4Institute of Food Chemistry and Food Biotechnology, Justus Liebig University Giessen, Giessen, Germany
5Fraunhofer Institute for Molecular Biology and Applied Ecology IME Business Area Bioresources, Heinrich-Buff-Ring 17, 35392 Giessen, Germany
Guest Editor: J. S. Dickschat
Beilstein J. Org. Chem. 2019, 15, 1000–1007. https://doi.org/10.3762/bjoc.15.98
Received 19 Feb 2019, Accepted 18 Apr 2019, Published 30 Apr 2019
The strophariaceous basidiomycete Cyclocybe aegerita (synonyms Agrocybe aegerita and A. cylindracea) is one of the most praised cultivated edible mushrooms and is being cultivated at large scale for food production. Furthermore, the fungus serves as a model organism to study fruiting body formation and the production of secondary metabolites during the life cycle of Basidiomycota. By studying the secondary metabolite profiles of C. aegerita, we found several terpenoids in submerged cultures. Aside from the main metabolite, bovistol (1), two new bovistol derivatives B and C (2, 3) and pasteurestin C as a new protoilludane (4) were isolated by preparative HPLC. Their structures were elucidated by mass spectrometry and NMR spectroscopy. The relative configurations of 2–4 were assigned by ROESY correlations, and 3JH,H coupling constants in the case of 4. Applying quantitative PCR for gene expression validation, we linked the production of bovistol and its derivatives to the respective biosynthesis gene clusters.
Keywords: bioinformatics; gene cluster analysis; natural products; secondary metabolites; structure elucidation; terpenes
The basidiomycete Agrocybe aegerita (synonym: A. cylindracea) was traditionally accommodated in the genus Agrocybe (family Bolbitiaceae) until a recent phylogenetic study based on comparisons of rDNA sequence data has resulted in its placement in the Strophariaceae family and it was accordingly moved into the resurrected genus Cyclocybe Velenovsky [1,2]. The original publication by Vizzini et al.  was published in a regional journal, rather than in one of the leading peer-reviewed taxonomic journals, and the authors did not follow good scientific practice for typification when proposing these taxonomic changes. However, they subsequently published their entries in Index Fungorum, making them valid according to the current nomenclature rules, and the phylogenetic tree they presented clearly revealed that the species now accommodated in the genus Cyclocybe are more closely related to the Strophariaceae and phylogenetically rather distinct from those of the family Bolbitiaceae, including the type species of Agrocybe which is A. praecox. Therefore, the currently valid scientific name of the fungus is Cyclocybe aegerita (V. Brig.) Vizzini.
In fact, C. aegerita is a rather important fungal species with regard to practical applications, as i) it belongs to the edible mushrooms that are being cultivated at industrial scale and it is highly esteemed for its excellent aroma and ii) it has been used as a model organism for microbiological and genetic investigations on fruiting body formation for many years. Herzog et al.  have recently reported a parental dikaryotic strain C. aegerita AAE-3 that completes its life cycle on agar plates in only three weeks, along with a set of sibling monokaryons derived from it. Among these monokaryons, C. aegerita AAE-3-32 has been used for histological analysis of monokaryotic fruiting sensu stricto (mushroom formation without previous mating) and, together with C. aegerita AAE-3-13, for exploring molecular tools for transformation and gene of interest expression, which has just been published . These strains could serve well for studies exploring the factors regulating monokaryotic fruiting in comparison to dikaryotic mushroom formation. In addition, strains of this fungal species show a reliable growth behaviour in liquid culture and could eventually serve as hosts for heterologous production of secondary metabolites derived from other Basidiomycota that are more difficult or even impossible to culture. With these goals in mind, we have initiated extensive studies of the secondary metabolism of the aforementioned strains, targeting both volatile and non-volatile compounds. The present paper will describe the discovery of one known and three new non-volatile terpenoids (Figure 1) that were isolated from liquid cultures of C. aegerita and their physicochemical and preliminary biological characterisation.
Both the ethyl acetate extract of the culture filtrate and the acetone extract of the mycelium of C. aegerita, grown in ZM/2 medium, contained a major metabolite with a molecular mass of 496 Da, as detected by HPLC–MS analysis. Its molecular formula C30H40O6 was deduced from its [M + Na]+ peak at m/z 519.2718 in the HRESIMS spectrum. 1H and 1H,13C-HSQC NMR data (Table 1) indicated the presence of four methyls and twelve methylenes, three of them oxomethylene groups. A database search with this data within the Chapman & Hall Dictionary of Natural Products on DVD suggested its identity as bovistol, which was confirmed by the elucidation of the structure by COSY and HMBC NMR data .
Table 1: NMR shifts (1H 700 MHz, 13C 175 MHz) of bovistol A–C (1–3) in chloroform-d.
|Atom#||13C, mult.||1H, mult. (J, Hz)||13C, mult.||1H, mult. (J, Hz)||13C, mult.||1H, mult. (J, Hz)|
|1||38.8, CH2||2.45, d (15.4)/2.40, d (15.4)||40.0, CH2||2.32, m/2.70, m||43.3, CH2||2.75, dt (18.1, 2.0)/2.43, br d (18.1)|
|2||135.4, C||156.0, C||161.1, C|
|3||130.7, C||143.6, C||75.4, C|
|4||7.5, CH2||1.26, m/0.64, ddd (9.8, 5.9, 5.7)||5.2, CH2||1.05, m/0.87, m||4.0, CH2||1.11, ddd (9.3, 6.7, 4.8)/0.30, ddd (9.3, 6.6, 4.8)|
|5||8.6, CH2||0.89, dt (10.0, 5.7)/0.79, dt (10.0, 5.9)||13.1, CH2||1.46, m/0.29, m||5.7, CH2||0.88, m|
|6||32.4, C||30.9, C||30.0, C|
|7||80.9, C||79.3, C||79.7, C|
|8||207.6, C||196.7, C||197.2, C|
|9||80.8, C||134.2, C||134.2, C|
|10||44.9, CH2||1.94, d (14.2)/1.48, d (14.2)||43.1, CH2||2.75, m/2.55, m||39.5, CH2||2.58, dt (16.8, 2.0)/2.24, br d (16.8)|
|11||41.2, C||42.8, C||42.5, C|
|12||15.1, CH3||1.50, s||112.3, CH2||5.16, s/5.11, s||18.5, CH3||1.164, s|
|13||27.7, CH2||2.84, m/1.72, td (13.0, 5.8)||29.2, CH2||2.21, m/1.89, td (13.5, 5.0)||28.5, CH2||2.78, m/1.72, td (13.5, 5.0)|
|14||71.6, CH2||3.26, s||70.3, CH2||3.49, s||70.4, CH2||3.48, s|
|15||26.4, CH3||1.26, s||24.8, CH3||1.20, s||24.7, CH3||1.160, s|
|1’||43.0, CH2||2.86, d (16.0)/2.61, d (16.0)||42.8, CH2||2.86, m/2.60, m||42.8, CH2||2.84, d (16.0)/2.59, d (16.0)|
|2’||141.6, C||141.4, C||141.1, C|
|3’||124.5, C||124.2, C||124.1, C|
|4’||61.7, CH2||3.69, m||62.0, CH2||3.70, br t (6.8)||62.1, CH2||3.71, m|
|5’||31.9, CH2||2.83, m||32.2, CH2||2.86, m||32.1, CH2||2.88, m|
|6’||133.0, C||132.4, C||132.2, C|
|7’||118.6, C||118.4, C||119.1, C|
|8’||148.5, C||149.2, C||149.1, C|
|9’||127.2, C||126.8, C||126.6, C|
|10’||39.4, CH2||2.94, d (16.4)/2.55, d (16.4)||39.6, CH2||2.86, m/2.52, m||39.6, CH2||2.83, d (16.5)/2.51, d (16.5)|
|11’||43.8, C||43.9, C||43.9, C|
|12’||15.6, CH3||2.12, s||15.5, CH3||2.14, s||15.5, CH3||2.14, s|
|13’||21.2, CH2||2.72, m||20.1, CH2||2.40, m||19.9, CH2||2.78, m/2.40, m|
|14’||71.3, CH2||3.50, s||71.2, CH2||3.51, s||71.2, CH2||3.51, s|
|15’||25.1, CH3||1.19, s||24.9, CH3||1.21, s||24.9, CH3||1.20, s|
|3OMe||50.5, CH3||3.33, s|
In the course of the isolation of 1 the minor metabolites 2 and 3 accrued. Metabolite 2 was analysed for a molecular weight of 478 Da. Its molecular formula C30H38O5, deduced from HRESIMS data, indicated the formal loss of one molecule of water. 1H and HSQC NMR data (Table 1) of 2 were very similar to those of 1, with the exception of the replacement of methyl CH3-12 by an exomethylene group. HMBC correlations from both exo-methylene protons 12-H2 to C-2, C-3, C-4, in addition to those from both 1-H2 and 10-H2 to the olefinic carbons C-2 and C-9, confirmed the structure of 2 (Figure 1). For 3, HRESIMS data revealed its molecular formula as C31H42O6. The 1H and 13C NMR data (Table 1) were highly similar to those of 1, with the key difference being an additional methoxy group (δH 3.33/δC 50.5). This methoxy was connected to C-3 due to its HMBC correlation to this carbon atom, along to the ones from 1-H2, 10-H2 and 12-H3 to C-3. Compared to 1, the Δ2,3 double bond is shifted to Δ2,9, explaining the high field shift of the conjugated ketone C-8 (δC 197.2). A ROESY correlation between 3-OCH3 and 13-Ha revealed a 3S configuration. The closest known structural relative of 3 is the 3-demethoxy-3-hydroxy derivative of 3, which has been described as a spontaneous dimerization product of psathyrellon B .
In addition to disesquiterpenoids 1–3, metabolite 4 with a molecular mass of 250 Da was isolated. 1H and 1H,13C-HSQC NMR data (Table 2) revealed the presence of three methyls, four methylenes and three methines, one of them oxygenated. The 13C NMR spectrum indicated furthermore a carboxylic acid in addition to two olefinic and two aliphatic carbons devoid bound protons. A large spin system comprising 1-H2/2-H/9-H(10-H2)/8-H was constructed by COSY and TOCSY correlations in addition to the small one of 4-H2/5-H2. These spin systems were connected by HMBC correlations to form the protoilludane skeleton, mainly to note the correlations from 14-H3 and 15-H3 to 1-H2/10-H2, 12-H3 to C-2/C-3/C-4/C-6, 5-H2 to C-6/C-7 and 8-H to C-6/C-7/C-13. The strong ROESY correlation between 2-H and 9-H indicated a cis configuration between these protons, and the large coupling constant between 8-H and 9-H, observed in the signal of 8-H, a trans configuration of 8-H/9-H. Finally, the ROESY correlation between 12-H3 and 1-Hb indicated methyl C-12 being on the opposite site of the molecular plane as 2-H and 9-H. This assignment was confirmed by the comparison of the 13C NMR shifts to pasteurestin A and B [6,7]. Since the absolute stereochemistry has been demonstrated for pasteurestins A and B by total synthesis, we tentatively conclude a 2S,3R,8S,9R absolute configuration for pasteurestin C (4). The systematic name for 4 is (4S,4aR,7aS,7bR)-4-hydroxy-6,6,7b-trimethyl-2,4,4a,5,6,7,7a,7b-octahydro-1H-cyclobuta[e]indene-3-carboxylic acid.
Table 2: NMR data (1H 700 MHz, 13C 175 MHz) of compound 4 in acetone-d6.
|Atom#||C Shift||H Shift||COSY||HMBC|
|1||41.6, CH2||1.44, m||1, 2||14, 11, 10, 9|
|1.39, m||1, 2||14, 15, 11, 2, 3|
|2||45.9, CH||2.43, m||1, 1||9, 12, 4, 3, 9, 8|
|4||36.4, CH2||1.95, m||5, 5||12, 5, 2, 3, 7, 6|
|5||29.9, CH2||3.13, m||4, 5, 8||4, 3, 7, 6|
|3.02, m||4, 5||3, 7, 6|
|8||72.3, CH||4.27, dt (8.0, 2.0)||9, 5||10, 7, 13, 6|
|9||50.9, CH||2.40, m||10, 10, 8||2, 3, 8|
|10||47.4, CH2||1.12, m||10, 9||14, 15, 11, 9, 8|
|1.793, br dd (11.2, 7.5)||10, 9||14, 1, 2|
|12||20.3, CH3||1.14, m||4, 2, 3, 6|
|14||27.4, CH3||0.96, s||15, 11, 1, 10|
|15||29.8, CH3||1.09, m||14, 11, 1, 10|
Bovistol A (1) showed weak cytotoxic effects (IC50 for L929 = 15 µg/mL, for KB3.1 = 7 µg/mL), but was inactive against all test organisms in our standard test panel, comprising selected Gram-positive and Gram-negative bacteria as well as fungi . Compound 4 was inactive in all assays of our test panel, and 3 could not be tested due to the insufficient amount isolated.
Our finding of the production of 1–4 by C. aegerita expands the number of secondary metabolites known from this fungus. From fungal cultures of the genus Cyclocybe the production of a broad variety of metabolites is known. This includes polyacetylenes [9,10] as well as sesquiterpenoids with illudine , aromadendrane , marasmene  and fomannosane  type skeletons. Although bovistol could formally be supposed to be a triterpene, it is thought to be derived by a hetero-Diels–Alder reaction of two sesquiterpenes to form a dimeric sesquiterpenoid .
In the recently published genome of C. aegerita , two putative sesquiterpene synthase gene clusters have been identified on the basis of the published Δ6-protoilludene gene cluster of Omphalotus olearius . The protein sequences of the genes clustering adjacent to the putative sesquiterpene synthase genes going by the gene IDs AAE3_04120 and AAE3_10454 (http://www.thines-lab.senckenberg.de/agrocybe_genome) reveal the presence of P450 monooxygenases, oxidoreductases as well as one putative Diels-Alderase 1 kb downstream of the putative Δ6-protoilludene synthase gene going by the gene ID AAE3_04120. To determine the correspondence between both putative sesquiterpene synthases and the analysed secondary metabolites 1–4 C. aegerita AAE-3 was cultivated in a stirred vessel bioreactor. Mycelial samples were analysed for the presence of the gene transcripts and 1 and 3 (Figure 2). At the beginning of the fermentation, the putative sesquiterpene synthase gene with the gene ID AAE3_04120 was upregulated with a maximum of transcripts at day 7 of cultivation. The second gene with the gene ID AAE3_10454 showed a more slight increase expression peaking at day 11 and day 14. The peak area of 1 in the supernatant increased until day 9 of cultivation and lowered afterwards, whereas in the mycelium the bovistol peak area increased until day 11 and dropped afterwards. This steady increase of 1 until day 9 respectively day 11 resembles the preceding transcriptional upregulation of the expression of the gene with the ID AAE3_04120 which indicates that this gene is presumably involved in the bovistol synthesis pathway. In addition, the deduced protein sequence of the adjacent gene with the ID AAE3_04121 shows similarities to the Diels-Alderase Sol5 from Alternaria solani, which is involved in the cycloaddition of prosolanapyrone II into solanapyrone . A similar cycloaddition is needed to form bovistol out of two illudine precursors. Although the respective illudine has not been detected in this study, it is known that C. aegerita is able to produce several illudanes . As proposed in recent studies on sesquiterpenes in O. olearius , Stereum hirsutum  and Diaporthe sp.  the illudin precursor Δ6-protoilludene undergoes subsequent reactions catalyzed by enzymes, whose genes cluster with the Δ6-protoilludene synthase. Nevertheless, evidence is still missing. In C. aegerita, Δ6-protoilludene is seemingly provided by the putative sesquiterpene synthase AAE3_04120. Combining these indications, an enzymatic cascade coded by the AAE3_04120 cluster is transforming Δ6-protoilludene into illudine(s) and the corresponding bovistol in C. aegerita (Figure S2, Supporting Information File 1). Further research has to verify this assumption.
We identified bovistol A (1) as the main metabolite of C. aegerita in cultures. In parallel, we isolated its new disesquiterpenoid derivatives bovistol B (2) and C (3) as well as the new protoilludane pasteurestin C (4). By a qPCR approach, we were able to link the production of bovistol to the putative Δ6-protoilludene synthase AAE3_04120 whose gene is located adjacent to a Diels-Alderase needed for cycloaddition of two illudine monomers. With this information, we made a biosynthesis proposal for these metabolites. Further studies will address this assumption to prove its validity.
Optical rotations were measured on a Perkin-Elmer 241 spectrometer, the UV spectra on a Shimadzu UV–vis spectrophotometer UV-2450. NMR spectra were recorded with a Bruker Avance III 700 spectrometer, equipped with 5 mm TCI cryoprobe (1H 700 MHz, 13C 175 MHz). Chemical shifts δ were referenced to the solvents chloroform-d (1H, δ = 7.27 ppm; 13C, δ = 77.0 ppm), acetone-d6 (1H, δ = 2.05 ppm; 13C, δ = 29.92 ppm). ESIMS spectra were acquired on an Amazon ion trap mass spectrometer (Bruker Daltonik); HRESIMS spectra were acquired on a Maxis time-of-flight mass spectrometer (Bruker Daltonik), both combined with an Agilent 1200 series HPLC-UV system [column 2.1 × 50 mm, 1.7 μm, C18 Acuity UPLC BEH (Waters), solvent A: H2O + 0.1% formic acid; solvent B: ACN + 0.1% formic acid, gradient: 5% B for 0.5 min increasing to 100% B in 19.5 min, maintaining 100% B for 5 min, flow rate = 0.6 mL min−1, UV detection at 200–600 nm].
A culture of the strain C. aegerita AAE-3 with a total volume of 4 L was prepared in ZM ½ medium [molasses 47% (Nord Zucker AG Schladen, Germany) 5.00 g/L, oatmeal (Herrnmühle, Harald Feick OHG, Reichelsheim, Germany) 5.00 g/L, D(+)-sucrose (Carl Roth GmbH & Co, Karlsruhe, Germany) 4.00 g/L, D-mannitol (AppliChem GmbH, ITW Company, Darmstadt, Germany) 4.00 g/L, D-glucose monohydrate (Cargill Holding Germany GmbH, Krefeld, Germany) 1.50 g/L, CaCO3 (Carl Roth GmbH & Co KG, Karlsruhe, Germany) 1.50 g/L, lactalbumin hydrolysate (Oxoid LDT, Basingstocke, Hampshire, England) 0.50 g/L, (NH4)2SO4 0.50 g/L]. The pH value of the medium was set to 7.2. To inoculate the medium, 5 mL of a preculture were used. The inoculated shaking flasks were incubated on a lab shaker (NORD Drive systems SK CSX-3H, Getriebebau NORD GmbH & Co KG Drive Systems) at 23 °C. After one week of incubation the glucose concentration in the medium was tested daily. If no more free glucose could be found in the medium, the cultivation was extracted.
The mycelium was separated from the fermentation broth with the help of a fluted filter. The filtered mycelium was overlaid with actone (1:1 ratio) and digested in an ultrasonic bath (Sonorex digital 10P, BANDELIN electronic GmbH & Co KG, Berlin, Germany) for 30 min (two times). After the digest the mycelium was separated from the filtrate. The filtrate was narrowed up to the aqueous phase in vacuo. The aqueous phase was shaken out in a 1:1 ratio with ethyl acetate (+ 50 mL deionised H2O) in a separating funnel (two times) and dried with water-free sodium sulfate (Na2SO4, ACROS Organics, New Jersey, USA). The sodium sulfate was filtered off and the extract was narrowed up to the dry with a rotary evaporator. The crude extract was dissolved in 4 mL methanol, evaporated under a nitrogen evaporator (VLM GmbH, Bielefeld, Germany) and stored in a freezer at −20 °C. The crude extract of the fermentation broth was obtained the same way.
The crude extract obtained from the extraction was dissolved in 1 mL of methanol and further separated via RP-LC with deionized water (+ 0.05% TFA, solvent A) and methanol (+ 0.05%, solvent B) by a Gilson RP-HPLC system (Middleton, Wisconsin, USA) equipped with a GX-271 Liquid handler, a diode array detector (DAD) 172 and a 305 and 306 pump. The separation was performed with a VP Nucleodur C18ec (150 × 40 mm, 7 µm; Macherey-Nagel, Düren, Germany) column and a flow rate of 20 mL/min. The gradient was set from 30 to 70% of solvent B in 45 min, with an increase to 100% B in 15 min, followed by isocratic conditions at 100% B for 15 min. All LC fractions were collected according to the UV absorption at 210 nm. Methanol was evaporated in vacuo. The aqueous residues were frozen and then removed by using an Alpha 1-4 LSC freeze dryer (Christ, Osterode, Germany). 12.6 mg of fraction V were obtained as a mixture of compounds 1, 2 and 3. Furthermore fraction VI yielded 5.2 mg of pure compound 4.
Subsequently fraction V was separated via another RP-LC under different conditions. The separation was performed with the same Gilson RP-HPLC system and flow by using a Gemini 10u C18 (250 × 21.20 mm, 10 micron, Phenomenex Inc., Torrance, USA) column. Solvent B was changed to acetonitrile and also no TFA was added. The gradient was set from 50% to 75% of solvent B in 45 min with an increase to 100% B in 15 min, followed by isocratic conditions at 100% B for 15 min. Collection and work-up of the obtained fractions was performed as described above. This separation yielded 4 mg of compound 1, 2.2 mg of compound 2 and 0.4 mg of compound 3.
Bovistol A (1): Colourless oil; 1H and 13C NMR data (1H 700 MHz, 13C 175 MHz) in CDCl3: see Table 1; ESIMS (m/z): 1015.52 [2M + Na]+, 479.30 [M + H − H2O]+, 991.64 [2M − H]−, 541.39 [M + HCOO]−; HRESIMS (m/z): [M + Na]+ calcd for C30H40O6Na, 519.2717; found, 519.2718.
Bovistol B (2): colourless oil; [α]D25 +3 (c 0.1, CH3OH); 1H and 13C NMR data (1H 700 MHz, 13C 175 MHz) in CDCl3: see Table 1; ESIMS (m/z): 979.57 [2M + Na]+, 957.61 [2M + H]+, 479.35 [M + H]+, 523.30 [M + HCOO]−, 477.29 [M − H]−; HRESIMS (m/z): [M + Na]+ calcd for C30H38O5Na, 501.2585; found, 501.2606.
Bovistol C (3): Colourless oil; [α]D25 +106 (c 0.1, CH3OH); 1H and 13C NMR data (1H 700 MHz, 13C 175 MHz) in CDCl3: see Table 1; ESIMS (m/z): 1043.65 [2M + Na]+, 533.37 [M + Na]+, 493.31 [M + H − H2O]+, 509.30 [M − H]−, 555.32 [M + HCOO]−; HRESIMS (m/z): [M + Na]+ calcd for C31H42O6Na, 533.2874; found, 533.2859; [M + H]+ calcd for C31H43O6, 511.3054; found, 511.3044.
Pasteurestin C (4): Colourless oil; [α]D25 +21 (c 0.1, CH3OH); 1H and 13C NMR data (1H 700 MHz, 13C 175 MHz) in acetone-d6: see Table 2; ESIMS (m/z): 523.32 [2M + Na]+, 233.13 [M + H − H2O]+, 249.04 [M − H]−; HRESIMS (m/z): [M + Na]+ calcd for C15H22O3Na, 273.1461; found, 273.1460; [M + H]+ calcd for C15H23O3, 251.1642; found, 251.1637.
A seed culture of the strain C. aegerita AAE-3 with a total volume of 500 mL was prepared in ZM ½ medium. After incubation for 11 days the seed culture was homogenized with an ULTRA-TURRAX under sterile conditions and used for inoculation of a 15 L bioreactor (xCUBIO in-situ bbi biotech) filled with 10 L ZM ½ medium. The pH value was set to 7.2 (unregulated); the DO was also not regulated. The temperature was regulated at 23 °C. Furthermore the submerged aeration rate and stirrer speed was fixed to 0.15 vvm and 200 rpm (rushton turbine). For foam destruction into the process Tego Antifoam D2310 (Evonik Nutrition & Care GmbH) was used. After 29 days of cultivation the fermentation broth was harvested. The biomass and suspended substrates was separated by centrifugation.
During fermentation, mycelial samples were taken at day 2, 4, 7, 9, 11 and 14 and stored in RNAlater (Qiagen, Venlo, Netherlands) until further use. Fungal mycelium was freeze-dried and ground with liquid nitrogen. RNA was extracted from ground mycelium using Ambion TRIzol™ Reagent (life Technologies, Carlsberg, California, USA) according to the manufacturer’s instructions with minor changes according to the method of Chomczynski and Sacchi . RNA concentration was determined photometrically by a NanoPhotometer® Pearl (Implen, Munich, Germany). Reverse transcription was performed with the Invitrogen M-MLV Reverse Transcriptase kit (ThermoFisher Scientific, Waltham, Massachusetts, USA) according to the manufacturer’s protocol. 10 µL of extracted RNA and 1 µL of 10 µM oligo-(dT)30 primer (Eurofins, Waltham, Massachusetts, USA) were used for cDNA synthesis. For removal of RNA in the transcribed cDNA sample, 1 µL of AMRESCO RNase A (VWR International, Radnor, Pennsylvania, USA) was added and the mixture was incubated at 37 °C for 20 min. Primers for qPCR analysis were designed using Geneious 11.0.4. (Biomatters, Auckland, New Zealand). Primer pairs for C. aegerita housekeeping genes going by the gene IDs AAE3_02268 and AAE3_07669 (http://www.thines-lab.senckenberg.de/agrocybe_genome) have been identified and validated by NormFinder and geNorm algorithm to be the best combination for qPCR-based transcription analyses of C. aegerita by means of qPCR (data not published). Briefly, KAPA SYBR® FAST qPCR Master Mix (Kapa Biosystems, Wilmington, MA, USA), 900 nM forward primer, 900 nM reverse Primer (Table 3), 10 ng of cDNA and nuclease-free water were mixed. The qPCR reactions were performed in triplicates using the CFX Connect™ RT-PCR Detection System (Bio-Rad Laboratories, Hercules, CA, USA). The following conditions were applied: enzyme activation at 94 °C for 20 s followed by 40 cycles of 94 °C for 30 s, 58 °C for 30 s and 72 °C for 10 s.
Table 3: Primer sequences for qPCR.
|Gene IDa||Primer sequence (5’ to 3’)||Exon spanning|
aReferring to the gene IDs from the genomic sequence of C. aegerita AAE-3 (http://www.thines-lab.senckenberg.de/agrocybe_genome).
|Supporting Information File 1: 1H and 13C NMR spectra of compound 1 and 1H, 13C, COSY, ROESY, HSQC and HMBC NMR spectra of compounds 2–4.|
|Format: PDF||Size: 1.4 MB||Download|
We kindly thank C. Kakoschke for recording NMR spectra, A. Gollasch und S. Karwehl for HRESIMS measurements, V. Stiller for technical assistance with cultivation, W. Collisi for conducting bioassays and S. Hüttel and co-workers for the large scale fermentation. N. Sella is financed by the LOEWE program (State-Offensive for the Development of Scientific and Economic Excellence) “AROMAplus”. The authors are thankful for this support.