH-II transfer electrons to UQ-8 to yield reduced UQ-8. Three quinol:oxygen oxidoreductases, cytochromes bo3, bd-I, bd-II, oxidize ...<|control11|><|separator|>
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Properties of the two terminal oxidases of Escherichia coli
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effects of mutations in components of the aerobic respiratory chain
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Modifications of the Aerobic Respiratory Chain of Paracoccus ... - NIH
Dec 3, 2019 · Paracoccus denitrificans is a strictly respiring bacterium with a core respiratory chain similar to that of mammalian mitochondria.
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The Paracoccus Denitrificans Electron Transport System
The electron transport system of Paracoccus denitrificans (then known as Micrococcus denitrificans) ... similar to those found in mitochondria. The identification ...
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The terminal quinol oxidases of Bacillus subtilis have ... - PubMed
Cytochrome aa3-600 was found to be the major terminal oxidase in log phase cells. This enzyme was shown to translocate protons across the membrane.Missing: resistant | Show results with:resistant
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Relationship between cardiolipin metabolism and oxygen ...
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New Model for Electron Flow for Sulfate Reduction in Desulfovibrio ...
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Genetics and Molecular Biology of the Electron Flow for ... - Frontiers
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Reduced coenzyme F420: Heterodisulfide oxidoreductase, a - PNAS
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Reduced coenzyme F420: heterodisulfide oxidoreductase, a proton
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The cytochrome bd respiratory oxygen reductases - PMC
Cytochrome bd is a respiratory quinol:O 2 oxidoreductase found in many prokaryotes, including a number of pathogens.
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Cytochrome bd Displays Significant Quinol Peroxidase Activity
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The genetic basis of energy conservation in the sulfate-reducing ...
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Electron Bifurcation and Confurcation in Methanogenesis ... - Frontiers
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Structure of Sr-substituted photosystem II at 2.1 Å resolution ... - PNAS
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Molecular basis of plastoquinone reduction in plant cytochrome b 6 f
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Structure of the far-red light utilizing photosystem I of Acaryochloris ...
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Photosynthetic electron partitioning between [FeFe]-hydrogenase ...
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The proton to electron stoichiometry of steady-state photosynthesis ...
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State transitions in Chlamydomonas reinhardtii strongly modulate ...
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A kinetic model of rapidly reversible nonphotochemical quenching
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Modeling the electron transport chain of purple non-sulfur bacteria
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Anoxygenic photosynthesis with emphasis on green sulfur bacteria ...
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Anoxygenic Photosynthesis in Photolithotrophic Sulfur Bacteria and ...
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Modeling the electron transport chain of purple non‐sulfur bacteria | Molecular Systems Biology
Summary of each segment:
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An overview of anoxygenic phototrophic bacteria and their ...
Anoxygenic phototropic bacteria such as purple bacteria, have a type II (Pheo-Q type) reaction center [52]. In these organisms, when light energy (in photons) ...
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Leigh Syndrome: A Comprehensive Review of the Disease and ...
Leigh syndrome (LS) is a severe neurodegenerative condition with an early onset, typically during early childhood or infancy.
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The genetics of Leigh syndrome and its implications for clinical ...
Deficiency of complex I is the most commonly identified defect in childhood-onset mitochondrial disease and accounts for approximately a third of all cases of ...
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Leber Hereditary Optic Neuropathy (LHON) - StatPearls - NCBI - NIH
These mutations are absent or very rare among normal controls. Except in rare cases of de novo occurrence of a primary LHON mutation, an mtDNA mutation will be ...Continuing Education Activity · Introduction · Etiology · History and Physical
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Respiratory Chain Complex I Deficiency in Leber Hereditary Optic ...
Nov 22, 2024 · Although the mutations in complex I of electric chain may cause ... Leber hereditary optic neuropathy primary mitochondrial DNA mutation.
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Mitochondrial complex I deficiency in Parkinson's disease - PubMed
These results indicated a specific defect of Complex I activity in the substantia nigra of patients with Parkinson's disease.Missing: seminal paper
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Mitochondrial Complex I deficiency: guilty in Parkinson's disease
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Mitochondria, Amyloid β, and Alzheimer's Disease - PMC
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Cytochrome c oxidase deficiency in neurons decreases both ... - PNAS
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The Warburg Effect: How Does it Benefit Cancer Cells? - PMC
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SDH defective cancers: molecular mechanisms and treatment ... - NIH
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Epigenetic and metabolic reprogramming of SDH-deficient ...
Dec 1, 2020 · SDHx mutations lead to the accumulation of succinate, which acts as an oncometabolite by inhibiting iron(II) and alpha-ketoglutarate-dependent ...
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Aging: A mitochondrial DNA perspective, critical analysis and an ...
That is: (1) increased ROS production in aging leads to increased mtDNA mutagenesis; and (2) increased mtDNA mutation loads result in increased mitochondrial ...
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Somatic mtDNA mutations cause aging phenotypes without ... - PNAS
Dec 19, 2005 · The profound aging phenotypes generated by accumulation of somatic mtDNA mutations are thus not mediated by dramatically increased ROS ...
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Reverse Electron Transport at Mitochondrial Complex I in Ischemic ...
Apr 6, 2023 · In this review, we provide a historical account of the roles of ROS ... Mitochondrial electron transport chain, ROS generation and uncoupling.
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Initial experience in the treatment of inherited mitochondrial disease ...
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Scientists use gene editing to correct harmful mitochondrial ...
Jun 24, 2025 · Gene editing technology allows to introduce and correct disease-linked mitochondrial DNA mutations in liver and skin cells.
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Therapies for Mitochondrial Disease: Past, Present, and Future - PMC
Jul 25, 2025 · Emerging therapies include dietary intervention, small molecule therapies aimed to restore mitochondrial function, stem cell or liver ...