- Protein family review
- Open Access
Cytochromes P450: a success story
Genome Biologyvolume 1, Article number: reviews3003.1 (2000)
Cytochrome P450 proteins, named for the absorption band at 450 nm of their carbon-monoxide-bound form, are one of the largest superfamilies of enzyme proteins. The P450 genes (also called CYP) are found in the genomes of virtually all organisms, but their number has exploded in plants. Their amino-acid sequences are extremely diverse, with levels of identity as low as 16% in some cases, but their structural fold has remained the same throughout evolution. P450s are heme-thiolate proteins; their most conserved structural features are related to heme binding and common catalytic properties, the major feature being a completely conserved cysteine serving as fifth (axial) ligand to the heme iron. Canonical P450s use electrons from NAD(P)H to catalyze activation of molecular oxygen, leading to regiospecific and stereospecific oxidative attack of a plethora of substrates. The reactions carried out by P450s, though often hydroxylation, can be extremely diverse and sometimes surprising. They contribute to vital processes such as carbon source assimilation, biosynthesis of hormones and of structural components of living organisms, and also carcinogenesis and degradation of xenobiotics. In plants, chemical defense seems to be a major reason for P450 diversification. In prokaryotes, P450s are soluble proteins. In eukaryotes, they are usually bound to the endoplasmic reticulum or inner mitochondrial membranes. The electron carrier proteins used for conveying reducing equivalents from NAD(P)H differ with subcellular localization. P450 enzymes catalyze many reactions that are important in drug metabolism or that have practical applications in industry; their economic impact is therefore considerable.
Gene organization and evolutionary history
P450 superfamily genes are subdivided and classified following recommendations of a nomenclature committee [1,2] on the basis of amino-acid identity, phylogenetic criteria and gene organization. The root symbol CYP is followed by a number for families (generally groups of proteins with more than 40% amino-acid sequence identity, of which there are over 200), a letter for subfamilies (greater than 55% identity) and a number for the gene; for example, CYP4U2. There are also designations for clades of CYP families (clans, which can be defined as groups of genes that clearly diverged from a single common ancestor; clans are named from the lowest family number in the clade)  and for specific alleles of a gene (in humans) [4,5]. The diversity of the cytochrome P450 superfamily arose by an extensive process of gene duplications and by probable, but less well documented, cases of gene amplifications, conversions, genome duplications, gene loss and lateral transfers. 'Fossil' evidence of these processes can be found by careful sequence alignments as well as from the presence of many P450 gene clusters in most organisms. These gene clusters can contain up to 15 P450 genes, the orientation and sequence similarity of which sometimes allows a reconstruction of the events leading to the formation of the cluster. For instance in maize, four clustered CYP71C genes are involved in a common biosynthetic pathway for the defense compound 2,4-dihydroxy-1,4-benzoxazin-3-one (DIBOA) , but in most cases there is no evidence for a functional link between members of a cluster of P450 genes.
The origin of the P450 superfamily lies in prokaryotes, before the advent of eukaryotes and before the accumulation of molecular oxygen in the atmosphere. Although Escherichia coli has no P450 gene, Mycobacterium tuberculosis has 20 , baker's yeast has three, and the fruit fly Drosophila melanogaster has 83 P450 genes  and seven pseudogenes. The fly situation seems the norm in 'higher' animals, with about 80 P450 genes in the nematode Caenorhabditis elegans and about 55 genes and 25 pseudogenes in humans. Higher plants have many more P450 genes, with about 286 in Arabidopsis thaliana . The plant P450s are polyphyletic, with one large clade, the A-type P450s, representing plant-specific enzymes involved mostly in the biosynthesis of natural products, and several other P450s (the non-A-type) being phylogenetically related to P450s from other phyla, often with some conservation of function (fatty acid or sterol metabolism). Only one P450 gene family, CYP51, is conserved across phyla, from plants to fungi and animals, and a CYP51 ortholog has also been found in the bacterium M. tuberculosis, possibly as a result of lateral gene transfer from its host. CYP51 genes encode the 14 a-demethylases of sterols that streamline the a face of sterols . In mammals, CYP51 is also involved in the synthesis of meiosis-activating sterols in oocytes and testis. The complex catalytic function of CYP51 (sequential hydroxylations followed by carbon-carbon bond cleavage) is a highly specialized, and thus derived, trait that evolved early in the eukaryotic lineage. It was lost in insects and nematodes, which are sterol heterotrophs. Various cladograms illustrating the concept of clans or several specific aspects of P450 evolution can be found in [2,6,9,10,11,12].
The exon-intron organization of P450 genes reveals a remarkable diversity of gene structure, and few, if any, intron positions are conserved between divergent P450 families [9,10,11,13]. Thus, the evolutionary history of P450 genes is one of multiple intron gain and loss.
Characteristic structural features
P450s can be divided into four classes depending on how electrons from NAD(P)H are delivered to the catalytic site. Class I proteins require both an FAD-containing reductase and an iron sulfur redoxin. Class II proteins require only an FAD/FMN-containing P450 reductase for transfer of electrons. Class III enzymes are self-sufficient and require no electron donor, while P450s from class IV receive electrons directly from NAD(P)H. This classification of the interactions with redox partners is unrelated to P450 evolutionary history.
Sequence identity among P450 proteins is often extremely low and may be less than 20%, and there are only three absolutely conserved amino acids. The determination of an increasing number of P450 crystal structures, however, shows that this unusual variability does not preclude a high conservation of their general topography and structural fold . Highest structural conservation is found in the core of the protein around the heme and reflects a common mechanism of electron and proton transfer and oxygen activation. The conserved core is formed of a four-helix (D, E, I and L) bundle, helices J and K, two sets of ß sheets, and a coil called the 'meander'. These regions comprise (Figures 1,2a): first, the heme-binding loop, containing the most characteristic P450 consensus sequence (Phe-X-X-Gly-X-Arg-X-Cys-X-Gly), located on the proximal face of the heme just before the L helix, with the absolutely conserved cysteine that serves as fifth ligand to the heme iron; second, the absolutely conserved Glu-X-X-Arg motif in helix K, also on the proximal side of heme and probably needed to stabilize the core structure; and finally, the central part of the I helix, containing another consensus sequence considered as P450 signature (Ala/Gly-Gly-X-Asp/Glu-Thr-Thr/Ser), which corresponds to the proton transfer groove on the distal side of the heme.
The most variable regions are associated with either amino-terminal anchoring or targeting of membrane-bound proteins, or substrate binding and recognition; the latter regions are located near the substrate-access channel and catalytic site and are often referred to as substrate-recognition sites or SRSs . They are described as flexible, moving upon binding of substrate so as to favor the catalytic reaction. Other variations reflect differences in electron donors, reaction catalyzed or membrane localization (Figure 1b). Most eukaryotic P450s are associated with microsomal membranes, and very frequently have a cluster of prolines (Pro-Pro-X-Pro) that form a hinge, preceded by a cluster of basic residues (the halt-transfer signal) between the hydrophobic amino-terminal membrane anchoring segment and the globular part of the protein (Figure 1a). Additional membrane interaction seems to be mediated essentially by a region, located between the F and G helices, that shows increased hydrophobicity . A signature for mitochondrial enzymes is, in addition to an amino-terminal cleavable signal peptide, the presence of two positive charges, usually arginines, at the beginning of the L helix. Such positive charges are also found in soluble bacterial P450s of class I, which receive their electrons from a ferredoxin. Strong variation from consensus in the core region, particularly an I helix lacking the characteristic threonine and surrounding residues, is characteristic of enzymes of class III catalyzing the rearrangement of hydroperoxides. These P450s do not require molecular oxygen nor electron donor for catalysis, which explains their unusual deviation from the canonical primary structure.
No class III P450 has been crystallized to date. The crystal structures of model proteins belonging to the three other classes are, however, available [17,18], including the substrate, oxygen and CO-bound, and activated reaction-intermediate forms of some enzymes (for example class I: P450cam or CYP101 [19,20]; class II: P450BM3 or CYP102 [16,21,22]; class IV: P450nor or CYP55A1 ). Prototype secondary and three-dimensional structures are shown in Figure 2.
Localization and function
P450s in prokaryotes are soluble proteins. Class I P450s require both an FAD-containing NAD(P)H-reductase and an iron-sulfur redoxin as electron donors. Prokaryotic class II require only an FAD/FMN-containing NADPH-P450 reductase, which is fused to the P450 protein. P450s often confer on prokaryotes the ability to catabolize compounds used as carbon source or to detoxify xenobiotics. Other functions described for prokaryotic P450s include fatty acid metabolism and biosynthesis of antibiotics.
Eukaryotic class I enzymes are found associated with the inner membrane of mitochondria and catalyze several steps in the biosynthesis of steroid hormones and vitamin D3 in mammals. Mitochondrial P450s are also found in insects and nematodes, but so far none has been described in plants. Animal mitochondrial P450s appear to have evolved by mistargeting of an animal microsomal P450, and they are not phylogenetically related to the class I P450s of bacteria despite their analogous electron transport chain. Class II enzymes are the most common in eukaryotes. P450s and NADPH-P450 reductases are dissociated and independently anchored on the outer face of the endoplasmic reticulum (ER) by amino-terminal hydrophobic anchors. An additional carboxy-terminally ER-anchored electron donor, cytochrome b5 which conveys electrons from NAD(P)H, has been found to enhance the activity of some P450 enzymes. Functions of enzymes of class II are extremely diverse. In fungi, they include synthesis of membrane sterols and mycotoxins, detoxification of phytoalexins, and metabolism of lipid carbon sources. In animals, physiological functions include many aspects of the biosynthesis and catabolism of signalling molecules, steroid hormones, retinoic acid and oxylipins [2,24,25]. Class II P450s from plants are involved in biosynthesis or catabolism of all types of hormones, in the oxygenation of fatty acids for the synthesis of cutins, and in all of the pathways of secondary metabolism - in lignification and the synthesis of flower pigments and defense chemicals (which are also aromas, flavors, antioxidants, phyto-estrogens, anti-cancer drugs and other drugs) [12,26]. Class I and class II P450s from all organisms participate in the detoxification or sometimes the activation of xenobiotics. They have been shown to contribute to carcinogenesis, and are essential determinants of drug and pesticide metabolism, tolerance, selectivity and compatibility [24,25,27,28]. P450s that actively metabolize xenobiotics often have their expression induced by exogenous chemicals [25,28,29,30]. Their pharmacologic and agronomic impact is thus considerable.
P450s from class III are self-sufficient and do not require molecular oxygen or an external electron source. They catalyze the rearrangement or dehydration of alkylhydroperoxides or alkylperoxides initially generated by dioxygenases . These enzymes are involved in the synthesis of signaling molecules such as prostaglandins in mammals and jasmonate in plants; they seem to have diverse subcellular localizations in plants, including plastidial. A P450 that receives its electrons directly from NADH has also been described that belongs to class IV. This unique fungal P450 is soluble and reduces NO generated by denitrification to N20 . The latter two classes might be considered as remains of the most ancestral forms of P450 involved in detoxification of harmful activated oxygen species.
There is no rule for the tissue distribution of P450 enzymes. As their functions are extremely diverse, they can be found in all types of tissues, with developmentally regulated patterns of expression, in all types of organisms. They were first described in mammalian liver where they are especially abundant and play an essential role in drug metabolism [32,33].
A list of selected mutant phenotypes that illustrate the various functions of P450 proteins is given in Table 1.
P450 enzymes have been compared to a blowtorch. They catalyze regiospecific and stereospecific oxidative attack of non-activated hydrocarbons at physiological temperatures. Such a reaction, uncatalyzed, would require extremely high temperature and would be nonspecific. The details of the mechanism by which P450s carry out all types of reactions, especially the most complex ones found in plants, are not yet understood. The best documented aspect is the oxygen activation that is common to most P450s, including soluble enzymes for which crystal structures of different forms have been obtained. The active center for catalysis is the iron-protoporphyrin IX (heme) with the thiolate of the conserved cysteine residue as fifth ligand. Resting P450 is in the ferric form and partially six-coordinated with a molecule of solvent (Figure 3).
The well characterized portion of the catalytic sequence involves four steps, which are indicated in Figure 3. The first step is substrate binding, with displacement of the sixth ligand solvent inducing a shift in the maximum of absorbance, spin state and redox potential of the heme protein system; the second is one-electron reduction of the complex to a ferrous state, driven by the increase in redox potential that results from the previous step; the third is binding of molecular oxygen to give a superoxide complex; and the fourth is a second reduction step leading to an 'activated oxygen species'. The exact nature of the very short-lived activated oxygen species that carries on substrate attack long remained uncertain, but the most recent data, from crystallography and mechanistic probes [20,34], strongly suggest that it is actually a mixture of two electrophilic oxidants ([B]- and [C] in Figure 3). Both iron-peroxo [B]- and iron-oxo [C] complexes are formed by protonation of the two-electrons-reduced dioxygen, a process that is allowed when a water channel forms in the groove of the I-helix upon binding of O2. The oxo (oxyferryl) species, resulting from the cleavage of the O-O bond - one atom of oxygen leaves with the two electrons and two protons as water - is apparently the most abundant. The iron-hydroperoxo species inserts the elements of OH+, producing protonated alcohols that can give cationic rearrangement products. The iron-oxo species inserts an oxygen atom. The result of P450 catalysis is not always insertion of oxygen, but can be a dealkylation, dehydration, dehydrogenation, isomerization, dimerization, carbon-carbon bond cleavage, and even a reduction . The substrate specificity and type of reaction catalyzed are governed by the less conserved regions of the protein and are therefore not well understood.
Carbon monoxide can bind ferrous P450 instead of dioxygen, inducing a shift of the maximum of absorbance of the heme (called the Soret peak) to 450 nm [32,33] (this property is a characteristic of P450 enzymes). CO is bound with high affinity and prevents binding and activation of O2. The result is an inhibition of P450 activity. CO binding and inhibition can be reversed by light, with maximal efficiency at 450 nm. Other ligands, substrates and inhibitors, induce absorbance shifts of the Soret in P450 enzymes. Differential spectrophotometry is thus widely used to monitor binding of such ligands . Substrates that displace the six-coordinated solvent in the resting P450 usually induce a shift to the blue (420 to 390 nm) which reflects a low- to high-spin transition of the iron. Inhibitors with an sp2 hybridized nitrogen (nitrogens in heterocycles such as azoles, pyridines, or pyrimidines) replace the sixth ligand for coordination with iron and induce a shift to the red (400 to 430 nm).
Issues most studied
Medical, pharmacological and toxicological studies of P450 enzymes and genes for the prediction of drug metabolism and the prevention of adverse drug reactions remain a key field of investigation. For instance, there are many allelic variants of the human CYP2D6 gene, which encodes a liver enzyme that metabolizes a quarter of all known drugs. The CYP2D6 genotype will determine a person's response to important drugs, such as antipsychotics and antidepressants. Another very active field is the tailoring of P450 enzymes for specific functions, via site-directed mutagenesis or in vitro directed evolution. The development of new approaches to improve solubility and implement crystallization of membrane-bound enzymes probably opens a new era for the understanding of P450 mechanisms and substrate specificity, as well as engineering of such catalytic properties.
Major unresolved questions
A major unresolved issue in the field is the physiological function of many of the newly discovered P450 enzymes. Whereas this question can be practically addressed in microorganisms or other organisms amenable to homologous recombination, this is not the case in most eukaryotes such as humans, where the endogenous substrate(s) of many enzymes that have been extensively studied for xenobiotic metabolism are still unknown. Also, the molecular basis and impact of receptor-mediated transcriptional activation of many P450 genes remains a challenging area of research. An interesting point to clarify is the subcellular localization of some P450 enzymes, some of which might have more than one localization. Many P450-catalyzed reactions in plants generate compounds that might be toxic if released in the cytoplasm. There is increasing evidence of the channeling of such compounds inside multi-enzyme complexes. How do P450s interact with such complexes, and do they serve to anchor them on membranes? From a mechanistic point of view, simple hydroxylation reactions are now rather well understood. More complex reactions, for example multi-step reactions or those involving no overt oxygen insertion, are still a very open field of investigation.
Nelson DR, Koymans L, Kamataki T, Stegeman JJ, Feyereisen R, Waxman DJ, Waterman MR, Gotoh O, Coon MJ, Estabrook RW, et al: P450 superfamily: update on new sequences, gene mapping, accession numbers and nomenclature. Pharmacogenetics. 1996, 6: 1-42. This paper defines the rules for P450 gene nomenclature, comments on some general characteristics of the P450 gene superfamilly, and gives a list (with references) of P450 genes identified in various organisms.
David Nelson's homepage. David Nelson keeps an update of P450 sequences characterized in all organisms and is also the 'P450 nomenclature committee', the person to contact to obtain a name for a new P450 sequence. Nelson also provides a simple introductory lecture on mammalian P450 enzymes and on all their physiological and other functions., [http://drnelson.utmem.edu/CytochromeP450.html]
Nelson DR: Cytochrome P450 and the individuality of species. Arch Biochem Biophys. 1999, 369: 1-10. 10.1006/abbi.1999.1352. This paper defines the clans in P450 classification and gives some examples. In addition to evolutionary considerations, it comments on new P450 genes and functions recently discovered and on P450 polymorphism and its impact on drug metabolism.
Ingelman-Sundberg M, Daly AK, Oscarson M, Nebert D: Human cytochrome P450 (CYP) gene: recommandations for the nomenclature of alleles. Pharmacogenetics. 2000, 10: 91-93. 10.1097/00008571-200002000-00012. This paper and the related website  give rules and examples for the nomenclature of P450 alleles.
Home Page of the Human Cytochrome P450 (CYP) Allele Nomenclature Committee. An update of the knowledge on allelic variants of the human genes; also provides instructions on the submission of new variants., [http://www.imm.ki.se/CYPalleles/]
Frey M, Chomet P, Glawischnig E, Stettner C, Grün S, Winklmair A, Eisenreich W, Bacher A, Meeley RB, Briggs SB, et al: Analysis of a chemical plant defense mechanism in grasses. Science. 1997, 277: 696-699. 10.1126/science.277.5326.696. The first analysis of a P450 gene cluster in plants (maize). Provides evidence that four evolutionary related P450 genes, belonging to same sub-family and clustered on the same chromosome, catalyze four successive steps in a single pathway.
Directory of P450-containing systems. Lists P450 and related genes. More information on P450 structure, ligands, domain structure, electron donors and useful links on human alleles, drug metabolism, commercially available forms; also contains references., [http://www.icgeb.trieste.it/~p450srv/]
The P450 site at the University of Arizona. A site with a list, annotation and a physical map of Drosophila and A. thaliana P450s., [http://ag.arizona.edu/p450/]
Rozman D, Stromstedt M, Tsui LC, Scherer SW, Waterman MR: Structure and mapping of the human lanosterol 14a-demethylase gene (CYP51) encoding the cytochrome P450 involved in cholesterol biosynthesis; comparison of exon/intron organization with other mammalian and fungal CYP genes. Genomics. 1996, 38: 371-381. 10.1006/geno.1996.0640. Provides a detailed analysis of a human P450 gene structure and comparative analysis of P450 gene structures in mammals and fungi.
Paquette SM, Bak S, Feyereisen R: Intron-exon organization and phylogeny in a large superfamily, the paralogous cytochrome P450 genes of Arabidopsis thaliana. DNA Cell Biol. 2000, 19: 307-317. 10.1089/10445490050021221. Provides a detailed analysis of the P450 gene family in A. thaliana: gene mapping, phylogeny and intron-exon organization.
Tijet N, Helvig C, Feyereisen R: The cytochrome P450 gene superfamily in Drosophila melanogaster: annotation, intron-exon organization and phylogeny. Gene. 2000, A complete report on the microsomal and mitochondrial P450s of the fruit fly, their gene structures and their distribution in the genome.,
Chapple C: Molecular genetics analysis of plant cytochrome P450-dependent monooxygenases. Ann Rev Plant Physiol Mol Biol. 1998, 49: 311-343. 10.1146/annurev.arplant.49.1.311. Provides some basic information on P450 characteristics and nomenclature; gives a list of plant P450 genes and mutants already isolated and their functions.
Gotoh O: Divergent structures of Caenorhabditis elegans cytochrome P450 genes suggest the frequent loss and gain of introns during the evolution of nematodes. Mol Biol Evol. 1998, 15: 1447-1459. An extensive study of gene structure in the nematode, with a thorough discussion of the process of intron gain and loss in the P450 superfamily.
Graham SE, Peterson JA: How similar are P450s and what can their differences teach us. Arch Biochem Biophys. 1999, 369: 24-29. 10.1006/abbi.1999.1350. A recent overview of the available data on P450 three-dimensional structure, comparison of the different crystallized structures in view of substrate specificity and redox partners of the different forms.
Gotoh O: Substrate recognition sites in cytochrome P450 family 2 (CYP2) protein inferred from comparative analyses of amino acid and coding nucleotide sequences. J Biol Chem. 1992, 267: 83-90. The reference paper defining the hyper-variable substrate recognition sites (SRSs).
Williams PA, Cosme J, Sridhar V, Johnson E, McRee DE: Mammalian microsomal cytochrome P450 monooxygenase: structural adaptations for membrane binding and functional diversity. Mol Cell. 2000, 5: 121-131. 10.1016/S1097-2765(00)80408-6. First structural report on a microsomal enzyme: describes similarities and difference with the soluble forms.
Julian A ('Bill') Peterson's home page. An easy access to didactic pictures illustrating P450 interaction with the P450-reductase and active-site structure., [http://p450terp.swmed.edu/Bills_folder/billhome.htm]
The Scripps Institute P450 protein site. Information on prosthetic group, different P450 types, reaction catalyzed, P450 enzyme, motif and alignment databases, three-dimensional (3D) structure databases and structural references., [http://metallo.scripps.edu/PROMISE/P450.html]
Poulos TL, Finzel BC, Gunsalus IC, Wagner GC, Kraut J: The 2.6-Å crystal structure of Pseudomonas putida cytochrome P-450. J Biol Chem. 1985, 260: 16122-16130. The first high-resolution structure of a bacterial soluble (class I) P450.
Schlichting I, Berendzen J, Chu K, Stock AM, Maves SA, Benson DE, Sweet RM, Ringe D, Petsko GA, Sligar SG: The catalytic pathway of cytochrome P450cam at atomic resolution. Science. 2000, 287: 1615-1622. 10.1126/science.287.5458.1615. The most recent update on the 3D structure of class I bacterial enzymes: includes the structure of one-electron-reduced forms and of the activated oxygen complex. Two forms of activated oxygen are detected in the crystal, confirming the biochemical data of .
Ravichandran KG, Boddupalli SS, Hasemann CA, Peterson JA, Deisendorfer J: Crystal structure of hemoprotein domain of P450BM-3, a prototype for microsomal P450's. Science. 1993, 261: 731-736. The first description of the 3D structure of a class II enzyme. Until the coordinates of the mammalian CYP2C5 become available, probably in the next year, this serves as a reference for the eukaryotic membrane-bound enzymes.
Li H, Poulos TL: The structure of the cytochrome P450BM-3 haem domain complexed with the fatty acid substrate, palmitoleic acid. Nat Struct Biol. 1997, 4: 140-146. A very interesting description of the class II enzyme crystallized with its substrate. A model for fatty-acid-metabolizing P450s in all kingdoms, providing the first detailed picture of substrate-induced conformational changes in a P450.
Park SY, Shimizu H, Adachi S, Nakagawa A, Tanaka I, Nakahara K, Shoun H, Obayashi E, Nakamura H, Iizuka T, Shiro Y: Crystal structure of nitric oxide reductase from denitrifying fungus Fusarium oxysporum. Nat Struct Biol. 1997, 10: 827-832. First description of the 3D structure of a class IV enzyme. Provides evidence of significant differences in proton delivery and access of NADH to the active site.
Hasler JA, Estabrook R, Murray M, Pikuleva I, Waterman M, Capdevila J, Holla V, Helvig C, Falck JR, Farrell G, et al: Human cytochromes P450. Mol Aspects Med. 1999, 20: 1-137. 10.1016/S0098-2997(99)00005-9. A very complete overview of P450 roles in human normal physiology, pathology and drug metabolism.
Feyereisen R: Insect cytochrome P450 enzymes. Annu Rev Entomol. 1999, 44: 507-533. 10.1146/annurev.ento.44.1.507. Provides a review of the physiological functions of insect P450 as well as the role and regulation of P450 in insecticide metabolism, insecticide resistance, and the adaptation to plant chemicals.
Kahn R, Durst F: Function and evolution of plant cytochrome P450. Recent Adv Phytochem. 2000, 34: 151-189. The most recent review on the role of P450 enzymes in the biosynthesis of plant natural compounds. Also comments on plant P450 evolution and techniques useful for plant P450 gene isolation.
Gonzalez FJ, Kimura S: Role of gene knockout mice in understanding the mechanisms of chemical toxicity and carcinogenesis. Cancer Lett. 1999, 143: 199-204. 10.1016/S0304-3835(99)00125-1. Provides a description of the gene disruption technology in the mouse and its application for the study of three P450 genes involved in xenobiotic metabolism.
Werck-Reichhart D, Hehn H, Didierjean L: Cytochromes P450 for engineering herbicide tolerance. Trends Plant Sci. 2000, 5: 116-123. 10.1016/S1360-1385(00)01567-3. Reviews available data in the metabolism of exogenous compounds, in particular herbicides, in higher plants and the impact of altered metabolism on weed resistance.
Waxman DJ: P450 gene induction by structurally diverse xenochemicals: central role of nuclear receptors CAR, PXR, and PPAR. Arch Biochem Biophys. 1999, 369: 11-23. 10.1006/abbi.1999.1351. Summarizes recent progress in nuclear receptor driven regulation of mammalian P450s by xenochemicals. The expression of different P450 families is driven by specific nuclear receptors of the family NR1 activated by exogenous and endogenous ligands.
Honkakoski P, Negishi M: Regulation of cytochrome P450 genes by nuclear receptors. Biochem J. 2000, 347: 321-337. 10.1042/0264-6021:3470321. Gives an overview of the nuclear receptors involved in P450 gene regulation, of their respective role in endobiotic and xenobiotic metabolism, with emphasis on the potential impact of exogenous compounds on cellular homeostasis.
Mansuy D: The great diversity of reactions catalyzed by cytochrome P450. Comp Biochem Physiol C Pharmacol Toxicol Endocrinol. 1998, 121: 5-14. 10.1016/S0742-8413(98)10026-9. A good simplified overview on the diversity and mechanism of reaction catalyzed by P450 enzymes.
Klingenberg M: Pigments of rat liver microsomes. Arch Biochem Biophys. 1958, 75: 376-386. First description of a pigment absorbing at 450 nm when reduced in mammalian liver microsomes.
Omura T, Sato R: The carbon monoxide-binding pigment of liver microsomes. I. Evidence for its hemoprotein nature. J Biol Chem. 1964, 239: 2370-2378. Demonstration of the hemoprotein nature of the pigment absorbing at 450 nm: gives the extinction coefficient used for all P450 quantifications.
Newcomb M, Shen R, Choi S-Y, Toy PH, Hollenberg PF, Vaz AND, Coon MJ: Cytochrome P450-catalyzed hydroxylation of mechanistic probes that distinguish between radical and cations. evidence for cationic but not radical intermediates. J Am Chem Soc. 2000, 122: 2677-2686. 10.1021/ja994106+. The most recent update on P450 catalytical mechanism. Provides evidence of the existence of two activated oxygen forms (iron-oxo and hydroperoxo-iron) for the same enzymes, both forms producing different products with mechanistic probes. Also gives evidence that the reaction occurs in both cases by direct insertion.
Jefcoate CR: Measurement of substrate and inhibitor binding to microsomal cytochrome P450 by optical difference spectroscopy. Methods Enzymol. 1978, 52: 258-279. 10.1016/S0076-6879(78)52029-6. A reference paper that provides the basis for ligand-binding detection by spectrophotometry.
Fred K. Friedman's Home Page. The place to see a model of P450 insertion in a membrane., [http://rex.nci.nih.gov/RESEARCH/basic/lm/fkf.htm]
Williams PA, Cosme J, Sridhar V, Johnson EF, McRee DE: Microsomal cytochrome P450 2C5: comparison to microbial P450s and unique features. J Inorg Biochem. 2000, 81: 183-190. 10.1016/S0162-0134(00)00102-1. More pictures to illustrate the differences between microbial and membrane-bound proteins.
Stoilov I, Akarsu AN, Sarfarazi M: Identification of three different truncating mutations in cytochrome P4501B1 (CYP1B1) as the principal cause of primary congenital glaucoma (Buphthalmos) in families linked to the GLC3A locus on chromosome 2p21. Hum Mol Genet. 1997, 6: 641-647. 10.1093/hmg/6.4.641. Three null alleles described in five well characterized families point to the lack of CYP1B1 as causing developmental defects in the anterior anterior uveal tract, which is involved in secretion of the aqueous humor. A point mutation in CYP1B1 has since been identified at very high frequency (10%) in an ethnic isolate of Slovak Gypsies, a population with increased incidence of primary congenital glaucoma. The substrate of CYP1B1 is unknown.
Geller DH, Auchus RJ, Mendonça BB, Miller W: The genetic and functional basis of isolated 17,20-lyase deficiency. Nat Genet. 1997, 17: 201-205. The mammalian P450 CYP17 is an unusual P450 catalyzing two successive reactions in the biosynthesis of steroids. Its 17a-hydroxylase activity is sufficient for the biosynthesis of glucocorticoids. Successive 17a-hydroxylase and 17,20-lyase activities catalyzed by CYP17 are needed for the biosynthesis of steroid hormones. Here human mutants forms are described which retain normal 17a-hydroxylase activity but are severely defective in 17,20-lyase activity. It is shown that the defect is due to a diminished ability of the P450 to interact with its redox partners.
Stratakis CA, Vottero A, Brodie A, Kirschner LS, DeAtkine D, Lu Q, Yue W, Mitsiades CS, Flor AW, Chrousos GP: The aromatase excess syndrome is associated with feminization of both sexes and autosomal dominant transmission of aberrant P450 aromatase gene transcription. J Clin Endocrinol Metab. 1998, 83: 1348-1357. 10.1210/jc.83.4.1348. A case of familial gynecomastia is described in which a new 5' splicing variant leads to the abnormal overexpression of an aromatase transcript with a new first exon. The excess aromatase syndrome is described in both sexes.
Delye C, Laigret F, Corio-Costet MF: A mutation in the 14a-demethylase gene of Uncinula necator that correlates with resistance to a sterol biosynthesis inhibitor. Appl Environ Microbiol. 1997, 63: 2966-2970. Resistance of the grape powdery mildew to 14a-demethylase inhibitors such as triadimenol was correlated in multiple isolates with a single Phe137Tyr point mutation in the CYP51 gene. The same mutation can be found in other resistant fungi.
Chapple CCS, Vogt T, Ellis BE, Somerville CR: An Arabidopsis mutant defective in the general phenylpropanoid pathway. Plant Cell. 1992, 4: 1413-1424. 10.1105/tpc.4.11.1413. Decribes a recessive mutant deficient in the synthesis of sinapoylmalate, selected on the basis of a change in leaf epidermis fluorescence (blue-green to red) under UV-light. On the basis of feeding and precursor supplementation experiments it is shown that this mutant is defective for the 5-hydroxylation step in the general phenylpropanoid pathway, a reaction previously shown to be catalyzed by a P450 enzyme. After isolation of the mutant, it took several years to identify the real substrate of the reaction, which was different from expected.
Szekeres M, Nemeth K, Koncs-Kalman Z, Mathur J, Kauschmann A, Altmann T, Redei GP, Nagy F, Schell J, Koncs C: Brassinosteroids rescue the deficiency of CYP90, a cytochrome P450 controlling cell elongation and de-etiolation in Arabidopsis. Cell. 1996, 85: 171-182. 10.1016/S0092-8674(00)81094-6. Describes a recessive mutant selected on the basis of hypocotyl and root elongation during skotomorphogenesis, displaying de-etiolation in the dark and dwarfism, male sterility and activation of stress-regulated genes in the light. The defect can be rescued by C23-hydroxylated brassinolide precursors, which demonstrates the involvement of the tagged gene in the biosynthesis of brassinosteroid hormones which are essential for plant development. Other P450-catalyzed steps were subsequently characterized in the same pathway using similar approaches.
Neff MM, Nguyen SM, Malancharuvil EJ, Fujioka S, Noguchi T, Seto H, Tsubuki M, Honda T, Takatsuto S, Chory J: BAS1: a gene regulating brassinosteroid level and light responsiveness in Arabidopsis. Proc Natl Acad Sci USA. 1999, 96: 15316-15323. 10.1073/pnas.96.26.15316. This paper reports the first functional characterization of a P450 gene by activation tagging. A dominant mutation suppresses the missense mutation in the photoreceptor phytochrome B. The mutant has no detectable brassinolide, the most active brassinosteroid hormone and accumulate a 26-hydroxylated inactive metabolite. Crosses suggest that the activated gene is a control point between photoreceptor signal transduction pathways and hormone signaling.
Holton TA, Brugliera F, Lester DR, Tanaka Y, Hyland CD, Menting JGT, Lu C-Y, Farcy E, Stevenson TW, Cornish EC: Cloning and expression of cytochrome P450 genes controlling flower colour. Nature. 1993, 366: 276-279. 10.1038/366276a0. Describes the PCR-based isolation of two P450 genes complementing flower-color mutations of petunia. Provides the definitive proof that P450-dependent hydroxylation of the ring B of flavonoids is a major determinant of pink-to-blue shift of flower color.
Chavez VM, Marques G, Delbecque JP, Kobayashi K, Hollingsworth M, Burr J, Natzle JE, O'Connor MB: The Drosophila disembodied gene controls late embryonic morphogenesis and codes for a cytochrome P450 enzyme that regulates embryonic ecdysone levels. Development. 2000, 127: 4115-4126. The dib gene is shown to encode CYP302AI, a mitochondrial P450. Mutants at this locus have very low titers of ecdysteroids (molting hormones) and are defective in edysteroid-regulated processes such as embryonic cuticle synthesis or induction of ecdysteroid-responsive genes.
Mingot JM, Penalva MA, Fernandez-Canon JM: Disruption of phacA, an Aspergillus nidulans gene encoding a novel cytochrome P450 monooxygenase catalyzing phenylacetate 2-hydroxylation, results in penicillin overproduction. J Biol Chem. 1999, 274: 14545-14550. 10.1074/jbc.274.21.14545. CYP504 is induced by and metabolizes phenylacetate in this aerobic fungus by a rare ortho-hydroxylation. This catabolism competes with the use of phenylacetate in the penicillin biosynthetic pathway, and disruption of the CYP504 gene leads to penicillin overproduction.