Menaquinones have long played a central role in bacterial metabolism due to their solubility in membranes and their ability to mediate electron transfer reactions between a large variety of enzymes. In addition to acting as important nodes in fermentation and respiration, menaquinones are critical to the formation of disulphide bonds in the periplasm. Their utility as molecular wires has also led to their incorporation into redox reactions in higher‐order organisms, where they participate in numerous physiological processes, including blood coagulation. Through studying the menaquinone‐dependent pathways in organisms across the phylogenetic spectrum, researchers have begun to uncover intriguing metabolic links and have identified novel compounds for modulating these vital pathways.
- vitamin K
- vitamin K epoxide reductase
- disulphide bond formation
1. Rise of the quinones
As life began to emerge in the seas of primordial Earth, one of the first orders of business was the construction of a plasma membrane to protect and concentrate biomolecules in the cytoplasm of what would become the first cell. This served to increase the efficiency of the biochemical reactions necessary for growth and propagation. The constant influx of salt water across the plasma membrane, however, would have led to extremely high internal osmotic pressure in what were essentially bags of chemicals, necessitating the invention of efflux pumps to drive ions back out into the surrounding milieu. These early efflux pumps most likely exported protons at the expense of ATP, which the cells were forced to make through substrate‐level phosphorylation, an inefficient process. However, leakage of protons back into the cell could drive the ATPase in the reverse direction, thus linking the extrusion of protons to the creation of cellular energy.
Aside from the issue of osmotic pressure, the plasma membrane also created a conundrum in that the organic molecules necessary to drive metabolism were prevented entry. Thus, cells developed membrane‐associated transporters capable of importing such nutrients. Catabolism of these organic molecules provided the cells with necessary building blocks and resulted in the liberation of electrons, which could then be collected on redox‐active molecules like NAD+ or FAD+, reducing them to NADH and FADH2.
To regenerate the pools of electron carriers, these ancient microbes resorted to fermentation, the process by which electrons are dropped onto self‐derived organic molecules. This freed up NAD+ and FAD+ to participate in more rounds of catabolism of carbon sources, thus driving metabolism. However, fermentation is an inefficient process and thus limited the growth rate and abundance of these microbes. Only when the enzymes involved in fermentation (i.e., nitrate reductase, fumarate reductase) evolved to associate with the plasma membrane did these ancient microbes begin to tap into the power they needed to flourish. Now, the process of passing electrons onto terminal acceptors could be coupled to the extrusion of protons into the extracellular space. With greater numbers of protons pumped out of the cell, their leakage back across the membrane could greatly increase the amount of ATP generated . In essence, the cells could target these molecular machines to the membrane to produce the chemical energy necessary to fuel metabolism. The effect could be further amplified by linking these redox reactions together, but that required cofactors capable of accepting and donating electrons to act as molecular wires. The earliest such cofactors were likely iron‐sulfur clusters and flavins, but these were not readily inserted into the highly lipophilic environment of the plasma membrane. Thus arose the quinones, which are fat‐soluble redox molecules capable of associating with membrane‐embedded enzymes. By linking together several modular redox complexes into an electron transport chain capable of extruding protons, quinones potentiated a huge leap forward in bioenergetics and greatly increased the capacity for complexity in biological systems.
To maximize the utility of having quinones available in their membranes, these ancient microbes needed to find a way to tap into more plentiful electron donors and acceptors. One potential source of electrons present in abundance on primordial Earth was water. However, the vast amounts of energy necessary to pull electrons from water presented a formidable obstacle to its utilization. Only when high‐energy solar radiation came to be employed in the process known as photosynthesis were “cyanobacteria” successful in linking the fixation of CO2 to hydrolysis . Quinones were key to the evolution of photosystem I, yet another example of their power and adaptability in biological systems.
While the increased access to electrons represented a potential windfall to energy‐starved cells, the development of photosynthesis was nonetheless catastrophic to life on Earth. Concomitant with the liberation of electrons from water by photosynthesis was the production of a new and toxic gas–oxygen. Among the many harmful effects of an oxygenated atmosphere were the generation of reactive oxygen species, which poisoned the metabolic pathways of early microbial cells by destroying important cofactors and enzymes . In this noxious environment lay opportunity, however, as oxygen could serve as an extremely effective electron acceptor if cells could evolve mechanisms for reducing it as part of their electron transport chains. Once again quinones mediated a metabolic breakthrough, linking the reduction of oxygen to membrane components via cytochrome oxidases. This process of aerobic respiration led to an estimated 16‐fold increase in the capacity to generate ATP  and may have opened the door to the development of complex eukaryotic life .
The metabolic flexibility of quinones means that their use is not limited simply to the respiratory chains of microbes or the photosynthetic centers of plants. Many higher‐order organisms not only incorporated quinones into their respiratory chains, but have utilized these highly effective molecular wires in many different redox‐dependent reactions. While the quinones are ancient, they remain very important to life on this planet.
2. Biosynthesis of menaquinone and phylloquinone
The major quinones found in nature are ubiquinone (UQ), menaquinone (MK), and phylloquinone (K1) (Figure 1). They differ not only in structure but also in their redox potentials, so the incorporation of one or the other as a cofactor allows for fine‐tuning of electron transfer reactions. The distribution in nature of genes involved in menaquinone biosynthesis suggests that it was most likely the original quinone; this is supported by the observation that menaquinone is readily oxidized in aerobic environments, suggesting that it existed long before the appearance of oxygen . There are many different species of menaquinone, though they differ only in the length of their isoprenyl side chains. These differences are reflected in the nomenclature of menaquinones, wherein the number of isoprene units is indicated (i.e., MK‐4). Phylloquinone, usually considered distinct from the menaquinones, is merely MK‐4 with a more heavily saturated lipophilic tail.
The canonical pathway for menaquinone biosynthesis in bacteria is well‐established and has been reviewed in great detail elsewhere . Of particular interest to this review, however, is the prenylation reaction mediated by MenA in which the lipophilic tail is attached to 1,4‐dihydroxy‐2‐naphthoic acid (Figure 2). In essence, this is the critical step that links the redox‐active quinone to the membrane. The lipophilic substrate of MenA is made up of repeating isoprenal subunits, the exact number of which is determined by the octaprenyl pyrophosphate (OPP) synthase encoded by the particular microbe. The ultimate chain length of these products is determined by a molecular ruler mechanism wherein bulky amino acid residues at the bottom of each of OPP's active sites block chain elongation , and it is this step that controls the identity of the primary MK produced by an organism. There is some evidence to suggest, however, that growth temperature also plays a role in the length and degree of saturation of the aliphatic side chain . Phylloquinone biosynthesis in cyanobacteria is predicted to proceed via a pathway very similar to that of MK biosynthesis. However, the cyanobacterial MenA incorporates a mostly saturated phytyl tail at position C‐3 rather than the partially unsaturated isoprenyl side chain associated with MK . Recently, an alternative pathway for menaquinone biosynthesis has been described in several Achaea and Gram‐negative bacteria, including
Phylloquinone biosynthesis in plants is not as well understood as in cyanobacteria, though the pathway likely mirrors that of menaquinone. One striking difference is that the first four reactions proceeding from chorismate, mediated by the products of the
Unlike the organisms mentioned above, higher‐order organisms are incapable of
Though humans cannot synthesize vitamin K
3. Sources of vitamin K
While the reactions requiring vitamin K in human metabolism are becoming clearer, the source of the vitamin K is still not completely understood. The presence of large numbers of bacteria in the human colon capable of synthesizing K2 would perhaps suggest that absorption of this bacterial byproduct might fulfill the human requirement. In fact, MK‐6 is made by
Low concentrations of vitamin K2 can be found in dairy, meat, and fermented foods like natto , but makes up only 10% of total dietary vitamin K intake. While K1, found in a variety of green leafy plants and vegetable oils, is present in much higher amounts, it is not readily absorbed in the intestines as it is strongly bound to vegetable fiber . Vitamin K is not transported by specific plasma carrier proteins like other fat‐soluble vitamins, but is instead shuttled by lipoproteins. The small fraction of K1 that is absorbed is almost exclusively incorporated into the triacylglycerol‐rich lipoprotein (TGRLP) fraction, while dietary K2 is associated with low‐density lipoprotein (LDL) fraction . These divergent pathways would deliver large amounts of K1 to the liver, but efficient delivery to extrahepatic tissues would only occur for K2. Measurements of the concentrations of vitamins K in various tissues mostly back this up, showing that K1 levels are low in the brain, kidneys, and lungs but high in the liver, heart, and pancreas; K2 (in the form of MK‐4) was found to be in high concentration in the brain, kidneys, and pancreas but in low concentration in the liver, heart, and lungs. As for longer chain K2s, MK6‐11 were found in the liver and trace amounts of MK6‐9 were found in the heart and pancreas . MK10 and MK11 may be major contributors to the hepatic pool of K2 , and the presence of these long‐chain MKs again raise the possibility that the commensal population of colonic bacteria may somehow contribute to overall vitamin K levels in the host, as analysis of tissue samples has only shown the ability to synthesize MK‐4 from K1. However, the presence of potential homologs for other prenyl diphosphate synthases in the genome further suggests that humans may be capable of producing longer chain MKs as well. Overall the data clearly indicate that dietary K1 is a major contributor to vitamin K levels in the body, but a full accounting of its sources has yet to emerge.
4. Uses of vitamin K
While the side chains of K1 and the various MKs differ, the redox‐active portion of the molecules (the napthoquinone) remains unchanged. The reactivity of these various species should therefore be very similar, a fact underlined by the nearly identical mid‐point redox potentials as determined by voltammetry [31, 32] (Figure 3). The degree of lipophilicity in the tails most likely dictates mobility of the quinones in the membrane, with the partially saturated isoprenyl tail of MK allowing for greater freedom of movement compared to the mostly unsaturated chain of K1. Additionally, longer chain MKs are likely stiffer and more viscous in the membrane due to the greater surface areas available for van der Waals interactions. For these reasons, the preferential incorporation of one MK over another into a redox‐active enzyme is most likely due to availability within the membrane as well as the ability of the enzyme to accommodate different length side chains. In microsomal fractions, MK2 and MK3 were shown to have much higher activities than K1 , while a partially purified enzymatic system showed similar activities for MK2‐6 compared to K1. MKs with seven or more isoprenoid units were not as active .
Vitamin K2 has been found to play a role in protection against oxidative stress and inflammation in mammals , and improved locomotion defects in mutant fruit flies , suggesting that it might benefit human patients suffering mitochondrial pathologies. Mounting evidence suggests that MK‐4 is an important component of sphingolipid biosynthesis and can inhibit the proliferation of several cancer cell lines . The exact role of vitamin K2 in these processes is unknown however—its most thoroughly understood use is in protein modification.
Numerous proteins in vertebrates are modified post‐translationally as a means of regulating and enhancing their activity. One such modification is the carboxylation of glutamate residues within Gla domains, which is mediated by the enzyme gamma‐glutamyl carboxylase (GGCX). This modification allows for the high‐affinity binding of calcium ions, which in turn mediates a conformational change necessary for proper folding of the protein. Gla‐containing proteins play important roles in the venom of snakes and the toxins of cone snails , and they have numerous functions in humans including bone development, calcification, and sphingolipid metabolism [35, 39]. The cell‐signaling activities of the vitamin K‐dependent proteins Gas6 and protein S may also be crucial to cognitive processes . Among the Gla‐containing proteins, however, those involved in blood coagulation have received the most attention. Carboxylation of several of these factors activates them and thereby sets off a cascade leading to clotting. The GGCX glycosylation reaction is coupled to the oxidation of vitamin K hydroquinone to vitamin K 2,3‐epoxide, and it is this step that shows sensitivity to anticoagulants like warfarin. When this vitamin K cycle is disrupted or insufficient quantities of vitamin K are present in the diet, excessive bleeding can and does occur, as was the case in the initial discovery of vitamin K's role in nutrition.
While the flexibility of K2s is crucial to all of these redox‐driven processes, short circuits occur wherein reduced menaquinones donate their electrons to “inappropriate” acceptors like oxygen. Such reactions result in the production of reactive oxygen species and can lead to massive damage to proteins and DNA [40, 41], underlining the importance of properly regulating the expression and distribution of MKs.
Clearly, MKs play a critical role in mediating the activity of numerous proteins in mammals, yet the levels of this important cofactor in tissues is relatively low. After passing electrons onto the appropriate acceptors, MK is oxidized to its inactive, oxidized form. In bacteria, MK is quickly reduced again by the flow of electrons from the electron transport chain or to a lesser extent by the delivery of electrons from the disulfide bond pathway. To recharge and replenish their redox‐active pool of MKs, mammals have evolved enzymes capable of reducing of vitamin K 2,3‐epoxide (KO) to vitamin K and vitamin K hydroquinone (KH2). These two steps occur via a warfarin‐sensitive pathway as well as a warfarin‐insensitive pathway, suggesting that two or more enzymes may be required to efficiently complete the reaction. While the enzymatic activity of vitamin K epoxide reductase (VKOR) had first been assayed in 1974 and VKOR had long been known to be the target of the anticoagulant warfarin, identification of the enzyme responsible for the regeneration of vitamin K did not come until 2004 [42, 43]. While this discovery set the stage for in‐depth analysis of the kinetics of blood coagulation, one of the most surprising early findings was that VKOR homologs could be found not only in a large family of vertebrates, but also in insects, plants, bacteria, and archaea . What role could VKOR possibly play in organisms that do not contain blood? The discovery of vitamin K‐dependent proteins in sea squirts  suggests that this modification arose much earlier than the blood coagulation cascade and that vertebrates simply repurposed Gla‐modified proteins.
To fully understand the function of a membrane‐bound protein, it is important to determine the topology of the enzyme within the membrane. This allows for greater insights into the catalytic site as well as to possible interactions with partner proteins. The topology of VKOR in the endoplasmic reticulum (ER) membrane, however, has been fraught with controversy. Initial reports suggested an enzyme with 4 transmembrane domains (TM) , though there is also mounting evidence that VKOR may adopt a 3‐TM structure (Figure 4). Of particular, importance to this debate is the potential positioning of critical cysteine residues. VKOR contains a total of four conserved cysteines, two of which are present in a C‐X‐X‐C motif characteristic of redox‐active thioredoxins. These two cysteines (C132 and C135) have been shown to be essential for the reduction of vitamin KO to vitamin K and vitamin KH2 using purified VKOR . The second set of conserved cysteines (C43 and C51) lie within a loop region between TMs. The 3‐TM model for VKOR places the N‐terminus of the protein and the active site cysteines on the ER side of the membrane, with the loop cysteines and C‐terminus in the cytoplasm. On the other hand, the 4‐TM model places both termini in the cytoplasm, while the active site and loop cysteines both face the ER lumen. This 4‐TM topology would immediately suggest an enzymatic mechanism wherein the loop cysteines receive electrons from interactions with redox partners in the lumen, and then pass them on to the active site C‐X‐X‐C. Because the 3 ‐TM model predicts that the two sets of cysteines are on opposite sides of the ER membrane, it is difficult to imagine how they might interact, and it suggests a distinctly different mechanism for reduction. The fact that several mutations encoding resistance to warfarin map to the loop region containing Cys43 and Cys51 further suggests that these loop cysteines may play a key role in VKOR activity.
The loop cysteines were not required for the enzymatic of activity of VKOR with the purified enzyme, though C51 was found to be important along with C132 and C135 for activity in cell extracts . Expression of Cys 43 and Cys 51 mutants in reporter cells in which endogenous VKOR and VKORL1 were knocked out show that these mutant alleles retain ∼90% activity . However, challenges to such results have emerged. Results with purified VKOR showing the non‐essentiality of the loop cysteines were obtained using dithiothreitol (DTT), a non‐physiological reductant. Because DTT is membrane permeable, it is possible that Cys43 and Cys51 are important for shuttling electrons to the active site cysteines under physiological conditions, but DTT bypasses this necessity. To this end, experiments utilizing the membrane impermeable system of NADPH, thioredoxin, and thioredoxin to drive reduction gave results showing that the loop cysteines were actually required for VKOR activity .
The membrane topology of VKOR has been directly tested through a number of biochemical approaches. The Stafford lab fused green fluorescent protein (gfp) to either the N‐ or C‐terminus and tested protease susceptibility. These studies showed that only the C‐terminus was proteolytically cleaved, which suggested that while the N‐terminus faced the ER lumen, the C‐terminus must face the cytoplasm. This architecture placed the two confirmed active site cysteines (Cys‐132 and Cys‐135) on the luminal side of the membrane, while the two conserved loop cysteines (Cys‐43 and Cys‐51) were on the opposite side . An important caveat to this work is that the protease sensitivity assay was performed after permeabilization with digitonin, a process not thought to affect the topology of membrane proteins. However, a very similar approach using live (i.e., non‐permeabilized) cells and a redox‐active gfp clearly demonstrated that both the N‐ and C‐termini are located within the cytoplasm . Further experiments showed that the loop region containing Cys43 and Cys51 could be glycosylated by machinery within the ER lumen and that the loop cysteines could form mixed disulfides with luminal proteins, thereby placing this loop region firmly in the ER in accordance with a 4‐TM topology.
The overall architecture of VKOR becomes most germane when attempting to identify its redox partners. If VKOR had three membrane‐spanning domains, the loop cysteines would not be accessible to soluble redox partners, yet the active site cysteines would need to be directly accessible to a partner. To achieve this, the partner must also be membrane bound, as has been suggested for GGCX , or must have a hydrophobic domain capable of inserting into the membrane during electron transfer. A potential membrane complex of VKOR and GGCX would explain how a transfer reaction between these two enzymes could be facilitated during blood coagulation, but it does not offer any insights into how electrons might be supplied to VKOR in the first place. Despite the fact that molecular dynamic simulations indicate that the 3‐TM model of human VKOR has a structural advantage in terms of protein stability over a VKOR with 4 TM , questions regarding this model still remain.
In a 4 TM structure of VKOR, the active site cysteines face the ER lumen. It has therefore been hypothesized that VKOR's redox partner must be a luminal protein that most likely bears at least some homology to thioredoxin‐like proteins, which encode cysteines in a C‐X‐X‐C motif. The proposed reaction scheme posits that Cys‐43 of VKOR forms a mixed disulfide with its redox partner, which subsequently attacks Cys‐51 to form an intramolecular disulfide bond in VKOR and releases the redox partner. By mutating the resolving Cys‐51, the mixed disulfide can be trapped, thus allowing identification of the redox partner. Such an approach identified several intriguing candidates including soluble proteins and the membrane‐bound TMX, TMX4, and ERp18 as forming mixed disulfides with VKOR, although it is not clear what the downstream effects of such interactions might be .
Early studies with microsomal fractions indicated that protein disulfide isomerase (PDI) might be an important source of electrons for VKOR , which is consistent with PDI's localization to the ER lumen. PDI can act as an electron acceptor by interacting with proteins containing multiple cysteine residues. By accepting electrons from such proteins, disulfide bonds form between these cysteines, which can serve to stabilize or activate these substrates. Following this reaction, the reduced form of PDI is free to donate its electrons to other partner proteins. Studies confirmed that PDI could stimulate VKOR's reductive activity and went on to suggest that VKOR and PDI may even form a complex in the ER membrane . In other words, the reduction of vitamin KO may be driven by the formation of disulfide bonds in the ER lumen. Such a mechanism appears to contribute to the overall redox homeostasis within the ER  and has also been suggested to operate in plants as well [58, 59].
While VKORs can be found in numerous classes of organisms, paralogs of VKOR are also quite prevalent. Known as “VKORLs” (“VKOR‐like”), the exact role of these enzymes is still unclear. The human VKOR and VKORL1 share 42% identity and 60% similarity. Like VKOR itself, VKORL1 can reduce KO to vitamin K, which may explain why patients treated with anticoagulants do not exhibit significant side effects that would be expected from the inability to turn over vitamin K, like arterial calcifications . Indeed, rat VKORL1 was shown to be up to 50‐fold more resistant to warfarin as compared to VKORC1 in one study , although such a finding has been contested . However, the rate at which VKORL1 reduces KO may be significantly slower than VKOR , and mice missing VKOR (but expressing VKORL1) bled to death shortly after birth , suggesting a different function for VKORL1. It has also been suggested that VKORL1 may play a role in the vitamin K cycle by reducing vitamin K to KH2 , although such a suggestion may be premature, as comparisons of VKOR and VKORL1 activity can be problematic . To gain further insight into the differential functions of VKORL1 versus VKOR, these authors looked at expression levels of the two genes in different tissues. They found clear evidence that VKOR and VKORL1 are differentially regulated in rats and mice, with VKOR showing higher expression in rat liver, lung, and kidney, VKORL1 showing higher expression in the brain, and similar expression profiles in the testis. Overall, the levels of VKORL1 were relatively constant across organs, while VKOR showed extremely high levels in the liver but much lower levels in the remaining tissues . Such findings have led some to hypothesize that VKOR may have evolved to provide cofactor to the vitamin K‐dependent proteins required for maintaining the high‐flux environment of the circulatory system and the homeostasis of a calcified skeleton, while the ability of VKORL1 to reduce vitamin K may be ancillary to its role in antioxidant functions and disulfide bond formation . The differential activity of VKORL1 compared to VKOR is supported by studies conclusively showing that the loop cysteines of VKORL1 are required for activity, in potential contrast to VKOR .
The quest to define a role for bacterial VKORs began with an observation that arose from studies of a well‐defined, quinone‐dependent pathway in bacteria responsible for catalyzing the formation of disulfide bonds in some periplasmic proteins. As covalent bonds between cysteine residues, disulfide bonds can stabilize otherwise energetically unfavorable conformations of certain proteins, thus promoting functionality, similar to binding of calcium ions in the Gla‐dependent proteins of eukaryotes. While most disulfide bonds in the bacterial cytoplasm exist transiently as part of an enzyme catalytic cycle, disulfide bonds in the periplasm are much more stable. This is due to the activity of
Despite the fact that there is little overall homology in the amino acid sequences of human VKOR and
Studies of the functionality of mammalian VKORs in bacteria have been more problematic. Expression of hVKOR in
6. Vitamin K2 as a target for inhibition
MKs are clearly critical components of many aspects of the growth and proliferation of bacterial and human cells, but most of the enzymes necessary for their biosynthesis are only bacterially encoded and are missing from humans. MK biosynthesis would appear to be an ideal target for the development of small molecule inhibitors as potent antibiotics. Among pathogenic bacteria,
As an inhibitor of vitamin K‐dependent reactions, warfarin has long been used as an anticoagulant that at least in part targets human VKOR. While the mycobacterial VKOR has been shown to be sensitive to warfarin, the amount necessary to inhibit the bacterial enzyme is orders of magnitudes higher than the amount needed to prevent blood coagulation . This would suggest that while the human and bacterial VKORs can perform similar functions and do so by similar mechanisms, the divergence in the amino acid sequence of the two is significant enough that treatment of mycobacterial infection with anticoagulants would not be an effective therapeutic strategy. However, ferulenol, an anticoagulant, shown to be approximately 20‐fold more potent against human VKOR than warfarin, showed similar potency against the VKOR from
Disulfide bond formation appears to be dispensable for
The fact that DsbB and
Since their incorporation into the electron transfer pathways of ancient microbes, menaquinones have become a cornerstone of redox‐dependent reactions in almost every domain of life. Their ability to interact with a large variety of proteins, to readily accept and donate electrons, and to easily move within biological membranes have combined to make MKs flexible and efficient molecular wires. As such, organisms have evolved to integrate MKs into many metabolic processes, thus plugging into previously untapped sources of power. While researchers have seemed to only scratch the surface of the myriad uses for MKs to this point, further investigation will yield not only fascinating insights into the biochemical pathways critical to life, but may be a crucial starting point for the development of therapies designed to protect and enhance those pathways.
This work was supported by US National Institute of General Medical Sciences grant GMO41883 (J.B.) and Ruth L. Kirschstein National Research Service Award 1F32GM108443-01 (B.M.M.)
Wilson TH, Lin EC. Evolution of membrane bioenergetics. J Supramol Struct. 1980; 13:421–46.
Falkowski PG. Evolution. Tracing oxygen's imprint on earth's metabolic evolution. Science. 2006;311(5768):1724–5.
Imlay JA. Pathways of oxidative damage. Annu Rev Microbiol. 2003;57:395–418.
Sessions AL, Doughty DM, Welander PV, Summons RE, Newman DK. The continuing puzzle of the great oxidation event. Curr Biol. 2009;19(14):R567–74.
Raymond J, Segrè D. The effect of oxygen on biochemical networks and the evolution of complex life. Science. 2006;311(5768):1764–7.
Hohmann‐Marriott MF, Blankenship RE. Evolution of photosynthesis. Annu Rev Plant Biol. 2011;62:515–48.
Bentley R, Meganathan R. Biosynthesis of vitamin K (menaquinone) in bacteria. Microbiol Rev. 1982;46(3):241–80.
Han X, Chen C‐C, Kuo C‐J, Huang C‐H, Zheng Y, Ko T‐P, et al. Crystal structures of ligand‐bound octaprenyl pyrophosphate synthase from Escherichia colireveal the catalytic and chain‐length determining mechanisms. Proteins. 2015;83(1):37–45.
Nowicka B, Kruk J. Occurrence, biosynthesis and function of isoprenoid quinones. Biochim Biophys Acta. 2010;1797(9):1587–605.
Johnson TW, Shen G, Zybailov B, Kolling D, Reategui R, Beauparlant S, et al. Recruitment of a foreign quinone into the A(1) site of photosystem I. I. Genetic and physiological characterization of phylloquinone biosynthetic pathway mutants in Synechocystissp. pcc 6803. J Biol Chem. 2000;275(12):8523–30.
Hiratsuka T, Furihata K, Ishikawa J, Yamashita H, Itoh N, Seto H, et al. An alternative menaquinone biosynthetic pathway operating in microorganisms. Science. 2008; 321(5896):1670–3.
Gross J, Cho WK, Lezhneva L, Falk J, Krupinska K, Shinozaki K, et al. A plant locus essential for phylloquinone (vitamin K1) biosynthesis originated from a fusion of four eubacterial genes. J Biol Chem. 2006;281(25):17189–96.
Reumann S. Biosynthesis of vitamin K1 (phylloquinone) by plant peroxisomes and its integration into signaling molecule synthesis pathways. Subcell Biochem. 2013;69:213–29.
Nakagawa K, Hirota Y, Sawada N, Yuge N, Watanabe M, Uchino Y, et al. Identification of UBIAD1 as a novel human menaquinone‐4 biosynthetic enzyme. Nature. 2010;468(7320):117–21.
Okano T, Shimomura Y, Yamane M, Suhara Y, Kamao M, Sugiura M, et al. Conversion of phylloquinone (Vitamin K1) into menaquinone‐4 (Vitamin K2) in mice: two possible routes for menaquinone‐4 accumulation in cerebra of mice. J Biol Chem. 2008;283(17):11270–9.
Hirota Y, Tsugawa N, Nakagawa K, Suhara Y, Tanaka K, Uchino Y, et al. Menadione (vitamin K3) is a catabolic product of oral phylloquinone (vitamin K1) in the intestine and a circulating precursor of tissue menaquinone‐4 (vitamin K2) in rats. J Biol Chem. 2013;288(46):33071–80.
Davidson RT, Foley AL, Engelke JA, Suttie JW. Conversion of dietary phylloquinone to tissue menaquinone‐4 in rats is not dependent on gut bacteria. J Nutr. 1998;128(2):220–3.
Nakagawa K, Sawada N, Hirota Y, Uchino Y, Suhara Y, Hasegawa T, et al. Vitamin K2 biosynthetic enzyme, UBIAD1 is essential for embryonic development of mice. Plos One. 2014;9(8):e104078.
Fernandez F, Collins MD. Vitamin K composition of anaerobic gut bacteria. FEMS Microbiol Lett. 1987;41:175–80.
Shearer MJ, Newman P. Recent trends in the metabolism and cell biology of vitamin K with special reference to vitamin K cycling and MK‐4 biosynthesis. J Lipid Res. 2014;55(3):345–62.
Coates ME. Gnotobiotic animals in nutrition research. Proc Nutr Soc. 1973;32(2):53–8.
Conly J, Stein K. Reduction of vitamin K2 concentrations in human liver associated with the use of broad spectrum antimicrobials. Clin Investig Med. 1994;6:531–9.
Newman DK, Kolter R. A role for excreted quinones in extracellular electron transfer. Nature. 2000;405(6782):94–7.
Groenen‐van Dooren MM, Ronden JE, Soute BA, Vermeer C. Bioavailability of phylloquinone and menaquinones after oral and colorectal administration in vitamin K‐deficient rats. Biochem Pharmacol. 1995;50(6):797–801.
Beulens JWJ, Booth SL, van den Heuvel EGHM, Stoecklin E, Baka A, Vermeer C. The role of menaquinones (vitamin K2) in human health. Br J Nutr. 2013;110(8):1357–68.
Suttie JW. The importance of menaquinones in human nutrition. Annu Rev Nutr. 1995;15:399–417.
Walther B, Karl JP, Booth SL, Boyaval P. Menaquinones, bacteria, and the food supply: the relevance of dairy and fermented food products to vitamin K requirements. Adv Nutr. 2013;4(4):463–73.
Gijsbers BL, Jie KS, Vermeer C. Effect of food composition on vitamin K absorption in human volunteers. Br J Nutr. 1996;76(2):223–9.
Schurgers LJ, Vermeer C. Differential lipoprotein transport pathways of K‐vitamins in healthy subjects. Biochim Biophys Acta. 2002;1570(1):27–32.
Kurosu M, Begari E. Vitamin K2 in electron transport system: are enzymes involved in vitamin K2 biosynthesis promising drug targets? Molecules. 2010;15(3):1531–53.
Schoepp‐Cothenet B, Lieutaud C, Baymann F, Verméglio A, Friedrich T, Kramer DM, et al. Menaquinone as pool quinone in a purple bacterium. Proc Natl Acad Sci USA. 2009;106(21):8549–54.
Wagner GC, Kassner RJ, Kamen MD. Redox potentials of certain vitamins K: implications for a role in sulfite reduction by obligately anaerobic bacteria. PNAS. 1974;71(2):253–6.
Friedman PA, Shia M. Some characteristics of a vitamin K‐dependent carboxylating system from rat liver microsomes. Biochem Biophys Res Commun. 1976;70(2):647–54.
Buitenhuis HC, Soute BA, Vermeer C. Comparison of the vitamins K1, K2 and K3 as cofactors for the hepatic vitamin K‐dependent carboxylase. Biochim Biophys Acta. 1990;1034(2):170–5.
Ferland G. Vitamin K, an emerging nutrient in brain function. Biofactors. 2012;38(2):151–7.
Vos M, Esposito G, Edirisinghe JN, Vilain S, Haddad DM, Slabbaert JR, et al. Vitamin K2 is a mitochondrial electron carrier that rescues pink1 deficiency. Science. 2012;336(6086):1306–10.
Shearer MJ, Newman P. Metabolism and cell biology of vitamin K. Thromb Haemost. 2008;100(4):530–47.
Czerwiec E, Begley GS, Bronstein M, Stenflo J, Taylor K, Furie BC, et al. Expression and characterization of recombinant vitamin K‐dependent gamma‐glutamyl carboxylase from an invertebrate, Conus textile. Eur J Biochem. 2002;269(24):6162–72.
Oldenburg J, Watzka M, Bevans CG. VKORC1 and VKORC1L1: why do vertebrates have two vitamin K 2,3‐epoxide reductases? Nutrients. 2015;7(8):6250–80.
Wakeman CA, Hammer ND, Stauff DL, Attia AS, Anzaldi LL, Dikalov SI, et al. Menaquinone biosynthesis potentiates haem toxicity in Staphylococcus aureus. Mol Microbiol. 2012;86(6):1376–92.
Korshunov S, Imlay JA. Detection and quantification of superoxide formed within the periplasm of Escherichia coli. J Bacteriol. 2006;188(17):6326–34.
Li T, Chang C‐Y, Jin D‐Y, Lin P‐J, Khvorova A, Stafford DW. Identification of the gene for vitamin K epoxide reductase. Nature. 2004;427(6974):541–4.
Rost S, Fregin A, Ivaskevicius V, Conzelmann E, Hörtnagel K, Pelz H‐J, et al. Mutations in VKORC1 cause warfarin resistance and multiple coagulation factor deficiency type 2. Nature. 2004;427(6974):537–41.
Goodstadt L, Ponting CP. Vitamin K epoxide reductase: homology, active site and catalytic mechanism. Trends Biochem Sci. 2004;29(6):289–92.
Kulman JD, Harris JE, Nakazawa N, Ogasawara M, Satake M, Davie EW. Vitamin K‐dependent proteins in Ciona intestinalis, a basal chordate lacking a blood coagulation cascade. Proc Natl Acad Sci USA. 2006;103(43):15794–9.
Jin D‐Y, Tie J‐K, Stafford DW. The conversion of vitamin K epoxide to vitamin K quinone and vitamin K quinone to vitamin K hydroquinone uses the same active site cysteines. Biochemistry. 2007;46(24):7279–83.
Rost S, Fregin A, Hünerberg M, Bevans CG, Müller CR, Oldenburg J. Site‐directed mutagenesis of coumarin‐type anticoagulant‐sensitive VKORC1: evidence that highly conserved amino acids define structural requirements for enzymatic activity and inhibition by warfarin. Thromb Haemost. 2005;94(4):780–6.
Tie J‐K, Jin D‐Y, Tie K, Stafford DW. Evaluation of warfarin resistance using transcription activator‐like effector nucleases‐mediated vitamin K epoxide reductase knockout HEK293 cells. J Thromb Haemost. 2013;11(8):1556–64.
Rishavy MA, Usubalieva A, Hallgren KW, Berkner KL. Novel insight into the mechanism of the vitamin K oxidoreductase (VKOR): electron relay through Cys43 and Cys51 reduces VKOR to allow vitamin K reduction and facilitation of vitamin K‐dependent protein carboxylation. J Biol Chem. 2011;286(9):7267–78.
Tie J‐K, Jin D‐Y, Stafford DW. Human vitamin K epoxide reductase and its bacterial homologue have different membrane topologies and reaction mechanisms. J Biol Chem. 2012;287(41):33945–55.
Cao Z, van Lith M, Mitchell LJ, Pringle MA, Inaba K, Bulleid NJ. The membrane topology of vitamin K epoxide reductase is conserved between Human isoforms and the bacterial enzyme. Biochem J. 2016;:BJ20151223.
Wu S, Liu S, Davis CH, Stafford DW, Kulman JD, Pedersen LG. A hetero‐dimer model for concerted action of vitamin K carboxylase and vitamin K reductase in vitamin K cycle. J Theor Biol. 2011;279(1):143–9.
Wu S, Tie J‐K, Stafford DW, Pedersen LG. Membrane topology for human vitamin K epoxide reductase. J Thromb Haemost. 2014;12(1):112–4.
Schulman S, Wang B, Li W, Rapoport TA. Vitamin K epoxide reductase prefers ER membrane‐anchored thioredoxin‐like redox partners. Proc Natl Acad Sci USA. 2010;107(34):15027–32.
Soute BA, Groenen‐van Dooren MM, Holmgren A, Lundström J, Vermeer C. Stimulation of the dithiol‐dependent reductases in the vitamin K cycle by the thioredoxin system. Strong synergistic effects with protein disulphide‐isomerase. Biochem J. 1992;281 (Pt 1):255–9.
Wajih N, Hutson SM, Wallin R. Disulfide‐dependent protein folding is linked to operation of the vitamin K cycle in the endoplasmic reticulum. A protein disulfide isomerase‐VKORC1 redox enzyme complex appears to be responsible for vitamin K1 2,3‐epoxide reduction. J Biol Chem. 2007;282(4):2626–35.
Rutkevich LA, Williams DB. Vitamin K epoxide reductase contributes to protein disulfide formation and redox homeostasis within the endoplasmic reticulum. Mol Biol Cell. 2012;23(11):2017–27.
Feng W‐K, Wang L, Lu Y, Wang X‐Y. A protein oxidase catalysing disulfide bond formation is localized to the chloroplast thylakoids. FEBS J. 2011;278(18):3419–30.
Wan C‐M, Yang X‐J, Du J‐J, Lu Y, Yu Z‐B, Feng Y‐G, et al. Identification and characterization of SlVKOR, a disulfide bond formation protein from Solanum lycopersicum, and bioinformatic analysis of plant VKORs. Biochem Mosc. 2014;79(5):440–9.
Westhofen P, Watzka M, Marinova M, Hass M, Kirfel G, Müller J, et al. Human vitamin K 2,3‐epoxide reductase complex subunit 1‐like 1 (VKORC1L1) mediates vitamin K‐dependent intracellular antioxidant function. J Biol Chem. 2011;286(17):15085–94.
Hammed A, Matagrin B, Spohn G, Prouillac C, Benoit E, Lattard V. VKORC1L1, an enzyme rescuing the vitamin K 2,3‐epoxide reductase activity in some extrahepatic tissues during anticoagulation therapy. J Biol Chem. 2013;288(40):28733–42.
Tie J‐K, Jin D‐Y, Stafford DW. Conserved loop cysteines of vitamin K epoxide reductase complex subunit 1‐like 1 (VKORC1L1) are involved in its active site regeneration. J Biol Chem. 2014;289(13):9396–407.
Spohn G, Kleinridders A, Wunderlich FT, Watzka M, Zaucke F, Blumbach K, et al. VKORC1 deficiency in mice causes early postnatal lethality due to severe bleeding. Thromb Haemost. 2009;101(6):1044–50.
Van Horn WD. Structural and functional insights into human vitamin K epoxide reductase and vitamin K epoxide reductase‐like1. Crit Rev Biochem Mol Biol. 2013;48(4):357–72.
Bardwell JC, McGovern K, Beckwith J. Identification of a protein required for disulfide bond formation in vivo. Cell. 1991;67(3):581–9.
Kadokura H, Katzen F, Beckwith J. Protein disulfide bond formation in prokaryotes. Annu Rev Biochem. 2003;72:111–35.
Bardwell JC, Lee JO, Jander G, Martin N, Belin D, Beckwith J. A pathway for disulfide bond formation in vivo. Proc Natl Acad Sci USA. 1993;90(3):1038–42.
Missiakas D, Georgopoulos C, Raina S. Identification and characterization of the Escherichia coli gene dsbB, whose product is involved in the formation of disulfide bonds in vivo. Proc Natl Acad Sci USA. 1993;90(15):7084–8.
Kadokura H, Beckwith J. Four cysteines of the membrane protein DsbB act in concert to oxidize its substrate DsbA. EMBO J. 2002;21(10):2354–63.
Bader MW, Xie T, Yu CA, Bardwell JC. Disulfide bonds are generated by quinone reduction. J Biol Chem. 2000;275(34):26082–8.
Takahashi Y‐H, Inaba K, Ito K. Characterization of the menaquinone‐dependent disulfide bond formation pathway of Escherichia coli. J Biol Chem. 2004;279(45):47057–65.
Dutton RJ, Boyd D, Berkmen M, Beckwith J. Bacterial species exhibit diversity in their mechanisms and capacity for protein disulfide bond formation. Proc Natl Acad Sci USA. 2008;105(33):11933–8.
Singh AK, Bhattacharyya‐Pakrasi M, Pakrasi HB. Identification of an atypical membrane protein involved in the formation of protein disulfide bonds in oxygenic photosynthetic organisms. J Biol Chem. 2008;283(23):15762–70.
Dutton RJ, Wayman A, Wei J‐R, Rubin EJ, Beckwith J, Boyd D. Inhibition of bacterial disulfide bond formation by the anticoagulant warfarin. Proc Natl Acad Sci USA. 2010;107(1):297–301.
Li W, Schulman S, Dutton RJ, Boyd D, Beckwith J, Rapoport TA. Structure of a bacterial homologue of vitamin K epoxide reductase. Nature. 2010;463(7280):507–12.
Liu S, Cheng W, Fowle Grider R, Shen G, Li W. Structures of an intramembrane vitamin K epoxide reductase homolog reveal control mechanisms for electron transfer. Nat Commun. 2014;5:3110.
Wang X, Dutton RJ, Beckwith J, Boyd D. Membrane topology and mutational analysis of Mycobacterium tuberculosisVKOR, a protein involved in disulfide bond formation and a homologue of human vitamin K epoxide reductase. Antioxid Redox Signal. 2011;14(8):1413–20.
Bevans CG, Krettler C, Reinhart C, Watzka M, Oldenburg J. Phylogeny of the vitamin K 2,3‐epoxide reductase (VKOR) family and evolutionary relationship to the disulfide bond formation protein B (DsbB) family. Nutrients. 2015;7(8):6224–49.
Tie J‐K, Jin D‐Y, Stafford DW. Mycobacterium tuberculosisvitamin K epoxide reductase homologue supports vitamin K‐dependent carboxylation in mammalian cells. Antioxid Redox Signal. 2012;16(4):329–38.
Jaenecke F, Friedrich‐Epler B, Parthier C, Stubbs MT. Membrane composition influences the activity of in vitro refolded human vitamin K epoxide reductase. Biochemistry. 2015;54(42):6454–61.
Hatahet F, Blazyk JL, Martineau E, Mandela E, Zhao Y, Campbell RE, et al. Altered Escherichia colimembrane protein assembly machinery allows proper membrane assembly of eukaryotic protein vitamin K epoxide reductase. Proc Natl Acad Sci USA. 2015;112(49):15184–9.
Heijne G. The distribution of positively charged residues in bacterial inner membrane proteins correlates with the trans‐membrane topology. EMBO J. 1986;5(11):3021–7.
Boyd D, Beckwith J. Positively charged amino acid residues can act as topogenic determinants in membrane proteins. PNAS. 1989;86(23):9446–50.
Dhiman RK, Mahapatra S, Slayden RA, Boyne ME, Lenaerts A, Hinshaw JC, et al. Menaquinone synthesis is critical for maintaining mycobacterial viability during exponential growth and recovery from non‐replicating persistence. Mol Microbiol. 2009;72(1):85–97.
Lu X, Zhang H, Tonge PJ, Tan DS. Mechanism‐based inhibitors of MenE, an acyl‐CoA synthetase involved in bacterial menaquinone biosynthesis. Bioorg Med Chem Lett. 2008;18(22):5963–6.
Kurosu M, Narayanasamy P, Biswas K, Dhiman R, Crick DC. Discovery of 1,4‐dihydroxy‐2‐naphthoate [corrected] prenyltransferase inhibitors: new drug leads for multidrug‐resistant gram‐positive pathogens. J Med Chem. 2007;50(17):3973–5.
Debnath J, Siricilla S, Wan B, Crick DC, Lenaerts AJ, Franzblau SG, et al. Discovery of selective menaquinone biosynthesis inhibitors against Mycobacterium tuberculosis. J Med Chem. 2012;55(8):3739–55.
Sassetti CM, Boyd DH, Rubin EJ. Genes required for mycobacterial growth defined by high density mutagenesis. Mol Microbiol. 2003;48(1):77–84.
Landeta C, Blazyk JL, Hatahet F, Meehan BM, Eser M, Myrick A, et al. Compounds targeting disulfide bond forming enzyme DsbB of Gram‐negative bacteria. Nat Chem Biol. 2015;11(4):292.