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Identification of the Sfp-Type PPTase EppA from the Lichenized Fungus Evernia prunastri

  • Olivia Schimming,

    Affiliation Fachbereich Biowissenschaften, Goethe Universität Frankfurt, Max-von-Laue-Str. 9, 60438, Frankfurt am Main, Germany

  • Imke Schmitt,

    Affiliation Senckenberg Biodiversity and Climate Research Centre BiK-F, Senckenberganlage 25, 60325, Frankfurt am Main, Germany

  • Helge B. Bode

    Affiliation Fachbereich Biowissenschaften, Goethe Universität Frankfurt, Max-von-Laue-Str. 9, 60438, Frankfurt am Main, Germany

Identification of the Sfp-Type PPTase EppA from the Lichenized Fungus Evernia prunastri

  • Olivia Schimming, 
  • Imke Schmitt, 
  • Helge B. Bode


In the last decades, natural products from lichens have gained more interest for pharmaceutical application due to the broad range of their biological activity. However, isolation of the compounds of interest directly from the lichen is neither feasible nor sustainable due to slow growth of many lichens. In order to develop a pipeline for heterologous expression of lichen biosynthesis gene clusters and thus the sustainable production of their bioactive compounds we have identified and characterized the phosphopantheteinyl transferase (PPTase) EppA from the lichen Evernia prunastri. The Sfp-type PPTase EppA was functionally characterized through heterologous expression in E. coli using the production of the blue pigment indigoidine as readout and by complementation of a lys5 deletion in S. cerevisiae.


Lichen-forming fungi are symbiotic organisms forming associations with green algae, cyanobacteria, or both [1]. They synthesize a plethora of natural products, many of which possess biological activities [2]. Extracts from whole lichens showed antimicrobial, anti-inflammatory, analgesic or cytotoxic activity [36], rendering lichens interesting organisms for pharmaceutical applications [7,8]. One of the ecological functions of lichen compounds is damage prevention from sunlight [9]. Anthraquinones or xanthones act as strong ultraviolet filters, which could prove beneficial for the development of novel sunscreens protecting from harmful UVA rays [9]. The majority of natural products are synthesized by the mycobiont [10]. Still, the photobiont contributes to the natural product profile, often lichenizing fungi do not produce biological active molecules without their suitable algal partner [10].

The slow growth and the difficulty to establish pure cultures of the mycobiont hamper experimental approaches to study lichens [11]. Moreover, there exist few direct transformation systems [12],and many genes remain silent under laboratory conditions [13,14]. For this reason, heterologous expression of lichen genes in surrogate hosts is a sought-after approach [11,15]. Promising hosts could be Escherichia coli and Saccharomyces cerevisiae with established transformation systems and vectors [14,16].

While up to 1000 substances from lichens are known to date [17], only a few have been characterized in detail for their biological and therapeutic potential. Prominent representatives are the anthraquinone parietin [18] having antifungal activity [19] and the dibenzofuran usnic acid [20] showing anti-inflammatory activity in tests with rats [21]. Most of the typical lichen compounds are polyketides synthesized by polyketide synthases (PKS). However, other natural products may have gone unnoticed due to low concentrations in the lichen thallus. Especially natural products derived from non-ribosomal peptide synthetases (NRPS) have remained unexplored.

So far, all fungal and bacterial NRPS as well as type I and type II PKS characterized to date require a phosphopantetheinyl transferase (PPTase) to post-translationally attach the 4’-phosphopantetheine (Ppant) arm from CoA to the serine residue of the thiolation domain [22,23]. Three main types of PPTases are known: Sfp-type, AcpS-type, and integrated PPTases. The Sfp-type PPTase is generally regarded to be associated with secondary metabolism. Sfp-type PPTases are approximately 240 aa long and have a monomeric structure [24]. The name is derived from Sfp which is associated with the surfactin biosynthesis gene cluster and was discovered first in Bacillus subtilis [25]. By contrast, the AcpS-type is only half the size of the Sfp-type and mainly associated with fatty acid biosynthesis (FAS) [26]. However, integrated PPTases are located within the fatty acid synthases like the type I fatty acid synthase from yeast [27] and in several PKS from plants and bacteria [28].

Besides playing a part in the secondary metabolism Sfp-type PPTases can also act in the primary metabolism such as in the lysine biosynthesis or FAS if there is no AcpS-type PPTase. [28]. Moreover, due to its low substrate specificity it accepts various CoA analogs including covalently attached reporter molecules like affinity or fluorescent tags and thus can be used as a biochemical toolbox or to label specific protein tags [29,30].

Sfp-type PPTases are found across all three domains of life so that the type was additionally grouped into the subclasses F/KES and W/KEA to specify its function. Apart from PPTases involved in polyketide, glycolipid and lysine biosynthesis as well as eukaryotic PPTases, Sfp belongs to the subtype W/KEA [28].

In this work, we identified a Sfp-type PPTase EppA from the lichenizing fungus Evernia prunastri. Furthermore, we expressed eppA heterologously in E. coli and S. cerevisiae to test its functionality by indigoidine production and complementation of lys5 deletion, respectively.

Material and Methods

Strains and culture conditions

All strains are listed in S1 Table. All E. coli strains were cultivated in LB media [31]. For solid media 1.5% (w/v) agar was added. S. cerevisiae CEN.PK2-1C and derivatives were cultured in YEPD media [32]. Uracil auxotroph yeast expression strains were grown in SC media [33] with 2% (v/v) glucose (SD-ura) or galactose (SG-ura), respectively. Solid media additionally contained 2% (w/v) agar. Ampicillin (100 μg/ml), chloramphenicol (20 μg/ml), kanamycin (50 μg/ml) and G418 (200 μg/ml) were used as selection markers. All strains were cultivated at 30°C.

General molecular methods

Polymerase chain reaction (PCR) was performed using oligonucleotides obtained from Eurofins Genomics (S3 Table). Fragments with homology arms were amplified in a two-step PCR program using Phire Hot Start II DNA polymerase (Thermo Scientific) according to the manufacturers’ instructions. DNA purification was performed using MinElute PCR Purification Kit (Qiagen). Transformation of S. cerevisiae cells was done by standard LiAc transformation.

Construction of pCK_eppA

For plasmids used in this study see S2 Table. The plasmid pCK_eppA was constructed on the basis of pCK_mtaA. The identified Sfp-type PPTase gene eppA was amplified from the genomic DNA of E. prunastri using the oligonucleotides OS_ck_eppA_for/OS_ck_eppA_rev. The vector pCK was amplified from the template pCK_mtaA with the oligonucleotides OS_ck_for/OS_ck_rev. The 1007 bp PCR product of eppA contained 40 bp homology sequences to either side of the amplified vector pCK. Both fragments were cloned by Gibson assembly [34,35].

Construction of pYES260_npgA and pYES260_eppA

For the complementation of the lys5 deletion npgA and eppA were cloned into the linearized vector pYES260 by yeast homologous recombination [36]. The gene npgA which originates from Aspergillus nidulans was amplified with the oligonucleotides OS_pYnpgA_for/OS_pYnpgA_rev taking pET28a_npgA as template. The gene eppA was directly taken from the genomic DNA of E. prunastri using the oligonucleotides OS_pYeppA_for/OS_pYeppA_rev.

Deletion strain S. cerevisiae CEN.PK2-1C∆lys5

The construction of the S. cerevisiae strain CEN.PK2-1C∆lys5 was carried out by substituting lys5 for a loxP-kanMX-loxP cassette. The deletion cassette was amplified from the plasmid pUG6 [37] with the oligonucleotides OS_SClys5_for/OS_SClys5_rev. The 1666 bp large PCR product contained 40 bp homologous sites upstream as well as downstream of lys5 and was cloned into S. cerevisiae CEN.PK2-1C via yeast homologous recombination. The chromosomal deletion of lys5 had been verified by PCR with the oligonucleotides OS_SClys5_a1/ OS_SClys5_a4 binding downstream and upstream of the gene, respectively. Furthermore, oligonucleotides OS_SClys5_a2 and OS_SClys5_a3 having their binding site within lys5 as well as OS_SClys5_k2 and OS_SClys5_k3 having their binding site in the introduced marker cassette have been used in combinations with the former ones to confirm the chromosomal deletion of lys5.

Indigoidine production in E. coli DH10B and spectroscopic analysis

The functional characterization of mtaA and eppA was carried out by heterologous expression in E. coli using the blue pigment indigoidine as reporter. The NRPS gene indC responsible for the production of indigoidine is located on the plasmid pUC18_indC and co-expressed with the PPTase genes from the plasmids pCK_mtaA and pCK_eppA, respectively [38,39]. The experiment was carried out on solid and liquid media.

Indigoidine was extracted from 10 ml expression cultures containing Amberlite® XAD-16. The harvested resin was washed with water to reduce impurities and the following extractions were carried out with one volume of methanol for 30 min at room temperature. After filtration and evaporating to dryness under reduced pressure the extracts were dissolved in 1 ml DMSO and the absorbance of the biological triplicates was measured at 595 nm [40,41].

Complementation of the lys5 deletion in S. cerevisiae CEN.PK2-1C

The functional characterization of npgA and eppA was carried out by complementation of the lys5 deletion in S. cerevisiae CEN.PK2-1C as described previously [42]. The cells were transformed with the expression plasmids pYES260_npgA and pYES260_eppA, respectively. The complementation experiment was carried out on SD-ura media containing lysine and SG-ura media without lysine. Through the carbon source the gene expression of pYES260_npgA and pYES260_eppA is regulated via the inducible promoter PGAL1.

Construction of PPTase phylogeny

Amino acid sequences of PPTases (listed in S4 Table) were aligned using ClustalW before a maximum likelihood phylogeny was constructed using the PhyML feature built into Geneious (v6.1.8). Branch formation was supported by bootstrapping (n = 100).


We are interested in the heterologous production of lichen natural products as sustainable contribution to the development of novel bioactive natural products. Here our main interest focuses on compounds derived from NRPS and type I PKS. So far, all NRPS and type I PKS known to date require a PPTase that modifies their thiolation domain from the inactive apo to the active holo form [43]. The PPTase catalyzes the covalent attachment of the Ppant arm obtained from CoA to the serine residue of the thiolation domain. The identification of the first PPTase from a lichen-forming fungus was managed through BLAST search of the genomic DNA from E. prunastri (unpublished data) against other PPTases. For the in silico search in the genome we have chosen EntD from E. coli [44], Lys5 from S. cerevisiae [45], meAcpS from Micromonaspora echinospora spp. [46], AcpS as well as Sfp from B. subtilis [25,47] and NpgA from A. nidulans [48]. Both, Sfp and NpgA, provided the same result and led to a gene with a length of 927 bp. All other sequences resulted in no hit.

Due to the organism and its purpose we named the gene eppA (Evernia prunastri PPTase A; Genbank accession number: KT369532). On the basis of the BLAST search and the amino acid sequence (Fig 1), EppA could be grouped into the Sfp-type PPTases next to other Sfp-like PPTases from different fungi (Fig 2). Furthermore, the alignment of EppA, NpgA and Sfp led to the subclassification W/KEA (Fig 1). Apparently, EppA is the only PPTase encoded in the genome of E. prunastri mycobiont. Since there is no direct genetic manipulation method to test its function in the original host we chose E. coli as surrogate host. Therefore, we amplified eppA with homologous arms and cloned it into the linearized vector fragment pCK. The resultant plasmid pCK_eppA was co-expressed with pUC18_indC. The vector pUC18_indC carries the gene indC encoding the NRPS IndC. IndC is responsible for the cyclization and oxidation of glutamine that with air forms the blue pigment indigoidine [49]. Since the production is visual to the naked eye indigoidine is a suitable reporter for NRPS and PPTase function. The co-expression of pUC18_indC with pACYC_tacI/I (negative control), pCK_mtaA (positive control) and pCK_eppA resulted in the formation of blue cells for the last two constructs although cells containing mtaA are apparently not as much pigmented as cells expressing eppA (Fig 3). The PPTase encoding gene mtaA from the myxobacterium Stigmatella aurantiaca [50] was used as a positive control as it had been described to function in IndC activation [38]. The spectroscopic analysis revealed an indigoidine production of 54.8±0.6 mg/L/OD595nm and 64.8±0.3 mg/L/OD595nm for samples containing MtaA and EppA, respectively.

Fig 1. Amino acid sequence and alignment of EppA.

Amino acid sequence of EppA (A) and partial sequence alignment of EppA from E. prunastri, NpgA from A. nidulans and Sfp from B. subtilis starting at amino acid 49 (counting from Sfp) showing motif 1–3 (M1-M3) as well as the W/KEA motif (grey box) and the corresponding conserved residues for Sfp (marked in black) (B).

Fig 2. Phylogenetic tree of Sfp- and AcpS-type PPTases from different organisms.

EppA (framed in red) is grouped in the Sfp-type next to PPTases from fungi and Bacillus subtilis. For accession numbers of sequences used see S4 Table.

Fig 3. Indigoidine production assay in E. coli DH10B on solid and in liquid media.

The co-expression of pUC18_indC and pACYC_tacI/I (empty vector), pCK_mtaA (mtaA) or pCK_eppA (eppA), respectively, led to blue cells for the co-expressed PPTase genes mtaA and eppA.

Encouraged by the functional production of EppA in E. coli its function was also tested in S. cerevisiae using a complementation test procedure according to Mootz et al. (2002) [42]. The PPTase Lys5 from S. cerevisiae is involved in the lysine biosynthesis as the enzymatic reduction of α-aminoadipate to α-aminoadipate semialdehyde takes place while the substrate is bound at the Ppant arm of the α-aminoadipate reductase Lys2. Thus the deletion of lys5 results in lysine auxotrophic yeast strain that can only survive with lysine in the medium or a complementing PPTase expressed in the cell.

The S. cerevisiae CEN.PK2-1C∆lys5 strain was constructed by inserting a loxP-kanMX-loxP gene disruption cassette into lys5. Furthermore, eppA and npgA from Aspergillus nidulans were cloned into the expression vector pYES260, respectively. This shuttle vector carries a galactose inducible promoter PGAL1 which is non-induced on glucose and induced on galactose. Accordingly, yeast cells should grow independently from a complementation on SD-ura plates with added lysine. In contrast, only cells carrying a functional PPTase can grow on SG-ura plates without lysine. The complementation assay was carried out on solid media with CEN.PK2-1C∆lys5 and the corresponding expression plasmids pYES260 (negative control), pYES260_npgA (positive control) or pYES260_eppA, respectively. For the empty vector no growth could be monitored. However, cell growth could be observed for the complementation with EppA and NpgA (Fig 4).

Fig 4. Complementation assay in S. cerevisiae CEN.PK2-1C∆lys5 by heterologously expressed PPTase encoding genes.

Constructs pYES260 (-), pYES260_npgA (npgA) and pYES260_eppA (eppA) were tested for complementation of the lys5 deletion on SD-ura media with supplementation of lysine (SD-ura + lys) and on SG-ura media without lysine (SG-ura–lys).

Thus, the function of the newly identified PPTase EppA from E. prunastri could be confirmed through heterologous expression in E. coli and S. cerevisiae.


Natural products from lichens have gained immense interest due to their broad range of biological activity [7,8]. From in silico analyses of the lichen genomes [12,5154] it is obvious that lichens harbor a yet underestimated number of PKS and NRPS encoding genes as it is also the case for fungal and bacterial natural product producers [55]. As all NRPS and type I PKS known up to date require a PPTase for activity, we initially focused on the identification of a PPTase from the lichen E. prunastri as model system that is also known as oakmoss.

The six selected PPTases used as BLAST query covered all types of known PPTases. Yet, only EppA could be identified as member of the Sfp-type PPTases related to similar PPTases from other fungi. Organisms with sole PPTases are quite common and often show a broad substrate tolerance activating several different acyl and peptidyl carrier proteins. For example PcpS from Pseudomonas aeruginosa can act in both primary and secondary metabolism [56].

Indigoidine production is an ideal reporter system for PPTase activity as it is highly sensitive [57]. Only a small amount of PPTase is required compared to the amount of NRPS to give the blue pigment [58]. It might be possible that the higher indigoidine production of samples containing EppA is due to a lower amount of EppA resulting from a suboptimal translation from a difference in codon usage. For the complementation of the lys5 deletion in S. cerevisiae, yeast cell growth could be shown for the positive control NpgA and the lichen PPTase EppA. Mootz and co-workers already functionally characterized two fungal genes from Schizosaccharomyces pombe with this method [42]. There is no background activity–the cells either grow when complemented or not, making it a powerful tool for screening of novel PPTases from different origins [42].

Since there are no transformation methods for lichen available, the only possibility to investigate these genes is the heterologous expression in surrogate hosts like E. coli, S. cerevisiae or Aspergillus [14,16,59]. The expression in Aspergillus has the advantage that it might work independently from cDNA or the knowledge of intron/exon boundaries since the organism is able to splice introns [59]. However, E. coli and S. cerevisiae have the benefit that they are well established and a broad set of expression plasmids with different promoters and selection markers already exist [14].

So far, there are only few reports of heterologous expression of genes from lichenizing fungi [11,18]. Testing PPTases has the advantage that already poor expression is sufficient to show a product formation whereas for NRPS production and product screening much higher production of proteins is required. Up to date, NRPS production in S. cerevisiae could be shown successfully for the fungal cluster pcbAB from Penicillium chrysogenum by Siewers et al. (2009) involved in the production of the antibiotic precursor δ-(L-α.aminoadipyl)-L-cysteinyl-D-valine [60]. Regarding lichen genes most progress had been made by investigation of a PKS gene from Cladonia grayi which was heterologously expressed in A. nidulans. Two introns were successfully spliced out and RT-PCR analysis revealed the transcription of the gene under the native promoter [61].

In conclusion, a start has been made by the expression of PKS and NRPS encoding genes from lichen and the identification of the PPTase EppA but it is still a long way to produce lichen natural products in heterologous hosts.

Supporting Information

S1 Table. Strains used in this study.


S2 Table. Plasmids used in this study.


S3 Table. Oligonucleotides used in this study.


S4 Table. Name and accession number of the protein sequences used in the phylogenetic tree.



This work was supported by the Hessian Ministry of Science and Art via the LOEWE research focus “Integrative fungal research (IPF)”. The authors thank Eckhard Boles for useful discussions regarding all aspects of yeast molecular biology, and Anjuli Meiser, Francesco Dal Grande and Jürgen Otte for providing the draft genome of E. prunastri.

Author Contributions

Conceived and designed the experiments: OS HBB. Performed the experiments: OS. Analyzed the data: OS. Contributed reagents/materials/analysis tools: OS IS. Wrote the paper: OS IS HBB.


  1. 1. Ahmadjian V. The lichen symbiosis. New York: John Wiley; 1993.
  2. 2. Boustie J, Grube M. Lichens—a promising source of bioactive secondary metabolites. issn: 1479–2621. 2005; 3: 273–287.
  3. 3. Burkholder PR, Evans AW, McVeigh I, Thornton HK. Antibiotic Activity of Lichens. Proc. Natl. Acad. Sci. U.S.A. 1944; 30: 250–255. pmid:16588653
  4. 4. Emmerich R, Giez I, Lange OL, Proksch P. Toxicity and antifeedant activity of lichen compounds against the polyphagous herbivorous insect Spodoptera littoralis. Phytochemistry. 1993; 33: 1389–1394.
  5. 5. Gollapudi SR, Telikepalli H, Jampani HB, Mirhom YW, Drake SD, Bhattiprolu KR, et al. Alectosarmentin, a new antimicrobial dibenzofuranoid lactol from the lichen, Alectoria sarmentosa. J. Nat. Prod. 1994; 57: 934–938. pmid:7964789
  6. 6. Lauterwein M, Oethinger M, Belsner K, Peters T, Marre R. In vitro activities of the lichen secondary metabolites vulpinic acid, (+)-usnic acid, and (-)-usnic acid against aerobic and anaerobic microorganisms. Antimicrob. Agents Chemother. 1995; 39: 2541–2543. pmid:8585741
  7. 7. Huneck S. The significance of lichens and their metabolites. Naturwissenschaften. 1999; 86: 559–570. pmid:10643590
  8. 8. Müller K. Pharmaceutically relevant metabolites from lichens. Appl. Microbiol. Biotechnol. 2001; 56: 9–16. pmid:11499952
  9. 9. Nguyen K, Chollet-Krugler M, Gouault N, Tomasi S. UV-protectant metabolites from lichens and their symbiotic partners. Nat Prod Rep. 2013; 30: 1490–1508. pmid:24170172
  10. 10. Culberson CF, Armaleo D. Induction of a complete secondary-product pathway in a cultured lichen fungus. Experimental Mycology. 1992; 16: 52–63.
  11. 11. Gagunashvili AN, Davídsson SP, Jónsson ZO, Andrésson OS. Cloning and heterologous transcription of a polyketide synthase gene from the lichen Solorina crocea. Mycol. Res. 2009; 113: 354–363. pmid:19100326
  12. 12. Park S, Choi J, Lee G, Jeong M, Kim JA, Oh S, et al. Draft Genome Sequence of Umbilicaria muehlenbergii KoLRILF000956, a Lichen-Forming Fungus Amenable to Genetic Manipulation. Genome Announc. 2014; 2.
  13. 13. Hamada N, Miyagawa H, Miyawaki H, Inoue M. Lichen Substances in Mycobionts of Crustose Lichens Cultured on Media with Extra Sucrose. The Bryologist. 1996; 99: 71.
  14. 14. Stocker-Wörgötter E. Metabolic diversity of lichen-forming ascomycetous fungi: culturing, polyketide and shikimate metabolite production, and PKS genes. Nat Prod Rep. 2008; 25: 188–200. pmid:18250902
  15. 15. Sinnemann SJ, Andrésson OS, Brown DW, Miao VP. Cloning and heterologous expression of Solorina crocea pyrG. Curr. Genet. 2000; 37: 333–338. pmid:10853771
  16. 16. Kealey JT, Liu L, Santi DV, Betlach MC, Barr PJ. Production of a polyketide natural product in nonpolyketide-producing prokaryotic and eukaryotic hosts. Proc. Natl. Acad. Sci. U.S.A. 1998; 95: 505–509. pmid:9435221
  17. 17. Muggia L, Imke I, Grube M. Lichens as treasure chest of natural products. SIM News. 2009: 85–97.
  18. 18. Solhaug KA, Gauslaa Y. Parietin, a photoprotective secondary product of the lichen Xanthoria parietina. Oecologia. 1996; 108: 412–418.
  19. 19. Basile A, Rigano D, Loppi S, Di Santi A, Nebbioso A, Sorbo S, et al. Antiproliferative, antibacterial and antifungal activity of the lichen Xanthoria parietina and its secondary metabolite parietin. Int J Mol Sci. 2015; 16: 7861–7875. pmid:25860944
  20. 20. Knop W. Chemisch-physiologische Untersuchung über die Flechten. Ann. Chem. Pharm. 1844; 49: 103–124.
  21. 21. Vijayakumar CS, Viswanathan S, Reddy MK, Parvathavarthini S, Kundu AB, Sukumar E. Anti-inflammatory activity of (+)-usnic acid. Fitoterapia. 2000; 71: 564–566. pmid:11449509
  22. 22. Stack D, Neville C, Doyle S. Nonribosomal peptide synthesis in Aspergillus fumigatus and other fungi. Microbiology (Reading, Engl.). 2007; 153: 1297–1306.
  23. 23. Walsh CT, Gehring AM, Weinreb PH, Quadri LE, Flugel RS. Post-translational modification of polyketide and nonribosomal peptide synthases. Curr Opin Chem Biol. 1997; 1: 309–315. pmid:9667867
  24. 24. Mofid MR, Finking R, Essen LO, Marahiel MA. Structure-based mutational analysis of the 4'-phosphopantetheinyl transferases Sfp from Bacillus subtilis: carrier protein recognition and reaction mechanism. Biochemistry. 2004; 43: 4128–4136. pmid:15065855
  25. 25. Mootz HD, Finking R, Marahiel MA. 4'-phosphopantetheine transfer in primary and secondary metabolism of Bacillus subtilis. J. Biol. Chem. 2001; 276: 37289–37298. pmid:11489886
  26. 26. Beld J, Sonnenschein EC, Vickery CR, Noel JP, Burkart MD. The phosphopantetheinyl transferases: catalysis of a post-translational modification crucial for life. Nat Prod Rep. 2014; 31: 61–108. pmid:24292120
  27. 27. Fichtlscherer F, Wellein C, Mittag M, Schweizer E. A novel function of yeast fatty acid synthase. Subunit alpha is capable of self-pantetheinylation. Eur. J. Biochem. 2000; 267: 2666–2671. pmid:10785388
  28. 28. Copp JN, Neilan BA. The phosphopantetheinyl transferase superfamily: phylogenetic analysis and functional implications in cyanobacteria. Appl. Environ. Microbiol. 2006; 72: 2298–2305. pmid:16597923
  29. 29. Clair La, James J, Foley TL, Schegg TR Regan CM, Burkart MD. Manipulation of carrier proteins in antibiotic biosynthesis. Chem. Biol. 2004; 11: 195–201. pmid:15123281
  30. 30. Clarke KM, Mercer AC, La Clair, James J, Burkart MD. In vivo reporter labeling of proteins via metabolic delivery of coenzyme A analogues. J. Am. Chem. Soc. 2005; 127: 11234–11235. pmid:16089439
  31. 31. LB (Luria-Bertani) liquid medium. Cold Spring Harbor Protocols. 2006; 2006: pdb.rec8141.
  32. 32. Yeast extract-peptone-dextrose growth medium (YEPD). Cold Spring Harbor Protocols. 2010; 2010: pdb.rec12161.
  33. 33. Complete Minimal (CM) or Synthetic Complete (SC) and Drop-out Media. Cold Spring Harbor Protocols. 2006; 2006: pdb.rec8190.
  34. 34. Gibson D. One-step enzymatic assembly of DNA molecules up to several hundred kilobases in size. Protocol Exchange. 2009.
  35. 35. Gibson DG, Young L, Chuang R, Venter JC, Hutchison CA, Smith HO. Enzymatic assembly of DNA molecules up to several hundred kilobases. Nat. Methods. 2009; 6: 343–345. pmid:19363495
  36. 36. Schimming O, Fleischhacker F, Nollmann FI, Bode HB. Yeast homologous recombination cloning leading to the novel peptides ambactin and xenolindicin. Chembiochem. 2014; 15: 1290–1294. pmid:24816640
  37. 37. Güldener U, Heck S, Fielder T, Beinhauer J, Hegemann JH. A new efficient gene disruption cassette for repeated use in budding yeast. Nucleic Acids Res. 1996; 24: 2519–2524. pmid:8692690
  38. 38. Brachmann AO, Kirchner F, Kegler C, Kinski SC, Schmitt I, Bode HB. Triggering the production of the cryptic blue pigment indigoidine from Photorhabdus luminescens. J. Biotechnol. 2012; 157: 96–99. pmid:22085970
  39. 39. Kegler C, Nollmann FI, Ahrendt T, Fleischhacker F, Bode E, Bode HB. Rapid determination of the amino acid configuration of xenotetrapeptide. Chembiochem. 2014; 15: 826–828. pmid:24616055
  40. 40. Myers JA, Curtis BS, Curtis WR. Improving accuracy of cell and chromophore concentration measurements using optical density. BMC Biophys. 2013; 6: 4. pmid:24499615
  41. 41. Müller M, Ausländer S, Ausländer D, Kemmer C, Fussenegger M. A novel reporter system for bacterial and mammalian cells based on the non-ribosomal peptide indigoidine. Metab. Eng. 2012; 14: 325–335. pmid:22543310
  42. 42. Mootz HD, Schörgendorfer K, Marahiel MA. Functional characterization of 4'-phosphopantetheinyl transferase genes of bacterial and fungal origin by complementation of Saccharomyces cerevisiae lys5. FEMS Microbiol. Lett. 2002; 213: 51–57. pmid:12127488
  43. 43. Schwarzer D, Finking R, Marahiel MA. Nonribosomal peptides: from genes to products. Nat Prod Rep. 2003; 20: 275–287. pmid:12828367
  44. 44. Lambalot RH, Gehring AM, Flugel RS, Zuber P, LaCelle M, Marahiel MA, et al. A new enzyme superfamily—the phosphopantetheinyl transferases. Chem. Biol. 1996; 3: 923–936. pmid:8939709
  45. 45. Borell CW, Bhattacharjee JK. Cloning and biochemical characterization of LYS5 gene of Saccharomyces cerevisiae. Curr. Genet. 1988; 13: 299–304. pmid:2839304
  46. 46. Murugan E, Liang Z. Evidence for a novel phosphopantetheinyl transferase domain in the polyketide synthase for enediyne biosynthesis. FEBS Lett. 2008; 582: 1097–1103. pmid:18319060
  47. 47. Quadri LE, Weinreb PH, Lei M, Nakano MM, Zuber P, Walsh CT. Characterization of Sfp, a Bacillus subtilis phosphopantetheinyl transferase for peptidyl carrier protein domains in peptide synthetases. Biochemistry. 1998; 37: 1585–1595. pmid:9484229
  48. 48. Keszenman-Pereyra D, Lawrence S, Twfieg M, Price J, Turner G. The npgA/ cfwA gene encodes a putative 4'-phosphopantetheinyl transferase which is essential for penicillin biosynthesis in Aspergillus nidulans. Curr. Genet. 2003; 43: 186–190. pmid:12664133
  49. 49. Reverchon S, Rouanet C, Expert D, Nasser W. Characterization of indigoidine biosynthetic genes in Erwinia chrysanthemi and role of this blue pigment in pathogenicity. J. Bacteriol. 2002; 184: 654–665. pmid:11790734
  50. 50. Gaitatzis N, Hans A, Müller R, Beyer S. The mtaA gene of the myxothiazol biosynthetic gene cluster from Stigmatella aurantiaca DW4/3-1 encodes a phosphopantetheinyl transferase that activates polyketide synthases and polypeptide synthetases. J. Biochem. 2001; 129: 119–124. pmid:11134965
  51. 51. Park S, Choi J, Kim JA, Yu N, Kim S, Kondratyuk SY, et al. Draft Genome Sequence of Lichen-Forming Fungus Caloplaca flavorubescens Strain KoLRI002931. Genome Announc. 2013; 1.
  52. 52. Park S, Choi J, Kim JA, Jeong M, Kim S, Lee Y, et al. Draft Genome Sequence of Cladonia macilenta KoLRI003786, a Lichen-Forming Fungus Producing Biruloquinone. Genome Announc. 2013; 1.
  53. 53. Park S, Choi J, Lee G, Kim JA, Oh S, Jeong M, et al. Draft Genome Sequence of Lichen-Forming Fungus Cladonia metacorallifera Strain KoLRI002260. Genome Announc. 2014; 2.
  54. 54. Wang Y, Liu B, Zhang X, Zhou Q, Zhang T, Li H, et al. Genome characteristics reveal the impact of lichenization on lichen-forming fungus Endocarpon pusillum Hedwig (Verrucariales, Ascomycota). BMC Genomics. 2014; 15: 34. pmid:24438332
  55. 55. Bode HB, Müller R. The impact of bacterial genomics on natural product research. Angew. Chem. Int. Ed. Engl. 2005; 44: 6828–6846. pmid:16249991
  56. 56. Finking R, Solsbacher J, Konz D, Schobert M, Schafer A, Jahn D, et al. Characterization of a new type of phosphopantetheinyl transferase for fatty acid and siderophore synthesis in Pseudomonas aeruginosa. J. Biol. Chem. 2002; 277: 50293–50302. pmid:12381736
  57. 57. Yu D, Xu F, Valiente J, Wang S, Zhan J. An indigoidine biosynthetic gene cluster from Streptomyces chromofuscus ATCC 49982 contains an unusual IndB homologue. J. Ind. Microbiol. Biotechnol. 2013; 40: 159–168. pmid:23053349
  58. 58. Müller M, Ausländer S, Ausländer D, Kemmer C, Fussenegger M. A novel reporter system for bacterial and mammalian cells based on the non-ribosomal peptide indigoidine. Metab. Eng. 2012; 14: 325–335. pmid:22543310
  59. 59. Pfeifer BA, Khosla C. Biosynthesis of polyketides in heterologous hosts. Microbiol. Mol. Biol. Rev. 2001; 65: 106–118. pmid:11238987
  60. 60. Siewers V, Chen X, Le Huang, Zhang J, Nielsen J. Heterologous production of non-ribosomal peptide LLD-ACV in Saccharomyces cerevisiae. Metab. Eng. 2009; 11: 391–397. pmid:19686863
  61. 61. Miao V. Genetic approaches to harvesting lichen products. Trends in Biotechnology. 2001; 19: 349–355. pmid:11513998