Abstract
Fungi contain a remarkable diversity of both primary and secondary metabolic pathways involved in ecologically specialized or accessory functions. Genes in these pathways are frequently physically linked on fungal chromosomes, forming metabolic gene clusters (MGCs). In this Review, we describe the diversity in the structure and content of fungal MGCs, their population-level and species-level variation, the evolutionary mechanisms that underlie their formation, maintenance and decay, and their ecological and evolutionary impact on fungal populations. We also discuss MGCs from other eukaryotes and the reasons for their preponderance in fungi. Improved knowledge of the evolutionary life cycle of MGCs will advance our understanding of the ecology of specialized metabolism and of the interplay between the lifestyle of an organism and genome architecture.
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References
Whittaker, R. H. New concepts of kingdoms or organisms. Science 163, 150–160 (1969).
Richards, T. A. & Talbot, N. J. Horizontal gene transfer in osmotrophs: playing with public goods. Nat. Rev. Microbiol. 11, 720–727 (2013).
Pusztahelyi, T., Holb, I. J. & Pocsi, I. Secondary metabolites in fungus-plant interactions. Frontiers Plant Sci. 6, 573 (2015).
Stergiopoulos, I., Collemare, J., Mehrabi, R. & De Wit, P. J. Phytotoxic secondary metabolites and peptides produced by plant pathogenic Dothideomycete fungi. FEMS Microbiol. Rev. 37, 67–93 (2013).
Keller, N. P., Turner, G. & Bennett, J. W. Fungal secondary metabolism — from biochemistry to genomics. Nat. Rev. Microbiol. 3, 937–947 (2005).
Keller, N. P. & Hohn, T. M. Metabolic pathway gene clusters in filamentous fungi. Fungal Genet. Biol. 21, 17–29 (1997).
Yue, Q. et al. Functional operons in secondary metabolic gene clusters in Glarea lozoyensis (Fungi, Ascomycota, Leotiomycetes). MBio 6, e00703 (2015).
Johnstone, I. L. et al. Isolation and characterisation of the crnA-niiA-niaD gene cluster for nitrate assimilation in Aspergillus nidulans. Gene 90, 181–192 (1990).
Slot, J. C. & Hibbett, D. S. Horizontal transfer of a nitrate assimilation gene cluster and ecological transitions in fungi: a phylogenetic study. PLOS One 2, e1097 (2007). This is the first reported case in fungi of the acquisition of an entire metabolic pathway by horizontal transfer of an MGC.
Wong, S. & Wolfe, K. H. Birth of a metabolic gene cluster in yeast by adaptive gene relocation. Nat. Genet. 37, 777–782 (2005). This is the first study to show that fungal MGCs originate by relocation of native genes.
Slot, J. C. & Rokas, A. Multiple GAL pathway gene clusters evolved independently and by different mechanisms in fungi. Proc. Natl Acad. Sci. USA 107, 10136–10141 (2010).
Hall, C. & Dietrich, F. S. The reacquisition of biotin prototrophy in Saccharomyces cerevisiae involved horizontal gene transfer, gene duplication and gene clustering. Genetics 177, 2293–2307 (2007). This study shows that the biotin pathway in the baker’s yeast, whose five of the six genes reside in two subtelomeric gene clusters, was lost in an ancestor but was subsequently rebuilt through acquisition of bacterial genes via HGT and gene duplication followed by neofunctionalization.
Penalva, M. A. A fungal perspective on human inborn errors of metabolism: alkaptonuria and beyond. Fungal Genet. Biol. 34, 1–10 (2001).
Hull, E. P., Green, P. M., Arst, H. N. Jr & Scazzocchio, C. Cloning and physical characterization of the L-proline catabolism gene cluster of Aspergillus nidulans. Mol. Microbiol. 3, 553–559 (1989).
Bobrowicz, P., Wysocki, R., Owsianik, G., Goffeau, A. & Ulaszewski, S. Isolation of three contiguous genes. ACR1, ACR2 and ACR3, involved in resistance to arsenic compounds in the yeast Saccharomyces cerevisiae. Yeast 13, 819–828 (1997).
Elmore, M. H. et al. Clustering of two genes putatively involved in cyanate detoxification evolved recently and independently in multiple fungal lineages. Genome Biol. Evol. 7, 789–800 (2015).
Yu, J. et al. Clustered pathway genes in aflatoxin biosynthesis. Appl. Environ. Microbiol. 70, 1253–1262 (2004).
Brown, D. W., Dyer, R. B., McCormick, S. P., Kendra, D. F. & Plattner, R. D. Functional demarcation of the Fusarium core trichothecene gene cluster. Fungal Genet. Biol. 41, 454–462 (2004).
Schardl, C. L. et al. Plant-symbiotic fungi as chemical engineers: multi-genome analysis of the clavicipitaceae reveals dynamics of alkaloid Loci. PLOS Genet. 9, e1003323 (2013). This is a comprehensive reconstruction of the evolutionary dynamics of MGCs responsible for four classes of alkaloid toxins, which are characterized by conserved cores of genes that specify the chemical skeleton structures of the toxins and various peripheral genes that are likely involved in chemical variations in toxin structures and their pharmacological effects.
Diez, B. et al. The cluster of penicillin biosynthetic genes. Identification and characterization of the pcbAB gene encoding the alpha-aminoadipyl-cysteinyl-valine synthetase and linkage to the pcbC and penDE genes. J. Biol. Chem. 265, 16358–16365 (1990).
Kennedy, J. et al. Modulation of polyketide synthase activity by accessory proteins during lovastatin biosynthesis. Science 284, 1368–1372 (1999).
Kimura, N. & Tsuge, T. Gene cluster involved in melanin biosynthesis of the filamentous fungus Alternaria alternata. J. Bacteriol. 175, 4427–4435 (1993).
Terabayashi, Y. et al. Identification and characterization of genes responsible for biosynthesis of kojic acid, an industrially important compound from Aspergillus oryzae. Fungal Genet. Biol. 47, 953–961 (2010).
Lind, A. L. et al. Examining the evolution of the regulatory circuit controlling secondary metabolism and development in the fungal genus Aspergillus. PLOS Genet. 11, e1005096 (2015).
Sanchez, J. F., Somoza, A. D., Keller, N. P. & Wang, C. C. Advances in Aspergillus secondary metabolite research in the post-genomic era. Nat. Prod. Rep. 29, 351–371 (2012).
Brakhage, A. A. Regulation of fungal secondary metabolism. Nat. Rev. Microbiol. 11, 21–32 (2013).
Bradshaw, R. E. et al. Fragmentation of an aflatoxin-like gene cluster in a forest pathogen. New Phytol. 198, 525–535 (2013).
Sanchez, J. F. et al. Genome-based deletion analysis reveals the prenyl xanthone biosynthesis pathway in Aspergillus nidulans. J. Am. Chem. Soc. 133, 4010–4017 (2011).
McGary, K. L., Slot, J. C. & Rokas, A. Physical linkage of metabolic genes in fungi is an adaptation against the accumulation of toxic intermediate compounds. Proc. Natl Acad. Sci. USA 110, 11481–11486 (2013). This study shows that fungal metabolic genes that handle toxic compounds are more likely to be clustered, suggesting that the phenotype selection acts on to drive gene clustering is the mitigation of toxicity of pathway intermediates.
Eidem, H. R., McGary, K. L. & Rokas, A. Shared selective pressures on fungal and human metabolic pathways lead to divergent yet analogous genetic responses. Mol. Biol. Evol. 32, 1449–1455 (2015).
Hane, J. K. et al. A novel mode of chromosomal evolution peculiar to filamentous Ascomycete fungi. Genome Biol. 12, R45 (2011).
Siverio, J. M. Assimilation of nitrate by yeasts. FEMS Microbiol. Rev. 26, 277–284 (2002).
Scazzocchio, C. Fungal biology in the post-genomic era. Fungal Biol. Biotechnol. 1, 7 (2014).
Yu, J., Chang, P., Bhatnagar, D. & Cleveland, T. E. Cloning of a sugar utilization gene cluster in Aspergillus parasiticus. Biochim. Biophys. Acta 1493, 211–214 (2000).
Schrettl, M. et al. Self-protection against gliotoxin — a component of the gliotoxin biosynthetic cluster, GliT, completely protects Aspergillus fumigatus against exogenous gliotoxin. PLOS Pathog. 6, e1000952 (2010). This study reports that a gene within the gliotoxin MGC is necessary and sufficient for conferring protection against gliotoxin poisoning, thus providing a competitive advantage for organisms carrying it when grown in the presence of competitors that produce gliotoxin.
Wiemann, P. et al. Biosynthesis of the red pigment bikaverin in Fusarium fujikuroi: genes, their function and regulation. Mol. Microbiol. 72, 931–946 (2009).
Hittinger, C. T., Rokas, A. & Carroll, S. B. Parallel inactivation of multiple GAL pathway genes and ecological diversification in yeasts. Proc. Natl Acad. Sci. USA 101, 14144–14149 (2004).
Martchenko, M., Levitin, A., Hogues, H., Nantel, A. & Whiteway, M. Transcriptional rewiring of fungal galactose metabolism circuitry. Curr. Biol. 17, 1007–1013 (2007).
Lim, F. Y. et al. Genome-based cluster deletion reveals an endocrocin biosynthetic pathway in Aspergillus fumigatus. Appl. Environ. Microbiol. 78, 4117–4125 (2012).
Szewczyk, E. et al. Identification and characterization of the asperthecin gene cluster of Aspergillus nidulans. Appl. Environ. Microbiol. 74, 7607–7612 (2008).
Chiang, Y. M. et al. Molecular genetic mining of the Aspergillus secondary metabolome: discovery of the emericellamide biosynthetic pathway. Chem. Biol. 15, 527–532 (2008).
Bushley, K. E. et al. The genome of Tolypocladium inflatum: evolution, organization, and expression of the cyclosporin biosynthetic gene cluster. PLOS Genet. 9, e1003496 (2013).
Inderbitzin, P., Asvarak, T. & Turgeon, B. G. Six new genes required for production of T-toxin, a polyketide determinant of high virulence of Cochliobolus heterostrophus to maize. Mol. Plant Microbe Interact. 23, 458–472 (2010).
Yin, W. B. et al. A nonribosomal peptide synthetase-derived iron(III) complex from the pathogenic fungus Aspergillus fumigatus. J. Am. Chem. Soc. 135, 2064–2067 (2013).
Umemura, M. et al. Characterization of the biosynthetic gene cluster for the ribosomally synthesized cyclic peptide ustiloxin B in Aspergillus flavus. Fungal Genet. Biol. 68, 23–30 (2014).
Gutierrez, S., Fierro, F., Casqueiro, J. & Martin, J. F. Gene organization and plasticity of the beta-lactam genes in different filamentous fungi. Antonie Van Leeuwenhoek 75, 81–94 (1999).
Lo, H. C. et al. Two separate gene clusters encode the biosynthetic pathway for the meroterpenoids austinol and dehydroaustinol in Aspergillus nidulans. J. Am. Chem. Soc. 134, 4709–4720 (2012).
Proctor, R. H., McCormick, S. P., Alexander, N. J. & Desjardins, A. E. Evidence that a secondary metabolic biosynthetic gene cluster has grown by gene relocation during evolution of the filamentous fungus Fusarium. Mol. Microbiol. 74, 1128–1142 (2009).
Nicholson, M. J. et al. Identification of two aflatrem biosynthesis gene loci in Aspergillus flavus and metabolic engineering of Penicillium paxilli to elucidate their function. Appl. Environ. Microbiol. 75, 7469–7481 (2009).
Wiemann, P. et al. Prototype of an intertwined secondary-metabolite supercluster. Proc. Natl Acad. Sci. USA 110, 17065–17070 (2013). This study is the first to report the existence of intertwined MGCs responsible for the production of at least two distinct secondary metabolites in fungal genomes.
Lind, A. L. et al. Drivers of genetic diversity in secondary metabolic gene clusters within a fungal species. PLOS Biol. 15, e2003583 (2017). This is the first study, together with that by Gibbons et al. (2012), to report that two non-homologous MGCs occupy the same locus (that is, an idiomorph polymorphism) and is the first to describe patterns of genome-wide variation of secondary MGCs in a fungal species.
Medini, D., Donati, C., Tettelin, H., Masignani, V. & Rappuoli, R. The microbial pan-genome. Curr. Opin. Genet. Dev. 15, 589–594 (2005).
Chang, P. K., Horn, B. W. & Dorner, J. W. Sequence breakpoints in the aflatoxin biosynthesis gene cluster and flanking regions in nonaflatoxigenic Aspergillus flavus isolates. Fungal Genet. Biol. 42, 914–923 (2005).
Wiemann, P. et al. Deciphering the cryptic genome: genome-wide analyses of the rice pathogen Fusarium fujikuroi reveal complex regulation of secondary metabolism and novel metabolites. PLOS Pathog. 9, e1003475 (2013).
Chiara, M. et al. Genome sequencing of multiple isolates highlights subtelomeric genomic diversity within Fusarium fujikuroi. Genome Biol. Evol. 7, 3062–3069 (2015).
Castella, G., Bragulat, M. R., Puig, L., Sanseverino, W. & Cabanes, F. J. Genomic diversity in ochratoxigenic and non ochratoxigenic strains of Aspergillus carbonarius. Sci. Rep. 8, 5439 (2018).
Hartmann, F. E. & Croll, D. Distinct trajectories of massive recent gene gains and losses in populations of a microbial eukaryotic pathogen. Mol. Biol. Evol. 34, 2808–2822 (2017).
Campbell, M. A., Rokas, A. & Slot, J. C. Horizontal transfer and death of a fungal secondary metabolic gene cluster. Genome Biol. Evol. 4, 289–293 (2012).
Campbell, M. A., Staats, M., van Kan, J. L. A., Rokas, A. & Slot, J. C. Repeated loss of an anciently horizontally transferred gene cluster in Botrytis. Mycologia 105, 1126–1134 (2013).
Schumacher, J. et al. A functional bikaverin biosynthesis gene cluster in rare strains of Botrytis cinerea is positively controlled by VELVET. PLOS One 8, e53729 (2013).
Hittinger, C. T. et al. Remarkably ancient balanced polymorphisms in a multi-locus gene network. Nature 464, 54–58 (2010).
Gibbons, J. G. et al. The evolutionary imprint of domestication on genome variation and function of the filamentous fungus Aspergillus oryzae. Curr. Biol. 22, 1403–1409 (2012). Together with the study by Lind et al., these are the first studies to report that two non-homologous MGCs occupy the same locus (that is, an idiomorph polymorphism) in the genome of a fungal species.
Keller-Seitz, M. U. et al. Transcriptional response of yeast to aflatoxin B1: recombinational repair involving RAD51 and RAD1. Mol. Biol. Cell 15, 4321–4336 (2004).
Fedorova, N. D. et al. Genomic islands in the pathogenic filamentous fungus Aspergillus fumigatus. PLOS Genet. 4, e1000046 (2008).
Metzenberg, R. L. & Glass, N. L. Mating type and mating strategies in Neurospora. Bioessays 12, 53–59 (1990).
Mukherjee, P. K., Horwitz, B. A. & Kenerley, C. M. Secondary metabolism in Trichoderma—a genomic perspective. Microbiology 158, 35–45 (2012).
Rank, C. et al. Distribution of sterigmatocystin in filamentous fungi. Fungal Biol. 115, 406–420 (2011).
Khaldi, N. et al. SMURF: genomic mapping of fungal secondary metabolite clusters. Fungal Genet. Biol. 47, 736–741 (2010).
de Vries, R. P. et al. Comparative genomics reveals high biological diversity and specific adaptations in the industrially and medically important fungal genus Aspergillus. Genome Biol. 18, 28 (2017).
Riley, R. et al. Comparative genomics of biotechnologically important yeasts. Proc. Natl Acad. Sci. USA 113, 9882–9887 (2016).
Khaldi, N., Collemare, J., Lebrun, M. H. & Wolfe, K. H. Evidence for horizontal transfer of a secondary metabolite gene cluster between fungi. Genome Biol. 9, R18 (2008).
Reynolds, H. T. et al. Differential retention of gene functions in a secondary metabolite cluster. Mol. Biol. Evol. 34, 2002–2015 (2017).
Zhang, H., Rokas, A. & Slot, J. C. Two different secondary metabolism gene clusters occupied the same ancestral locus in fungal dermatophytes of the Arthrodermataceae. PLOS One 7, e41903 (2012).
Dalal, C. K. et al. Transcriptional rewiring over evolutionary timescales changes quantitative and qualitative properties of gene expression. elife 5, e18981 (2016).
Proctor, R. H. et al. Evolution of structural diversity of trichothecenes, a family of toxins produced by plant pathogenic and entomopathogenic fungi. PLOS Pathog. 14, e1006946 (2018).
Carbone, I., Ramirez-Prado, J. H., Jakobek, J. L. & Horn, B. W. Gene duplication, modularity and adaptation in the evolution of the aflatoxin gene cluster. BMC Evol. Biol. 7, 111 (2007).
Slot, J. C. & Rokas, A. Horizontal transfer of a large and highly toxic secondary metabolic gene cluster between fungi. Curr. Biol. 21, 134–139 (2011). This study reports the horizontal transfer of a large MGC (at least 57 kb of sequence, 24 genes) involved in the making of the mycotoxin sterigmatocystin between fungi.
Ehrlich, K. C., Chang, P. K., Yu, J. & Cotty, P. J. Aflatoxin biosynthesis cluster gene cypA is required for G aflatoxin formation. Appl. Environ. Microbiol. 70, 6518–6524 (2004).
Proctor, R. H., Busman, M., Seo, J. A., Lee, Y. W. & Plattner, R. D. A fumonisin biosynthetic gene cluster in Fusarium oxysporum strain O-1890 and the genetic basis for B versus C fumonisin production. Fungal Genet. Biol. 45, 1016–1026 (2008).
Rosewich, U. L. & Kistler, H. C. Role of horizontal gene transfer in the evolution of fungi. Annu. Rev. Phytopathol. 38, 325–363 (2000).
Wisecaver, J. H. & Rokas, A. Fungal metabolic gene clusters-caravans traveling across genomes and environments. Front. Microbiol. 6, 161 (2015).
Reynolds, H. T. et al. Horizontal gene cluster transfer increased hallucinogenic mushroom diversity. Evol. Lett. 2, 88–101 (2018).
Patron, N. J. et al. Origin and distribution of epipolythiodioxopiperazine (ETP) gene clusters in filamentous ascomycetes. BMC Evol. Biol. 7, 174 (2007).
Matasyoh, J. C., Dittrich, B., Schueffler, A. & Laatsch, H. Larvicidal activity of metabolites from the endophytic Podospora sp. against the malaria vector Anopheles gambiae. Parasitol. Res. 108, 561–566 (2011).
Matsuzawa, T. et al. New insights into galactose metabolism by Schizosaccharomyces pombe: isolation and characterization of a galactose-assimilating mutant. J. Biosci. Bioeng. 111, 158–166 (2011).
Ortiz, J. F. & Rokas, A. CTDGFinder: a novel homology-based algorithm for identifying closely spaced clusters of tandemly duplicated genes. Mol. Biol. Evol. 34, 215–229 (2017).
Nei, M. Modification of linkage intensity by natural selection. Genetics 57, 625–641 (1967).
Ward, T. J., Bielawski, J. P., Kistler, H. C., Sullivan, E. & O’Donnell, K. Ancestral polymorphism and adaptive evolution in the trichothecene mycotoxin gene cluster of phytopathogenic Fusarium. Proc. Natl Acad. Sci. USA 99, 9278–9283 (2002). This is the first study to report evidence for trans-specific polymorphism in the gene cluster of the trichothecene mycotoxin, which is maintained by balancing selection acting on chemotype differences.
Carbone, I., Jakobek, J. L., Ramirez-Prado, J. H. & Horn, B. W. Recombination, balancing selection and adaptive evolution in the aflatoxin gene cluster of Aspergillus parasiticus. Mol. Ecol. 16, 4401–4417 (2007).
Hartmann, F. E., McDonald, B. A. & Croll, D. Genome-wide evidence for divergent selection between populations of a major agricultural pathogen. Mol. Ecol. 27, 2725–2741 (2018).
Grandaubert, J., Dutheil, J. Y. & Stukenbrock, E. H. The genomic determinants of adaptive evolution in a fungal pathogen. Preprint at bioRxiv. https://doi.org/10.1101/176727 (2018).
Morris, J. J., Lenski, R. E. & Zinser, E. R. The Black Queen hypothesis: evolution of dependencies through adaptive gene loss. MBio 3, e00036–12 (2012).
Hurst, L. D., Pal, C. & Lercher, M. J. The evolutionary dynamics of eukaryotic gene order. Nat. Rev. Genet. 5, 299–310 (2004).
Gibbons, J. G. et al. Global transcriptome changes underlying colony growth in the opportunistic human pathogen Aspergillus fumigatus. Eukaryot. Cell 11, 68–78 (2012).
Lind, A. L., Smith, T. D., Saterlee, T., Calvo, A. M. & Rokas, A. Regulation of secondary metabolism by the Velvet complex is temperature-responsive in Aspergillus. G3 6, 4023–4033 (2016).
Yu, J. J. et al. Tight control of mycotoxin biosynthesis gene expression in Aspergillus flavus by temperature as revealed by RNA-Seq. FEMS Microbiol. Lett. 322, 145–149 (2011).
Andersen, M. R. et al. Accurate prediction of secondary metabolite gene clusters in filamentous fungi. Proc. Natl Acad. Sci. USA 110, E99–E107 (2013).
Lawler, K., Hammond-Kosack, K., Brazma, A. & Coulson, R. M. Genomic clustering and co-regulation of transcriptional networks in the pathogenic fungus Fusarium graminearum. BMC Syst. Biol. 7, 52 (2013).
Wisecaver, J. H. et al. A global coexpression network approach for connecting genes to specialized metabolic pathways in plants. Plant Cell 29, 944–959 (2017).
Kensche, P. R., Oti, M., Dutilh, B. E. & Huynen, M. A. Conservation of divergent transcription in fungi. Trends Genet. 24, 207–211 (2008).
Fernandes, M., Keller, N. P. & Adams, T. H. Sequence-specific binding by Aspergillus nidulans AflR, a C6 zinc cluster protein regulating mycotoxin biosynthesis. Mol. Microbiol. 28, 1355–1365 (1998).
Gacek, A. & Strauss, J. The chromatin code of fungal secondary metabolite gene clusters. Appl. Microbiol. Biotechnol. 95, 1389–1404 (2012).
Moore, G. G., Singh, R., Horn, B. W. & Carbone, I. Recombination and lineage-specific gene loss in the aflatoxin gene cluster of Aspergillus flavus. Mol. Ecol. 18, 4870–4887 (2009). Extensive analysis of patterns of linkage disequilibrium in the aflatoxin gene cluster of A. flavus suggests that recombination events are unevenly distributed across the cluster, including the absence of recombination for the subcluster of genes acting early in the aflatoxin synthesis pathway.
Olarte, R. A. et al. Effect of sexual recombination on population diversity in aflatoxin production by Aspergillus flavus and evidence for cryptic heterokaryosis. Mol. Ecol. 21, 1453–1476 (2012).
Walton, J. D. Horizontal gene transfer and the evolution of secondary metabolite gene clusters in fungi: an hypothesis. Fungal Genet. Biol. 30, 167–171 (2000).
Lang, G. I. & Botstein, D. A test of the coordinated expression hypothesis for the origin and maintenance of the GAL cluster in yeast. PLOS One 6, e25290 (2011). This study reports that disruption of the clustering in the galactose pathway does not reduce fitness, arguing against the hypothesis that gene clustering increases fitness because it enables greater coordination of gene expression.
Naseeb, S. & Delneri, D. Impact of chromosomal inversions on the yeast DAL cluster. PLOS One 7, e42022 (2012).
Leslie, N. D. Insights into the pathogenesis of galactosemia. Annu. Rev. Nutr. 23, 59–80 (2003).
Alam, M. K. & Kaminskyj, S. G. W. Aspergillus galactose metabolism is more complex than that of Saccharomyces: the story of GalD(GAL7) and GalE(GAL1). Botany 91, 467–477 (2013).
Slot, J. C. Fungal gene cluster diversity and evolution. Adv. Genet. 100, 141–178 (2017).
Wisecaver, J. H., Slot, J. C. & Rokas, A. The evolution of fungal metabolic pathways. PLOS Genet. 10, e1004816 (2014).
Gibbons, J. G. & Rokas, A. The function and evolution of the Aspergillus genome. Trends Microbiol. 21, 14–22 (2013).
Lynch, M. The Origins of Genome Architecture. (Sinauer, 2007).
Lewontin, R. C. On measures of gametic disequilibrium. Genetics 120, 849–852 (1988).
Fridovich-Keil, J. L. Galactosemia: the good, the bad, and the unknown. J. Cell. Physiol. 209, 701–705 (2006).
Mumma, J. O. et al. Distinct roles of galactose-1P in galactose-mediated growth arrest of yeast deficient in galactose-1P uridylyltransferase (GALT) and UDP-galactose 4′-epimerase (GALE). Mol. Genet. Metab. 93, 160–171 (2008).
del Campo, J. et al. The others: our biased perspective of eukaryotic genomes. Trends Ecol. Evol. 29, 252–259 (2014).
Loftus, B. et al. The genome of the protist parasite Entamoeba histolytica. Nature 433, 865–868 (2005).
Brayton, K. A. et al. Genome sequence of Babesia bovis and comparative analysis of apicomplexan hemoprotozoa. PLOS Pathog. 3, 1401–1413 (2007).
Corradi, N., Pombert, J. F., Farinelli, L., Didier, E. S. & Keeling, P. J. The complete sequence of the smallest known nuclear genome from the microsporidian Encephalitozoon intestinalis. Nat. Commun. 1, 77 (2010).
Eichinger, L. et al. The genome of the social amoeba Dictyostelium discoideum. Nature 435, 43–57 (2005).
Zhu, G. et al. Cryptosporidium parvum: the first protist known to encode a putative polyketide synthase. Gene 298, 79–89 (2002).
John, U. et al. Novel insights into evolution of protistan polyketide synthases through phylogenomic analysis. Protist 159, 21–30 (2008).
Monroe, E. A., Johnson, J. G., Wang, Z. H., Pierce, R. K. & Van Dolah, F. M. Characterization and expression of nuclear-encoded polyketide synthases in the brevetoxin-producing dinoflagellate. Karenia brevis. J. Phycol. 46, 541–552 (2010).
Wang, H., Fewer, D. P., Holm, L., Rouhiainen, L. & Sivonen, K. Atlas of nonribosomal peptide and polyketide biosynthetic pathways reveals common occurrence of nonmodular enzymes. Proc. Natl Acad. Sci. USA 111, 9259–9264 (2014).
Rokas, A. & Hittinger, C. T. Transcriptional rewiring: the proof is in the eating. Curr. Biol. 17, R626–628 (2007).
Johnston, M. A model fungal gene regulatory mechanism: the GAL genes of Saccharomyces cerevisiae. Microbiol. Rev. 51, 458–476 (1987).
Rubio-Texeira, M. A comparative analysis of the GAL genetic switch between not-so-distant cousins: Saccharomyces cerevisiae versus Kluyveromyces lactis. FEMS Yeast Res. 5, 1115–1128 (2005).
Wolfe, K. H. et al. Clade- and species-specific features of genome evolution in the Saccharomycetaceae. FEMS Yeast Res. 15, fov035 (2015).
Moyrand, F., Fontaine, T. & Janbon, G. Systematic capsule gene disruption reveals the central role of galactose metabolism on Cryptococcus neoformans virulence. Mol. Microbiol. 64, 771–781 (2007).
Moyrand, F., Lafontaine, I., Fontaine, T. & Janbon, G. UGE1 and UGE2 regulate the UDP-glucose/UDP-galactose equilibrium in Cryptococcus neoformans. Eukaryot. Cell 7, 2069–2077 (2008).
Christensen, U. et al. Unique regulatory mechanism for d-galactose utilization in Aspergillus nidulans. Appl. Environ. Microbiol. 77, 7084–7087 (2011).
Boycheva, S., Daviet, L., Wolfender, J. L. & Fitzpatrick, T. B. The rise of operon-like gene clusters in plants. Trends Plant Sci. 19, 447–459 (2014).
Nutzmann, H. W., Huang, A. & Osbourn, A. Plant metabolic clusters — from genetics to genomics. New Phytol. 211, 771–789 (2016).
Frey, M. et al. Analysis of a chemical plant defense mechanism in grasses. Science 277, 696–699 (1997).
Handrick, V. et al. Biosynthesis of 8-O-methylated benzoxazinoid defense compounds in maize. Plant Cell 28, 1682–1700 (2016).
Schneider, L. M. et al. The Cer-cqu gene cluster determines three key players in a beta-diketone synthase polyketide pathway synthesizing aliphatics in epicuticular waxes. J. Exp. Bot. 67, 2715–2730 (2016).
Olsen, K. M. & Small, L. L. Micro- and macroevolutionary adaptation through repeated loss of a complete metabolic pathway. New Phytol. 219, 757–766 (2018).
Takos, A. M. et al. Genomic clustering of cyanogenic glucoside biosynthetic genes aids their identification in Lotus japonicus and suggests the repeated evolution of this chemical defence pathway. Plant J. 68, 273–286 (2011).
Winzer, T. et al. A Papaver somniferum 10-gene cluster for synthesis of the anticancer alkaloid noscapine. Science 336, 1704–1708 (2012).
Itkin, M. et al. Biosynthesis of antinutritional alkaloids in solanaceous crops is mediated by clustered genes. Science 341, 175–179 (2013).
Qi, X. et al. A gene cluster for secondary metabolism in oat: implications for the evolution of metabolic diversity in plants. Proc. Natl Acad. Sci. USA 101, 8233–8238 (2004).
Shimura, K. et al. Identification of a biosynthetic gene cluster in rice for momilactones. J. Biol. Chem. 282, 34013–34018 (2007).
Field, B. & Osbourn, A. E. Metabolic diversification — independent assembly of operon-like gene clusters in different plants. Science 320, 543–547 (2008).
Swaminathan, S., Morrone, D., Wang, Q., Fulton, D. B. & Peters, R. J. CYP76M7 is an ent-cassadiene C11alpha-hydroxylase defining a second multifunctional diterpenoid biosynthetic gene cluster in rice. Plant Cell 21, 3315–3325 (2009).
Field, B. et al. Formation of plant metabolic gene clusters within dynamic chromosomal regions. Proc. Natl Acad. Sci. USA 108, 16116–16121 (2011).
Krokida, A. et al. A metabolic gene cluster in Lotus japonicus discloses novel enzyme functions and products in triterpene biosynthesis. New Phytol. 200, 675–690 (2013).
Matsuba, Y. et al. Evolution of a complex locus for terpene biosynthesis in Solanum. Plant Cell 25, 2022–2036 (2013).
King, A. J., Brown, G. D., Gilday, A. D., Larson, T. R. & Graham, I. A. Production of bioactive diterpenoids in the Euphorbiaceae depends on evolutionarily conserved gene clusters. Plant Cell 26, 3286–3298 (2014).
Shang, Y. et al. Biosynthesis, regulation, and domestication of bitterness in cucumber. Science 346, 1084–1088 (2014).
Chu, H. Y., Wegel, E. & Osbourn, A. From hormones to secondary metabolism: the emergence of metabolic gene clusters in plants. Plant J. 66, 66–79 (2011).
Boutanaev, A. M. et al. Investigation of terpene diversification across multiple sequenced plant genomes. Proc. Natl Acad. Sci. USA 112, E81–E88 (2015).
Schlapfer, P. et al. Genome-wide prediction of metabolic enzymes, pathways, and gene clusters in plants. Plant Physiol. 173, 2041–2059 (2017).
Topfer, N., Fuchs, L. M. & Aharoni, A. The PhytoClust tool for metabolic gene clusters discovery in plant genomes. Nucleic Acids Res. 45, 7049–7063 (2017).
Kautsar, S. A., Suarez Duran, H. G., Blin, K., Osbourn, A. & Medema, M. H. plantiSMASH: automated identification, annotation and expression analysis of plant biosynthetic gene clusters. Nucleic Acids Res. 45, W55–W63 (2017).
Kliebenstein, D. J. & Osbourn, A. Making new molecules — evolution of pathways for novel metabolites in plants. Curr. Opin. Plant Biol. 15, 415–423 (2012).
Itkin, M. et al. The biosynthetic pathway of the nonsugar, high-intensity sweetener mogroside V from Siraitia grosvenorii. Proc. Natl Acad. Sci. USA 113, E7619–E7628 (2016).
Klein, A. P. & Sattely, E. S. Biosynthesis of cabbage phytoalexins from indole glucosinolate. Proc. Natl Acad. Sci. USA 114, 1910–1915 (2017).
Gladyshev, E. A., Meselson, M. & Arkhipova, I. R. Massive horizontal gene transfer in bdelloid rotifers. Science 320, 1210–1213 (2008).
Moran, N. A. & Jarvik, T. Lateral transfer of genes from fungi underlies carotenoid production in aphids. Science 328, 624–627 (2010).
Derelle, E. et al. Genome analysis of the smallest free-living eukaryote Ostreococcus tauri unveils many unique features. Proc. Natl Acad. Sci. USA 103, 11647–11652 (2006).
Fernandez, E. & Galvan, A. Inorganic nitrogen assimilation in Chlamydomonas. J. Exp. Bot. 58, 2279–2287 (2007).
McDonald, S. M., Plant, J. N. & Worden, A. Z. The mixed lineage nature of nitrogen transport and assimilation in marine eukaryotic phytoplankton: a case study of Micromonas. Mol. Biol. Evol. 27, 2268–2283 (2010).
Foflonker, F. et al. The unexpected extremophile: tolerance to fluctuating salinity in the green alga Picochlorum. Algal Res. 16, 465–472 (2016).
Vallon, O. & Spalding, M. H. in The Chlamydomonas Sourcebook Vol. 2 (ed. Stern, D.) 115–158 (Academic Press, 2009).
Foflonker, F. et al. Genome of the halotolerant green alga Picochlorum sp. reveals strategies for thriving under fluctuating environmental conditions. Environ. Microbiol. 17, 412–426 (2015).
Medema, M. H. et al. antiSMASH: rapid identification, annotation and analysis of secondary metabolite biosynthesis gene clusters in bacterial and fungal genome sequences. Nucleic Acids Res. 39, W339–W346 (2011).
Acknowledgements
The authors thank past and present members of the Rokas laboratory, particularly J. Slot, J. Gibbons, M. Mead, K. McGary and J. Steenwyk, as well as long-time collaborator C. T. Hittinger for discussions over the years on the evolution of metabolic gene clusters in fungi. Research in the Rokas laboratory has been supported by the National Science Foundation, the Searle Scholars Program, the Guggenheim Foundation, the Burroughs Wellcome Trust, the National Institutes of Health, the Beckman Scholars Program and the March of Dimes.
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Nature Reviews Microbiology thanks B. McDonald and the other anonymous reviewer(s) for their contribution to the peer review of this work.
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A.R., J.H.W. and A.L.L. wrote the article, researched data for the article, made substantial contributions to discussions of the content and reviewed and/or edited the manuscript before submission.
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Glossary
- Primary metabolism
-
The part of metabolism involving pathways associated with growth, such as those for macronutrients (for example, carbohydrates, fat and proteins).
- Secondary metabolism
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(Or specialized metabolism). The part of metabolism involving pathways associated with the production of small, bioactive molecules, such as mycotoxins, pigments and antibiotics.
- Metabolic gene clusters
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(MGCs) A set of genes from the same metabolic pathway that is physically linked and occupies the same genetic locus in the chromosome; in other organisms, similarly organized co-adapted gene complexes are associated with non-metabolic traits and have come to be known as supergenes.
- Pangenome
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The full complement of genes present in a population or species, which includes genes present in all individuals as well as genes that are present in only some individuals (or even in a single individual).
- Idiomorph alleles
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The non-homologous alleles that determine the fungal mating type of an isolate.
- Regulatory rewiring
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The same metabolic pathway (or other biological process) is regulated by different (non-homologous) transcriptional factors (and circuits) in different species.
- Horizontal gene transfer
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(HGT; also known as lateral gene transfer). The transfer of genetic material from one organism to another through a process other than reproduction.
- Convergent evolution
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The independent evolution of similar traits or features in organisms belonging to different, unrelated lineages.
- Black queen hypothesis
-
The idea that the loss of genes whose functions are associated with public goods (for example, the production of an antitoxin) may be individually advantageous (up to the point at which the cost associated with loss of public goods exceeds the benefit of loss).
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Rokas, A., Wisecaver, J.H. & Lind, A.L. The birth, evolution and death of metabolic gene clusters in fungi. Nat Rev Microbiol 16, 731–744 (2018). https://doi.org/10.1038/s41579-018-0075-3
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DOI: https://doi.org/10.1038/s41579-018-0075-3
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