- Open Access
Boosting the biosynthesis of betulinic acid and related triterpenoids in Yarrowia lipolytica via multimodular metabolic engineering
© The Author(s) 2019
- Received: 31 January 2019
- Accepted: 24 April 2019
- Published: 3 May 2019
Betulinic acid is a pentacyclic lupane-type triterpenoid and a potential antiviral and antitumor drug, but the amount of betulinic acid in plants is low and cannot meet the demand for this compound. Yarrowia lipolytica, as an oleaginous yeast, is a promising microbial cell factory for the production of highly hydrophobic compounds due to the ability of this organism to accumulate large amounts of lipids that can store hydrophobic products and supply sufficient precursors for terpene synthesis. However, engineering for the heterologous production of betulinic acid and related triterpenoids has not developed as systematically as that for the production of other terpenoids, thus the production of betulinic acid in microbes remains unsatisfactory.
In this study, we applied a multimodular strategy to systematically improve the biosynthesis of betulinic acid and related triterpenoids in Y. lipolytica by engineering four functional modules, namely, the heterogenous CYP/CPR, MVA, acetyl-CoA generation, and redox cofactor supply modules. First, by screening 25 combinations of cytochrome P450 monooxygenases (CYPs) and NADPH-cytochrome P450 reductases (CPRs), each of which originated from 5 different sources, we selected two optimal betulinic acid-producing strains. Then, ERG1, ERG9, and HMG1 in the MVA module were overexpressed in the two strains, which dramatically increased betulinic acid production and resulted in a strain (YLJCC56) that exhibited the highest betulinic acid yield of 51.87 ± 2.77 mg/L. Then, we engineered the redox cofactor supply module by introducing NADPH- or NADH-generating enzymes and the acetyl-CoA generation module by directly overexpressing acetyl-CoA synthases or reinforcing the β-oxidation pathway, which further increased the total triterpenoid yield (the sum of the betulin, betulinic acid, betulinic aldehyde yields). Finally, we engineered these modules in combination, and the total triterpenoid yield reached 204.89 ± 11.56 mg/L (composed of 65.44% betulin, 23.71% betulinic acid and 10.85% betulinic aldehyde) in shake flask cultures.
Here, we systematically engineered Y. lipolytica and achieved, to the best of our knowledge, the highest betulinic acid and total triterpenoid yields reported in microbes. Our study provides a suitable reference for studies on heterologous exploitation of P450 enzymes and manipulation of triterpenoid production in Y. lipolytica.
- Betulinic acid
- Multimodular metabolic engineering
- Yarrowia lipolytica
Betulinic acid is a pentacyclic lupane-type triterpenoid that widely exists in plants and possesses many pharmacological activities, such as antiviral (especially anti-HIV infection) [1, 2], antitumor (as a melanoma-specific cytotoxic agent) [3, 4] and other antimetabolic syndrome activities [5–8]. This compound can be acquired by purification of extracts from the outer bark of a variety of tree species . Though this process has been optimized, problems such as low natural abundance, requirement of a large amount of land resources and long processing time are nonnegligible. The necessity for the development of an economical, ecofriendly and efficient production process has inspired researchers to use microorganisms for the production of betulinic acid .
Multimodular metabolic engineering is an efficient strategy for addressing perturbances such as imbalance in pathway flux, module incompatibility or accumulation of intermediates caused by manipulation of endogenous genes and the introduction of heterologous pathways, and this method enables systematic manipulation of strains and metabolic pathways [24, 25]. This potential strategy has been widely implemented in Escherichia coli and S. cerevisiae for the production of value-added compounds. By partitioning the biosynthetic pathway of the diterpene taxadiene into two modules—an upstream methylerythritol-phosphate (MEP) module and a heterologous downstream terpenoid-forming module—and balancing the two modules by using various promoters and gene copy numbers in E. coli, production of the taxadiene was increased 15,000-fold compared to that in the parent strain and a yield of 1.02 ± 0.08 g/L achieved in fed-batch bioreactor fermentations . Similarly, the production of miltiradiene (a kind of diterpenoid) in S. cerevisiae was improved from 0.5 to 12.5 mg/L by engineering MVA and heterologous synthase modules . Recently, this strategy was also used to boost the production of a kind of triterpene—protopanaxadiol. By dividing the biosynthetic pathway of this compound into four modules—MVA, triterpene biosynthesis, sterol biosynthesis, and acetyl-CoA formation modules—and manipulating these modules simultaneously, protopanaxadiol production was enhanced to 66.55 mg/L/OD600 . These studies demonstrated the potential of multimodular metabolic engineering for high-level production of terpenes and for addressing module incompatibility.
Yarrowia lipolytica, as a GRAS (generally recognized as safe) and oleaginous microorganism, has become a potential platform for the production of highly hydrophobic compounds [29, 30] because of the ability of this organism to accumulate large amounts of lipids that can store hydrophobic products [31, 32] and to supply sufficient intermediates and energy for terpene synthesis [33, 34]. In addition, the recent development of efficient and predictable synthetic biological tools in Y. lipolytica has contributed to the convenience of genetic manipulation in this organism [35–38]. Based on these factors, Y. lipolytica has been used to produce various hydrophobic terpenoids, such as linalool (monoterpene alcohol) , α-farnesene (sesquiterpene) , squalene (triterpene) , β-carotene, astaxanthin and lycopene (tetraterpene) [42–45]. In some cases, terpenoid production in Y. lipolytica was even higher than that in S. cerevisiae. For example, maximum production of β-carotene in Y. lipolytica was realized at 6.5 g/L , which demonstrated the potential of this strain for terpenoid production.
In this study, we used a multimodular metabolic engineering strategy to systematically engineer Y. lipolytica for production of the hydrophobic betulinic acid and related triterpenoids by dividing the biosynthetic pathway into four functional modules, including the heterogenous CYP/CPR, MVA, acetyl-CoA generation, and redox cofactor supply modules. By introducing exogenous genes or overexpressing endogenous key genes associated with these modules, we obtained a 51.87 ± 2.77 mg/L yield of betulinic acid and a 204.89 ± 11.56 mg/L yield of triterpenoids, both of which were the highest yields reported in shake flask cultures.
Screening the CYP/CPR module for biosynthesis of betulinic acid in Y. lipolytica
Previous studies have shown that in S. cerevisiae, recombinant plant CYPs work well with endogenous CPRs [21, 23]. However, our results and those of several other studies [20, 46, 47] indicated that in Y. lipolytica, plant CYPs might require the coexpression of heterogenous CPRs for exogenous terpenoid production. Accordingly, five CPR genes from different sources, namely, ATR2 from Arabidopsis thaliana, CrCPR from C. roseus, GuCPR from Glycyrrhiza uralensis, LjCPR from Lotus japonicus and MTR from M. truncatula, were expressed under the TEFin promoter and integrated into the IntF site (YALI0F3161413 to YALI0F3162449) . Twenty-five strains were generated, and the fermentation results are shown in Fig. 2a (GC profiles and mass spectra of YLJCC6 are shown as an example in Additional file 4: Figure S3a and b). The results show that the combinations of CYPs from two sources (BPLO or VvAO15) and CPRs from three sources (ATR2, LjCPR, or MTR) could achieve the synthesis of betulinic acid (six strains were generated: YLJCC2, YLJCC5, YLJCC6, YLJCC20, YLJCC23, YLJCC24). Among the various CYPs, BPLO possesses relatively higher catalytic capacity for betulinic acid production in S. cerevisiae [16, 17]. In this study, BPLO also showed high catalytic capacity in Y. lipolytica. VvAO15 shared close evolutionary relationships and high homology with BPLO (Additional file 5: Figure S4a and b), which might be the reason why VvAO15 also performed well in Y. lipolytica. In addition, among the six strains, YLJCC5 and YLJCC6 showed the highest production of betulinic acid and total triterpenoids (Fig. 2a), which might be caused by the efficient interaction between BPLO and the related CPRs (that is LjCPR or MTR) [17, 48]. The titer of betulinic acid in YLJCC5 and YLJCC6 was 25.62 ± 2.20 mg/L and 32.33 ± 4.34 mg/L, respectively.
To further optimize the CYP/CPR module, we tried to fuse BPLO with LjCPR or MTR or to localize the proteins in the endoplasmic reticulum (ER) (Fig. 2b, c). We used two strategies for fusion of CYP and CPR. In the first strategy, the two proteins were fused without any linker and designated L0. In the second strategy, CYP and CPR were fused with four different linkers, designated L1, L2, L3 and L4. The amino acid sequences of these four linkers were GGGS, GSG, GGGGS, EAAAK, where the first three represent flexible linkers and the last one represents a rigid linker. The results showed that when CYP was fused to the N-terminus of the CPRs, the generated strains YLJCC31-35 and YLJCC41-45 showed a dramatic decline in the production of betulinic acid compared with the control strains, regardless of the strategy of fusion (with or without linker, or with any kind of linker). However, when CYP was fused to the C-terminus of the CPRs, the engineered strains barely produced any triterpenoids (Fig. 2b). In summary, the fusion of CYP with CPR could not further improve betulinic acid production. On the other hand, an ER-targeting peptide (KDEL) was fused to the C-terminus of the CYP (BPLO) and CPRs (LjCPR and MTR)  to generate strains YLJCC101 and YLJCC102, which coexpressed LUS, CYP-ER and CPR-ER (Fig. 2c). Although previous studies reported that the involvement of the ER could facilitate P450 function [49, 50], neither total triterpenoid production nor betulinic acid production was improved in the engineered strains, possibly because we used the full-length sequences of CYP and CPR, not truncated sequences, for heterologous expression, and these sequences already have signal peptides in the N-terminus of the proteins for membrane translocation [26, 51]. We fused a sfGFP  to the C-terminus of BPLO, LjCPR and MTR (without the ER-targeting peptide), and the confocal microscopy images confirmed our hypothesis. As shown in Additional file 6: Figure S5, the expressed proteins were already located in the membrane or organelle in Y. lipolytica due to the presence of the native signal peptide.
Finally, because no further improvement was observed upon fusion of CYP with CPR or upon addition of the ER-targeting peptide, the two best production strains from the above optimization, namely, YLJCC5 and YLJCC6 (Fig. 2a), were selected and subjected to further engineering.
Improving the production of triterpenoids by engineering the MVA module
First, squalene epoxidase (encoded by ERG1), which is responsible for the first oxygenation step in sterol biosynthesis and is recognized as the key enzyme in this pathway , was overexpressed under the control of the EXP promoter in strains YLJCC5 and YLJCC6, generating strains YLJCC51 and YLJCC54. As shown in Fig. 3, the total triterpenoid levels in YLJCC51 and YLJCC54 were slightly increased. Then, we further overexpressed squalene synthase (encoded by ERG9), which converts FPP to squalene and represents the branching point of synthetic pathways of triterpenoids, sterols and sesquiterpenoids. The resulting strains, namely, YLJCC52 and YLJCC55, exhibited a further increase in betulinic acid and total triterpenoid production (Fig. 3). Finally, with the addition of HMG1, which encodes a rate-limiting enzyme in the MVA pathway, the production of betulinic acid in the generated strains YLJCC53 and YLJCC56 improved 1.25- and 1.60-fold, respectively, compared with YLJCC5 and YLJCC6, and the total triterpenoid production increased by 1.34-fold and 1.91-fold, respectively (Fig. 3).
Previously, overexpression of ERG1 in S. cerevisiae increased the levels of the triterpenoid protopanaxadiol . It has been demonstrated that overexpression of ERG9 enhanced triterpenoid accumulation in plants [55–57] and β-amyrin production in S. cerevisiae . Overexpression of tHMG1 (encoding the N-terminal truncated version of HMG1) is a commonly used approach to improve the production of terpenoids because this method can overcome the tight regulation of HMG1 in host cells [40, 42, 59–61]. However, some data indicated that overexpression of homologous HMG1 was more effective than overexpression of tHMG1 for production of the monoterpene limonene in Y. lipolytica . Recently, overexpression of endogenous HMG1 improved squalene synthesis 3.2-fold in Y. lipolytica . Hence, we chose to overexpress HMG1 rather than tHMG1 in Y. lipolytica. Our results suggested that overexpression of ERG1 and ERG9 only slightly enhanced betulinic acid production in Y. lipolytica. Further overexpression of HMG1 led to a marked improvement in the yield of the product.
Improving triterpenoid production via engineering of the redox cofactor supply module
Improving triterpenoid synthesis via engineering of the acetyl-CoA generation module
Overexpression of the endogenous ATP citrate lyase gene (ylACL1) has been previously shown to increase the level of cytosolic acetyl-CoA 1.5-fold in Y. lipolytica [41, 63]. However, in this study, overexpression of ACL1 (YLJCC71) failed to improve the production of triterpenes, while overexpression of ACL2 (YLJCC72) increased the titers of total triterpenoids and betulinic acid 1.23- and 1.30-fold, respectively (Fig. 5). On the other hand, overexpression of all the genes in the β-oxidation pathway except PEX10 in YLJCC5 led to increased triterpene production. Among the generated strains, YLJCC76 (overexpressing POT1) exhibited the most significant enhancement of production with a triterpene yield of 66.77 ± 2.79 mg/L. Similarly, this elevated production did not occur in the strains generated from YLJCC6, which might be caused by module incompatibility.
In most cases, studies have focused on elimination of the competition pathway to reduce carbon loss. For example, α-santalene production increased upon knocking out of citrate synthase or malate synthase, which convert acetyl-CoA to citrate or C4 organic acids, respectively . Fatty acid biosynthesis is also considered to be a competitive pathway for terpenoid synthesis because these pathways use the same precursor—acetyl-CoA. To reduce competition, the endogenous promoters of the key genes in the fatty acid pathway were replaced with relatively weak promoters, and the betulinic acid yield increased to 1.92 mg/L/OD in S. cerevisiae . In this study, we applied a different strategy to address competition by enhancing fatty acid β-oxidation to recover acetyl-CoA. The results indicated that the strategy was effective for betulinic acid-related triterpenoid production in Y. lipolytica.
Further increasing the production of triterpenoids by multimodular optimization
Herein, we systematically engineered Y. lipolytica using a multimodular strategy to increase triterpenoid production. By matching CYPs and CPRs, both of which originated from five different sources, and coexpressing these proteins with LUS, we established betulinic acid synthesis in Y. lipolytica. Then, the MVA module, acetyl-CoA generation module, and redox cofactor supply module were optimized separately. The betulinic acid yield improved to 51.87 ± 2.77 mg/L when ERG1, ERG9, and HMG1 in the MVA module were overexpressed with RcLUS, BPLO and MTR. Finally, the optimal modules were integrated, and a 204.89 ± 11.56 mg/L total triterpenoid yield was realized when RcLUS, BPLO and LjCPR were coexpressed with the upregulated MVA (overexpressing ERG1, ERG9 and HMG1) and acetyl-CoA generation module (overexpressing MFE1). Both betulinic acid and total triterpenoid production achieved the highest reported yields in microbes in shake flask cultures. This study can serve as a foundation for the construction of efficient triterpene production strains of Y. lipolytica.
Strains, medium and culture conditions
Strains used in this work
Y. lipolytica ATCC 201249
MATA, ura3-302, leu2-270, lys8-11, pex17-HA
Provided by professor Yuan Yingjin (Tianjin University, China)
201249 Δku70::PTEFin-RcLUS-acot, hisG
YLJCC0 Δku80::PFBAin-BPLO-octt, hisG
YLJCC0 Δku80::PFBAin-CrAO-octt, hisG
YLJCC0 Δku80::PFBAin-MtAO12-octt, hisG
YLJCC0 Δku80::PFBAin-VvAO15-octt, hisG
YLJCC0 Δku80::PFBAin-VvAO17-octt, hisG
YLJCC0 Δku80::PFBAin-BPLO-LjCPR-octt, hisG-URA3-hisG
YLJCC0 Δku80::PFBAin-BPLO-L1-LjCPR-octt, hisG-URA3-hisG
YLJCC0 Δku80::PFBAin-BPLO-L2-LjCPR-octt, hisG-URA3-hisG
YLJCC0 Δku80::PFBAin-BPLO-L3-LjCPR-octt, hisG-URA3-hisG
YLJCC0 Δku80::PFBAin-BPLO-L4-LjCPR-octt, hisG-URA3-hisG
YLJCC0 Δku80::PFBAin-LjCPR-BPLO-octt, hisG-URA3-hisG
YLJCC0 Δku80::PFBAin-LjCPR-L1-BPLO-octt, hisG-URA3-hisG
YLJCC0 Δku80::PFBAin-LjCPR-L2-BPLO-octt, hisG-URA3-hisG
YLJCC0 Δku80::PFBAin-LjCPR-L3-BPLO-octt, hisG-URA3-hisG
YLJCC0 Δku80::PFBAin-BPLO-MTR-octt, hisG-URA3-hisG
YLJCC0 Δku80::PFBAin-BPLO-L1-MTR-octt, hisG-URA3-hisG
YLJCC0 Δku80::PFBAin-BPLO-L2-MTR-octt, hisG-URA3-hisG
YLJCC0 Δku80::PFBAin-BPLO-L3-MTR-octt, hisG-URA3-hisG
YLJCC0 Δku80::PFBAin-BPLO-L4-MTR-octt, hisG-URA3-hisG
YLJCC0 Δku80::PFBAin-MTR-BPLO-octt, hisG-URA3-hisG
YLJCC0 Δku80::PFBAin-MTR-L2-BPLO-octt, hisG-URA3-hisG
YLJCC0 Δku80::PFBAin-MTR-L3-BPLO-octt, hisG-URA3-hisG
YLJCC0 Δku80::PFBAin-MTR-L4-BPLO-octt, hisG-URA3-hisG
YLJCC5 rDNA::PEXP-ERG1-xpr2t, PTEFin-ERG9-lip2t
YLJCC5 rDNA::PEXP-ERG1-xpr2t, PTEFin-ERG9-lip2t, PTEFin-HMG1-octt
YLJCC6 rDNA::PEXP-ERG1-xpr2t, PTEFin-ERG9-lip2t
YLJCC6 rDNA::PEXP-ERG1-xpr2t, PTEFin-ERG9-lip2t, PTEFin-HMG1-octt
YLJCC5 IntE::PTEFin-EMC-pex20t, hisG-URA3-hisG
YLJCC5 IntE::PTEFin-EMT-pex20t, hisG-URA3-hisG
YLJCC5 IntE::PTEFin-Rtme-pex20t, hisG-URA3-hisG
YLJCC5 IntE::PTEFin-Gapc-pex20t, hisG-URA3-hisG
YLJCC6 IntE::PTEFin-EMC-pex20t, hisG-URA3-hisG
YLJCC6 IntE::PTEFin-EMT-pex20t, hisG-URA3-hisG
YLJCC6 IntE::PTEFin-Rtme-pex20t, hisG-URA3-hisG
YLJCC6 IntE::PTEFin-Gapc-pex20t, hisG-URA3-hisG
YLJCC5 IntE::PTEFin-ACL1-pex20t, hisG-URA3-hisG
YLJCC5 IntE::PTEFin-ACL2-pex20t, hisG-URA3-hisG
YLJCC5 IntE::PTEFin-PXA1-pex20t, hisG-URA3-hisG
YLJCC5 IntE::PTEFin-MFE1-pex20t, hisG-URA3-hisG
YLJCC5 IntE::PTEFin-PEX10-pex20t, hisG-URA3-hisG
YLJCC5 IntE::PTEFin-POT1-pex20t, hisG-URA3-hisG
YLJCC5 IntE::PTEFin-TGL3-pex20t, hisG-URA3-hisG
YLJCC6 IntE::PTEFin-ACL1-pex20t, hisG-URA3-hisG
YLJCC6 IntE::PTEFin-ACL2-pex20t, hisG-URA3-hisG
YLJCC6 IntE::PTEFin-PXA1-pex20t, hisG-URA3-hisG
YLJCC6 IntE::PTEFin-MFE1-pex20t, hisG-URA3-hisG
YLJCC6 IntE::PTEFin-PEX10-pex20t, hisG-URA3-hisG
YLJCC6 IntE::PTEFin-POT1-pex20t, hisG-URA3-hisG
YLJCC6 IntE::PTEFin-TGL3-pex20t, hisG-URA3-hisG
YLJCC53 IntE::PTEFin-EMT-pex20t, hisG-URA3-hisG
YLJCC53 IntE::PTEFin-Rtme-pex20t, hisG-URA3-hisG
YLJCC56 IntE::PTEFin-EMT-pex20t, hisG-URA3-hisG
YLJCC56 IntE::PTEFin-Rtme-pex20t, hisG-URA3-hisG
YLJCC53 IntE::PTEFin-ACL2-pex20t, hisG-URA3-hisG
YLJCC53 IntE::PTEFin-PXA1-pex20t, hisG-URA3-hisG
YLJCC53 IntE::PTEFin-MFE1-pex20t, hisG-URA3-hisG
YLJCC53 IntE::PTEFin-POT1-pex20t, hisG-URA3-hisG
YLJCC53 IntE::PTEFin-TGL3-pex20t, hisG-URA3-hisG
YLJCC56 IntE::PTEFin-ACL2-pex20t, hisG-URA3-hisG
YLJCC56 IntE::PTEFin-PXA1-pex20t, hisG-URA3-hisG
YLJCC56 IntE::PTEFin-MFE1-pex20t, hisG-URA3-hisG
YLJCC56 IntE::PTEFin-POT1-pex20t, hisG-URA3-hisG
YLJCC56 IntE::PTEFin-TGL3-pex20t, hisG-URA3-hisG
YLJCC0 Δku80::PFBAin-BPLO-ER-octt, hisG; IntE::PTEFin-LjCPR-ER-pex20t, hisG-URA3-hisG
YLJCC0 Δku80::PFBAin-BPLO-ER-octt, hisG; IntE::PTEFin-MTR-ER-pex20t, hisG-URA3-hisG
201249 Δku80::PFBAin-BPLO-sfGFP-octt, hisG-URA3-hisG
201249 Δku80::PFBAin-LjCPR-sfGFP-octt, hisG-URA3-hisG
201249 Δku80::PFBAin-MTR-sfGFP-octt, hisG-URA3-hisG
The proper auxotrophic medium used to grow transformants consisted of 20 g/L glucose H2O, 5 g/L (NH4)2SO4, 1.7 g/L yeast nitrogen base without amino acids, 2 g/L complete supplement mixture (CSM) lacking uracil (SC-Ura) or leucine (SC-Leu). YPD-hum medium containing 200 mg/L hygromycin was also used to screen the recombined strains, and 20 g/L agar was added for preparation of solid plates. Rich YPD medium, consisting of 50 g/L glucose, 20 g/L peptone, and 10 g/L yeast extract, was used for fermentation.
The seed cultures were first prepared in 25-mL polypropylene tubes containing 5 mL of YPD medium. After 24 h, the seed cultures were inoculated into a 250-mL shake flask containing 50 mL of rich YPD medium with an initial OD600 of 0.2 for 168 h. A 1/5 volumetric ratio of isopropyl myristate (IPM) was added to the shake flasks at 120 h to extract the products. All the titers presented in this research were based on the volume of the fermentation media. All assays were performed in at least triplicate (at least three independent assays for three different clones).
Plasmids and strain construction
Plasmids used in this work
Ku70up-PTEFin-acot-hisG-URA3-hisG-Ku70dn cassette in PUC57-1.8k
Ku80up-PFBAin-octt-hisG-URA3-hisG-Ku80dn cassette in PUC57-kan
IntFup-PTEFin-lip1t-LUE-IntFdn cassette in PUC57-1.8k
IntEup-PTEFin-pex20t-hisG-URA3-hisG-IntEdn cassette in PUC57-1.8k
RcLUS was cloned into pIntK
BPLO was cloned into pK8FB
CrAO was cloned into pK8FB
MtAO12 was cloned into pK8FB
VvAO15 was cloned into pK8FB
VvAO17 was cloned into pK8FB
ATR2 was cloned into pIntF
CrCPR was cloned into pIntF
GuCPR was cloned into pIntF
LjCPR was cloned into pIntF
MTR was cloned into pIntF
BPLO-L0-LjCPR was cloned into pK8FB
BPLO-L1-LjCPR was cloned into pK8FB
BPLO-L2-LjCPR was cloned into pK8FB
BPLO-L3-LjCPR was cloned into pK8FB
BPLO-L4-LjCPR was cloned into pK8FB
LjCPR-L0-BPLO was cloned into pK8FB
LjCPR-L1-BPLO was cloned into pK8FB
LjCPR-L2-BPLO was cloned into pK8FB
LjCPR-L3-BPLO was cloned into pK8FB
BPLO-L0-MTR in pK8FB
BPLO-L1-MTR was cloned into pK8FB
BPLO-L2-MTR was cloned into pK8FB
BPLO-L3-MTR was cloned into pK8FB
BPLO-L4-MTR was cloned into pK8FB
MTR-L0-BPLO was cloned into pK8FB
MTR-L2-BPLO was cloned into pK8FB
MTR-L3-BPLO was cloned into pK8FB
MTR-L4-BPLO was cloned into pK8FB
ERG1 was cloned into pLD01
ERG9 was cloned into pLD02in
HMG1 was cloned into pLD03in
ACL1 was cloned into pIntE
ACL2 was cloned into pIntE
PXA1 was cloned into pIntE
POT1 was cloned into pIntE
MFE1 was cloned into pIntE
TGL3 was cloned into pIntE
PEX10 was cloned into pIntE
EMC was cloned into pIntE
EMT was cloned into pIntE
Gapc was cloned into pIntE
Rtme was cloned into pIntE
BPLO-ER was cloned into pK8FB
LjCPR-ER was cloned into pIntE
MTR-ER was cloned into pIntE
BPLO-sfGFP was cloned into pK8FB
LjCPR-sfGFP was cloned into pK8FB
MTR-sfGFP was cloned into pK8FB
Fusion protein-encoding genes were obtained by overlap extension polymerase chain reaction (PCR). All the primers used to construct fusion protein-encoding genes were synthesized by Genewiz Inc. (China) and are listed in Additional file 7: Table S2. We applied two types of fusion between CYP and CPR. In the first case, CYPs were fused with CPRs directly (marked as L0) and generated pK8FB-BPLO-LjCPR, pK8FB-BPLO-MTR, pK8FB-LjCPR-BPLO, and pK8FB-MTR-BPLO. In the other case, CYPs and CPRs were fused with different linkers, which contained linker1 (L1) “GGAGGAGGATCT”, linker2 (L2) “GGATCTGGA, linker3 (L3) “GGAGGAGGAGGATCT”, and linker4 (L4) “GAGGC CGCCGCCAAG” (the first three represents flexible linkers and the last one represents rigid linker), and generated pK8FB-BPLO-L1-LjCPR, pK8FB-BPLO-L2-LjCPR, pK8FB-BPLO-L3-LjCPR, pK8FB-BPLO-L4-LjCPR, pK8FB-LjCPR-L1-BPLO, pK8FB-LjCPR-L2-BPLO, pK8FB-LjCPR-L3-BPLO, pK8FB-BPLO-L1-MTR, pK8FB-BPLO-L2-MTR, pK8FB-BPLO-L3-MTR, pK8FB-BPLO-L4-MTR, pK8FB-MTR-L2-BPLO, pK8FB-MTR-L3-BPLO and pK8FB-MTR-L4-BPLO. All the fragments were amplified with the proper sticky ends and incorporated into the integration plasmid K8FB by Golden Gate assembly. The ER-targeting peptide (KDEL) and sfGFP were fused to the C-terminus of CYP and CPR to generate pK8FB-BPLO-ER, pIntE-LjCPR-ER, pIntE-MTR-ER, and pK8FB-BPLO-sfGFP, pK8FB-LjCPR-sfGFP, and pK8FB-MTR-sfGFP.
All the integrative fragments were transformed into Y. lipolytica using the Zymogen Frozen EZ Yeast Transformation Kit II (Zymo Research Corporation). Two micrograms of linearized DNA were used in the transformation reaction, and then, the cells were harvested and plated on selective solid plates. The Ura3 selection maker was recycled by incubating the transformants in 4 mL of YPD for 4 days and diluting 10,000 times on SC solid medium containing 1.2 mg/mL 5-fluoroorotic acid for 2 days. The genotypes of all the strains were confirmed by colony PCR using KOD FX DNA polymerase (Toyobo Co., Ltd.; Shanghai, China). The restriction endonucleases and ligase used for plasmid construction were purchased from NEB. Plasmid extraction and DNA fragment purification were performed using the TIANprep Mini Plasmid Kit and TIANgal Midi Purification Kit, respectively (TIANGEN BIOTECH, China). Gibson assembly was carried out using the ClonExpressII One Step Cloning Kit (Vazyme, China).
Lupeol, betulinic acid, betulin, and betulinic aldehyde extraction and analysis
The IPM phase was collected by centrifugation of 10 mL of fermentation broth mixture (10 min, 5000 rpm) followed by filtration with a 0.22-μm film. Then, 50 μL of the resulting extract was trimethylsilylated by mixing with 150 μL of N-methyl-N-(trimethylsilyl) trifluoracetamide (MSTFA) at 80 °C for 1 h and filtering with a 0.22-μm film. Appropriate concentrations of lupeol, betulin (Aladdin Industrial Corporation, US) and betulinic acid (MedChemExpress, US) were dissolved in IPM to prepare standard curves via GC–MS analysis. The methods used for betulinic acid detection were based on previous studies with some modification [15–17, 20]. A Rts-5 MS (30 m × 0.25 mm × 0.5 μm) GC column was used on a SHIMADZU GCMS-QP2020 system. A 1-μL sample was injected by AOC-20i+s with a split ratio of 10. The temperature of the injector was set at 250 °C. The initial oven temperature was maintained at 80 °C for 2 min, and then, the temperature was increased to 300 °C at a rate of 20 °C/min and held for 17 min. The GC system was operated under a constant pressure of 91 kPa. For the MS system, the temperature of the ion source was 230 °C, and full scan mode was used from 50 to 700 m/z.
Squalene extraction and analysis
Extraction and analysis of squalene were performed according to Guo XJ et al.  with some modification. Cells were harvested by centrifugation and washed 3 times with distilled water. Then, 1 mL of 3 M HCl was added for resuspension, followed by boiling in a 100 °C water bath for 5 min. The cell debris was washed with distilled water until the pH was neutral. NaOH solution was used to neutralize the residual HCl. Then, the cell pellet was resuspended with 1.5 M NaOH-methanol solution and incubated at 60 °C for 4 h. Then, 500 μL of hexyl hydride was added to the tubes, and the mixture was vortexed for 20 min. After centrifugation, the hexyl hydride layer was transferred to new tubes. This process was repeated once. The hexyl hydride layer was vacuum-dried, resuspended in 100 μL of MSTFA and incubated at 30 °C for 2 h. After filtering with a 0.22-μm film, the sample was used for GC–MS detection. A Rts-5 MS (30 m × 0.25 mm × 0.5 μm) GC column was used on the SHIMADZU GCMS-QP2020 system. A 1-μL sample was injected by AOC-20i + s with a split ratio of 5. The temperature of the injector was set at 280 °C. The initial oven temperature was maintained at 70 °C for 1 min, and then, the temperature was increased to 250 °C at a rate of 30 °C/min and held for 2 min. Then, the temperature was increased to 280 °C at a rate of 20 °C/min and held for 20 min. The GC system was operated under a constant pressure of 91 kPa. For the MS system, the temperature of the ion source was 220 °C, and full scan mode was used from 50 to 600 m/z.
Lipid extraction and analysis
Extraction and analysis of lipids were performed according to Wang et al. . Cells were harvested by centrifugation and washed 3 times with distilled water. One milliliter of methanol containing 3 M HCl and 100 mg/L heptadecanoic acid (as an internal standard) was added to the tubes and vortexed for mixing. Then, these tubes were incubated at 70 °C for 3 h and inverted several times for 40 min. Then, these tubes were cooled naturally to the indoor temperature. Then, sodium chloride was added into the solutions until saturation, and the solutions were shaken for 1 min. Then, 500 μL of hexyl hydride was added into these tubes with shaking for 1 min. The hexyl hydride phase was collected by centrifugation, filtered with a 0.22-μm film and used for the detection of lipid production by GC–MS. A Rts-5 MS (30 m × 0.25 mm × 0.5 μm) GC column was used on a SHIMADZU GCMS-QP2020 system. A 1-μL sample was injected by AOC-20i+s with a split ratio of 50. The temperature of the injector was set at 260 °C. The initial oven temperature was maintained at 70 °C for 2 min, and then, the temperature was increased to 290 °C at a rate of 8 °C/min and held for 6 min. The GC system was operated under a constant pressure of 91 kPa. For the MS system, the temperature of the ion source was 220 °C, and full scan mode was used from 50 to 500 m/z.
Phylogenetic tree and homology analyses
Full-length amino acid sequences were obtained from GenBank and aligned by ClustalW. A phylogenetic tree was constructed using the neighbor-joining method with 1000 replicates using MEGA6 software. Amino acid sequence homology analysis was performed with BLASTP.
Confocal laser scanning microscopy
Cell imaging was performed using UltraView Vox (PerkingElmer, America) after washing with ddH2O. Excitation/emission wavelengths were 488 nm/530 nm for GFP.
CCJ and JLZ performed the experiments. YXC, CCJ, JLZ and HS conceived of this study and drafted the manuscript. All authors read and approved the final manuscript.
The authors are grateful for the financial support from the Major Program of The National Natural Science Foundation of China (21621004) and the Young Elite Scientists Sponsorship Program by Tianjin (TJSQNTJ-2018-16).
The authors declare that they have no competing interests.
Availability of data and materials
Data will be made available from the corresponding author on reasonable request.
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