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  • Research article
  • Open Access

Metabolic engineering of microbes for branched-chain biodiesel production with low-temperature property

Biotechnology for Biofuels20158:92

https://doi.org/10.1186/s13068-015-0270-7

©  Tao et al. 2015

  • Received: 17 March 2015
  • Accepted: 5 June 2015
  • Published:

Abstract

Background

The steadily increasing demand for diesel fuels calls for renewable energy sources. This has attracted a growing amount of research to develop advanced, alternative biodiesel worldwide. Several major disadvantages of current biodiesels are the undesirable physical properties such as high viscosity and poor low-temperature operability. Therefore, there is an urgent need to develop novel and advanced biodiesels.

Results

Inspired by the proven capability of wax ester synthase/acyl-coenzyme A, diacylglycerol acyltransferase (WS/DGAT) to generate fatty acid esters, de novo biosynthesis of fatty acid branched-chain esters (FABCEs) and branched fatty acid branched-chain esters (BFABCEs) was performed in engineered Escherichia coli through combination of the (branched) fatty acid biosynthetic pathway and the branched-chain amino acid biosynthetic pathway. Furthermore, by modifying the fatty acid pathway, we improved FABCE production to 273 mg/L and achieved a high proportion of FABCEs at 99.3 % of total fatty acid esters. In order to investigate the universality of this strategy, Pichia pastoris yeast was engineered and produced desirable levels of FABCEs for the first time with a good starting point of 169 mg/L.

Conclusions

We propose new pathways of fatty acid ester biosynthesis and establish proof of concept through metabolic engineering of E. coli and P. pastoris yeast. We were able to produce advanced biodiesels with high proportions FABCEs and BFABCEs. Furthermore, this new strategy promises to achieve advanced biodiesels with beneficial low-temperature properties.

Keywords

  • Biodiesel
  • Branched-chain esters
  • Metabolic engineering
  • Branched-chain amino acid biosynthesis
  • WS/DGAT
  • E. coli
  • Pichia pastoris

Background

With rapidly diminishing reserves of petroleum and increasing concerns about climate change, the development of renewable fuels as alternatives to fossil fuels has become a worldwide priority. Currently, the predominant alternative fuels for transportation are corn ethanol and soybean biodiesel, but they cannot satisfy the increasing demands [1–3]. Biodiesel, derived from transesterification of vegetable oils or animal fats with monohydric alcohols, is an environmentally attractive alternative for conventional diesel fuels [4, 5]. Compared with petroleum, biodiesel has a large number of advantages including inherent lubricity and low toxicity. However, large-scale commercial biodiesel production requires very large amounts of vegetable oil that will result in competition with food industries and agriculture [6, 7]. To circumvent these hurdles, several biosynthetic pathways have been engineered to produce advanced biofuels [8–12]. Since fatty acids are precursors that can be converted to various products, the fatty acid biosynthetic pathway is especially attractive among these pathways, and many strategies have been applied to increase fatty acid production, for example, overexpression of acetyl-CoA carboxylase and thioesterase [13–16], in vitro reconstitution assay [17], reversal of the β-oxidation cycle strategy [18], and modular optimization of multi-gene pathways [19].

However, fatty acids cannot be utilized directly as biofuel due to the ionic nature of their carboxyl groups [3]; many studies have focused on the direct biosynthesis of biodiesels. After the identification of a novel wax ester synthase/acyl-CoA, diacylglycerol acyltransferase (WS/DGAT), which can synthesize fatty acid esters from alcohols and fatty acyl-CoAs [20, 21], this process became more popular. In Escherichia coli, Steinbüchel’s group achieved 0.26 g/L fatty acid ethyl esters (FAEEs) with exogenous oleic acid [22], and Keasling’s group obtained 674 mg/L FAEEs without feeding fatty acids [6]. In addition, fed-batch cultivation and a dynamic sensor-regular system also improved FAEEs production to 0.922 and 1.5 g/L, respectively [23, 24]. Moreover, several groups also engineered Saccharomyces cerevisiae to produce FAEEs [25, 26], and Nielsen’s group achieved a FAEE production of 34 mg/L by chromosome engineering and achieved another 40 % increase in FAEE production by overexpression of two genes (ACB1 and gapN) [27].

In general, biodiesels usually refer to fatty acid methyl esters (FAMEs) or FAEEs. However, many recent studies have reported enhanced ester biosynthesis, especially the work of Atsumi’s group, which demonstrated the biosynthesis of a multitude of esters by combination of various alcohols and a diversity of CoA molecules, achieving a high production of isobutyl acetate from glucose (17.2 g/L) [28]. In addition, some investigations focused on the production of medium-chain esters in E. coli, such as isobutyl acetate and isoamyl acetate as well as butyrate esters [29, 30]. In our previous work, we presented fatty acid short-chain ester (FASE) biosynthesis as an improvement of the low-temperature properties of traditional fuels. This was achieved by expression of WS/DGAT, which catalyzes the esterification of fatty acyl-CoAs and short-chain alcohols, synthesized from the 2-keto acid pathway by expression of 2-keto acid decarboxylase (ARO10) and an alcohol dehydrogenase (ADH2). After further engineering, the optimal strain produced 209 ± 2.6 mg/L FASEs with 50 % being fatty acid branched-chain esters (FABCEs) [31].

Although we have a chieved biosynthesis of FASEs, a higher proportion of FABCEs would still be desirable due to their improved low-temperature properties. One disadvantage of biodiesels is their poor performance at temperatures below 0 °C because crystals can plug fuel lines and filters, causing problems in fuel pumping and engine operation [32]. Structural features, such as chain length, degree of unsaturation, and branching of the chain, influence the physical and fuel properties of a fatty acid ester molecule [33]. As reported earlier, when branches were introduced into linear, long-chain esters, the intramolecular associations should be attenuated and the crystallization temperatures reduced; furthermore, methyl branches can improve the low-temperature properties of biodiesels without increasing their oxidative susceptibility [34]. As previously reported, FABCEs exhibit lower freezing point and have a lower cloud point. For example, the cloud points of isopropyl and 2-butyl soyate are −9 and −12 °C, while the cloud point of methyl soyate is 0 °C [32, 35].

Since both the fatty acid chain and the alcohol functionality contribute to the overall properties of a fatty acid ester molecule [33] and there are several studies which have reported the biosynthesis of branched-chain alcohols, such as isopropanol, isobutanol, and isoamylol, using branched-chain amino acid biosynthetic precursors in E. coli [36–39], here we present de novo biosynthesis of a higher proportion of FABCEs, including fatty acid isobutyl esters (FAIBEs) and fatty acid isoamyl esters (FAIAEs), which can be achieved through combination of the branched-chain amino acid biosynthetic pathways and fatty acid biosynthetic pathways in E. coli (Fig. 1). In addition, since some studies have reported the biosynthesis of branched-chain fatty acids [40–42], we successfully incorporated branched chains into both the fatty acid module and the alcohol module, yielding branched fatty acid branched-chain esters (BFABCEs) which expended the branched-chain ester variety. Finally, to test the universality of our strategy, we introduced the FABCE biosynthetic pathway into a eukaryote, Pichia pastoris yeast, resulting in a high production of FABCEs for the first time.
Fig. 1
Fig. 1

Engineered pathways for the production of FABCEs. Branched-chain alcohols (isobutanol and isoamylol) were produced through the branched-chain amino acid biosynthetic pathway by overexpression of alsS, ilvC, ilvD, aro10, and adh2. FABCEs were synthesized through esterification of branched-chain alcohols and fatty acyl-CoAs by overexpression of ws/dgat. Furthermore, BFABCEs were produced by overexpression of ws/dgat which can catalyze esterification of branched-chain alcohols and branched fatty acyl-CoAs produced by the overexpression of bckd and fabHB

Results

De novo biosynthesis of FAIBEs and FAIAEs in E. coli

The valine and leucine biosynthetic pathways can generate two 2-keto acids: 2-ketoisovalerate and 2-ketoisocaproate. These can be converted into isobutanol and 3-methyl-1-butanol, respectively, via 2-keto-acid decarboxylase (KDC), and subsequently into alcohols by alcohol dehydrogenase (ADH) [36, 37]. We successfully generated FABCEs by combining fatty acid biosynthetic pathways with the valine and leucine biosynthetic pathways (Fig. 1). The alsS gene from Bacillus subtilis and ilvCD genes from E. coli were sub-cloned into the plasmid pDG102 [31], which expressed ws/dgat, aro10, adh2, and fadD genes under the control of T7 promoter. The resulting plasmid pDG104 was transformed into the E. coli BL21 (DE3) strain.

Recombinant E. coli cells were cultivated in a modified M9 medium and treated with isopropyl β-d-thiogalactopyranoside (IPTG) to induce expression of the genes mentioned above. Cell cultures were extracted 28 h after induction, and FABCEs quantified by gas chromatography–mass spectrometry (GC-MS, Additional file 1: Figure S1). Each FABCE was confirmed by corresponding standards that were synthesized by esterification of authentic fatty acid standards and alcohols (Additional file 2). The FABCE titer, yield, and productivity were 56 ± 6.3 mg/L, 2.8 ± 0.32 mg/g glycerol, and 2.0 ± 0.23 mg/L/h (Table 1), respectively. In this strain, 2015 ± 171.0 mg/L isobutanol and 838 ± 57.6 mg/L isoamylol were detected.
Table 1

Production of FABCEs in engineered E. coli

Strains

Concentration (mg/gDCW)

Yield (mg/g glycerol)

Productivity (mg/L/h)

BL21/pDG104

19 ± 1.3

2.8 ± 0.32

2.0 ± 0.23

BL21/pDG104/pDG105

142 ± 19.1

13.7 ± 2.05

9.8 ± 1.46

TL101/pDG104/pDG105

296 ± 26.8

8.9 ± 1.10

6.3 ± 0.79

Because we observed a large amount of branched-chain alcohols, we hypothesized that the amount of the other substrates, fatty acyl-CoAs, was not sufficient in our recombinant strain. Thus, increasing the fatty acyl-CoA supply should probably improve FABCE production. As previously described, the accumulation of fatty acyl-acyl carrier proteins (ACP) inhibits fatty acid biosynthesis [16, 43]. In order to overcome this problem, we attempted to overexpress a cytoplasmic thioesterase (TesA’ lacking the leader sequence for periplasmic secretion), which can alleviate the feedback inhibition of fatty acid biosynthesis by the accumulated fatty acyl-ACPs [13–16, 44, 45]. Therefore, we constructed the plasmid pDG105 expressing the tesA’ gene under the control of T7 promoter with a pSC101 replication origin. Coupled with pDG105, the modified strain (BL21/pDG104/pDG105) produced higher levels of FABCEs (273 ± 40.9 mg/L) with a high proportion of FABCEs at 99.3 % of total fatty acid ester production. FABCE yield and productivity were calculated to be 13.7 ± 2.05 mg/g glycerol and 9.8 ± 1.46 mg/L/h, respectively (Table 1). In addition, the branched-chain alcohols were quantified to be 513 ± 24.9 mg/L isobutanol and 499 ± 28.9 mg/L isoamylol. Thus, overexpression of TesA’ improved FABCE production by 4.9-fold compared to strain BL21/pDG104.

However, substantial accumulations of branched-chain alcohols were still present in cells, prompting us to take further measures to increase the fatty acyl-CoA supply. Since fatty acyl-CoAs can be degraded via the β-oxidation pathway, the plasmids pDG104 and pDG105 were transformed into E. coli TL101 which was constructed to block fatty acyl-CoA degradation by deleting the fadE operon in strain BL21 (DE3) as previously described [17]. Falling short to our expectations, the resulting strain (TL101/pDG104/pDG105) only achieved a titer of 177 ± 21.9 mg/L, which was even lower than that of strain BL21/pDG104/pDG105 (Fig. 2a). The yield and productivity of strain TL101/pDG104/pDG105 were 8.9 ± 1.10 mg/g glycerol and 6.3 ± 0.79 mg/L/h (Table 1). Similarly, 205 ± 15.9 mg/L isobutanol and 345 ± 36.2 mg/L isoamylol were measured. Nevertheless, in this study, the strain TL101/pDG104/pDG105 showed poor growth rate due to the large amount of intracellular FABCEs that may have adverse effects on the growth of cells (Additional file 3: Figure S2). When the cell mass was counted by optical cell densities at 600 nm (OD600) with a coefficient of 0.3 gDCW/OD600, the FABCE concentration of strain TL101/pDG104/pDG105 was calculated to be 296 ± 26.8 mg/gDCW (Table 1), which was almost twofold that of strain BL21/pDG104/pDG105 (Fig. 2b). Thus, blocking the β-oxidation pathway could also contribute to the FABCE production if inhibition of cell growth is reduced.
Fig. 2
Fig. 2

Production of FABCEs and branched-chain alcohols in engineered E. coli strains. The GC-MS quantification results showed the FABCE composition of engineered E. coli strains. Methyl pentadecanoic acid was used as the internal standard. Each FABCE was confirmed by corresponding standards that were synthesized by esterification of authentic fatty acid standards and alcohols (Additional file 2). All experiments were performed in triplicate and SD (standard deviation) is indicated. Each color indicates one particular product. a Titer of fatty acid esters and branched-chain alcohols in engineered E. coli strains. b Concentration of fatty acid esters and branched-chain alcohols in engineered E. coli strains when the cell mass was counted by OD600 with a coefficient of 0.3 gDCW/OD600

Incorporation of branched chains into both fatty acid and alcohol modules for expanding ester biosynthesis in E. coli

Because we confirmed that engineered E. coli can produce FABCEs by coupling fatty acyl-CoAs with branched-chain alcohols, we further investigated whether branched chains could be incorporated into fatty acid carbon chains as well. As previously reported, E. coli cannot produce branched fatty acids (BFAs) naturally because the native E. coli β-ketoacyl-ACP synthase III (FabH) can only catalyze the condensation of malonyl-ACP and linear acetyl-CoA or propionyl-CoA in the first step of fatty acid elongation and the substrates required by FabH for production of branched chains are not present in E. coli, either. Fortunately, B. subtilis has a native pathway to supply branched starter substrates and FabH, which can accept branched starter substrates [46, 47].

Consequently, in order to assemble a BFA biosynthetic pathway in E. coli, β-ketoacyl-ACP synthase III (FabHB) and branched-chain α-keto acid dehydrogenase complex (BCKD) from B. subtilis were overexpressed in E. coli. The resulting plasmid pDG110 was then transformed into BL21 (DE3) and TL101, respectively, and cultivated using the same methods as described above. BFAs were extracted by chloroform-methanol (1:1 by v/v) as described earlier [48] and quantitatively analyzed by GC-MS using pentadecanoic acid as an internal standard (Additional file 4: Figure S3A). The recombinant strains BL21/pDG110 and TL101/pDG110 produced BFAs namely 12-methyltetradecanoate, 14-methylpentadecanoate, and 14-methylhexadecanoate. 12-Methyltetradecanoate and 14-methylpentadecanoate were confirmed by their corresponding standard methyl esters, which were synthesized by esterification of BFA standards and methanol (Additional file 5). Besides, 14-methylhexadecanoate which has no available standard was identified by comparing the mass spectrum to that of corresponding standard in the mass spectral libraries and that of similar branched-chain products. The BFA production of strains BL21/pDG110 and TL101/ pDG110 were 17 ± 0.7 and 33 ± 5.4 mg/L, respectively (Fig. 3a). However, these results showed that although the deletion of the fadE gene increased BFA production by 94.1 %, the total BFA production was still very low compared to straight chain fatty acid production.
Fig. 3
Fig. 3

BFA and BFABCE titers in engineered E. coli strains. All experiments were performed in triplicate and SD is indicated. Each color indicated one particular product. a BFA titers in engineered E. coli strains. The total fatty acids were extracted and quantified by GC-MS after esterification with methanol. Pentadecanoic acid was used as the internal standard. 12-Methyltetradecanoate and 14-methylpentadecanoate were confirmed by their corresponding standard methyl esters which were made by esterification of BFA standards and methanol (Additional file 5). 14-Methylhexadecanoate had no available standard and was identified by comparing the mass spectrum to that of corresponding standard in the mass spectral libraries and that of relatively similar branched products. b BFABCE titers in engineered E. coli strains. The BFABCEs were quantified by GC-MS when methyl pentadecanoic acid was used as the internal standard. Except for isobutyl 12-methyltridecanoate, which was identified by comparing the mass spectrum to that of the corresponding standard in the mass spectral libraries, all BFABCEs were identified by the standard made by esterification of the corresponding fatty acid standards and alcohols (Additional file 5)

Because E. coli can produce BFAs using the strategy described above, we hypothesized that E. coli can produce BFABCEs by combining the BFA biosynthetic pathway and the branched-chain amino acid biosynthetic pathway. The plasmids pDG104, pDG105, and pDG110 were transformed into TL101 and cultivated and analyzed in the same way as previously described. The total ion chromatogram (TIC) of BFABCEs is shown in Additional file 4: Figure S3B, and the GC-MS quantification results of BFABCEs are shown in Fig. 3b. Except for isobutyl 12-methyltridecanoate, which was identified by comparing its mass spectrum to that of the corresponding standard in the mass spectral libraries, all BFABCEs were identified using the standard synthesized by the esterification of corresponding fatty acid and alcohols (Additional file 5). The recombinant strain TL101/pDG104/pDG105/pDG110 produced 35 ± 5.7 mg/L BFABCEs with a yield of 1.9 ± 0.28 mg/g glycerol and productivity of 1.3 ± 0.20 mg/L/h. This result indicated that we can incorporate a branched chain into both the fatty acid module and the alcohol module to produce new species of biodiesel with improved performance at low temperatures.

Development of FABCE biosynthesis in P. pastoris

Because the 2-keto acid biosynthetic pathway and the fatty acid biosynthetic pathway naturally exist in various microorganisms, we hypothesized that our FABCE biosynthetic strategy could be applied to other hosts. In fact, several groups have reported the biosynthesis of FAEEs from glucose by engineered S. cerevisiae [25–27, 49, 50]. P. pastoris yeast has been proven to be an excellent system to express various recombinant, heterologous proteins with a high cell density due to low hyper-glycosylation [51]. However, it has not been reported to produce FABCEs. Recently, P. pastoris yeast whole cell catalysts were constructed for biodiesel synthesis with intracellular expression of a lipase [52]. Therefore, we tested our hypothesis by developing a FABCE biosynthetic pathway in P. pastoris. First, we constructed a pDG10 vector for multiple gene expression under the control of GAP promoter. Three genes, aro10, adh2, and ws/dgat, were assembled into pDG10, yielding the plasmid pDG103. Subsequently, pDG103 was linearized and integrated into chromosome of P. pastoris GS115. Then, we cultured the recombinant strain P. pastoris/pDG103 in shake flasks and analyzed the products by GC-MS (Additional file 6: Figure S4). The recombinant strain produced 169 ± 11.7 mg/L of FABCEs (Fig. 4). Similarly, we detected 231 ± 25.4 mg/L of isobutanol and 485 ± 24.6 mg/L of isoamylol.
Fig. 4
Fig. 4

Titer of FABCEs and branched-chain alcohols in engineered P. pastoris yeast. The GC-MS quantification results show the FABCE composition of engineered P. pastoris yeast. Methyl pentadecanoic acid was used as the internal standard. Each FABCE was confirmed by corresponding standards synthesized by esterification of authentic fatty acid standards and alcohols (Additional file 2). All experiments were performed in triplicate, and SD is indicated. Each color indicates one particular product

Discussion

The commonly used biodiesels FAME and FAEE have many unwanted characteristics, especially poor low-temperature properties which can be affected by both fatty acid and alcohol moieties [33]. When methyl is replaced with a branched-chain group such as isobutyl and isoamyl, the resulting FABCEs display lower melting points [32, 35, 53, 54]. FABCEs may have higher energy densities compared with short or medium-chain esters. However, FABCE biosynthesis has not been reported yet. In this work, we provide strategies complementary to other engineering efforts. Specifically, we present de novo biosynthesis of high proportion of FABCEs, including FAIBEs and FAIAEs, by combining the branched-chain amino acid biosynthetic pathway and the fatty acid biosynthetic pathway. Because both fatty acid chain and alcohol portions can affect the low-temperature properties of biodiesels [33], branches were incorporated into fatty acid as well as alcohol chains, successfully generating BFABCEs. E. coli is an ideal host for genetic modification and metabolic engineering. Nevertheless, E. coli is a prokaryotic organism and has some disadvantages for industrial application, so we engineered P. pastoris yeast to produce FABCEs for the first time in order to test the universality of our strategy.

The engineered E. coli strain BL21/pDG104/pDG105 achieved a FABCE production of 273 ± 40.9 mg/L with a high proportion of FABCEs at 99.3 % of total fatty acid ester production (Fig. 2a). In other words, the engineered strain produced an extremely high proportion of FABCEs which can be utilized as advanced biodiesel with better low-temperature properties. The high proportion of FABCEs was most likely achieved due to several reasons. Steinbüchel’s group showed that the enzyme WS/DGAT accepts a broad range of various chain-length alcohols including short-chain alcohols such as ethanol and butanol. However, as reported in their work, the specificity of WS/DGAT toward C4–C8 alcohols was about five times that of ethanol [21]. This finding could explain why FABCEs were the predominant products in this work. Furthermore, besides the higher specificity of WS/DGAT toward C4–C8 alcohols, the overexpression of genes for branched-chain amino acid biosynthesis is another reason for the high proportion of FABCEs because these genes lead to the accumulation of a large amount of branched-chain alcohols such as isobutanol and isoamylol [2, 36–39] which are essential substrates for FABCE production.

On the other hand, when we introduced fabHB and bckd from B. subtilis into E. coli, the production of BFABCEs was only 22 % of all the fatty acid esters. This result can be explained by previous studies: overexpression of fabHB in E. coli results in two FabHs competing for malonyl-ACP [40, 42, 43]. However, the specific activity of E. coli FabH on acetyl-CoA is higher than the activity of B. subtilis FabHB to branched-chain substrates. Moreover, acetyl-CoA is native to E. coli in large amounts, whereas branched-chain substrates for FabHB are difficult to accumulate in E. coli [46, 55].

Because E. coli is not a robust host which is likely to suffer from phages, we presented this capability in P. pastoris yeast. The large amount (169 ± 11.7 mg/L) of FABCEs produced by P. pastoris yeast proved the universality of our strategy and gave us the implication that we can simply apply this strategy to other hosts that might be more potential for FABCE production. Compared with the highest FAEE production (50 mg/L, without precursor supplementation) achieved by S. cerevisiae [27], P. pastoris yeast described in this work indicates that P. pastoris yeast has greater potential to produce biodiesels because not only 32.9 mg/L FAEE but also 169 mg/L FABCEs were produced by P. pastoris yeast (Fig. 4). A potential explanation is that P. pastoris yeast shows superior expression of heterologous proteins [52]. The integration of genes in the chromosome and the use of the powerful GAP promoter also contributed to the high production of FABCEs by P. pastoris yeast. Because these strategies provide a more stable and efficient system, for example, in Nielsen’s work, the integration of genes results in a sixfold increase compared to the equivalent plasmid-based production in S. cerevisiae [27]. Above all, branched-chain alcohols with C4–C5 carbons are better substrates to WS/DGAT than ethanol [21, 56].

However, for both E. coli and S. cerevisiae, the titers are still below commercial levels, and further work will be necessary. Previous studies [57, 58], in which a specific residue was modified in WS/DGAT, show an increasing selectivity toward shorter chain fatty alcohol substrates, and this supports the potential for future efforts to improve the selectivity of WS/DGAT toward branched-chain alcohols by tailoring and modifying the enzyme WS/DGAT. Of course, studies focusing on finding more specific enzymes are also needed. The present work indicates that the bottleneck in FABCE production is the low proportion of fatty acyl-CoAs. However, this difficulty exists worldwide, and it might be alleviated by in vitro reconstitution [17] and modified enzymes used in the fatty acid biosynthesis pathway through rational protein design, as well as improved fatty acyl-CoAs supply. In addition, the universality of the present results indicates that other hosts might have greater potential for FABCE production, such as oleaginous yeast, which can accumulate a large amount of lipids [59].

Conclusions

Several approaches to the low-temperature problems of biodiesels have been investigated including blending with conventional diesel fuel, winterization, and additives; this work provides a new strategy to solve the poor cold-flow performance of currently used biodiesels [33, 60]. The combination of the fatty acid biosynthetic pathway and the branched-chain amino acid biosynthetic pathway achieved a high proportion of FABCEs with improved low-temperature properties and high energy densities. The biosynthesis of FABCEs in both E. coli and P. pastoris proved the universality of our strategy although more work is needed to reach the level of commercialization. Nevertheless, using an approach that generates high proportions of FABCEs, the low-temperature performance of conventional biodiesels can be optimized. Our strategy can provide a start point for engineering more appropriate hosts to produce advanced biodiesels.

Methods

Materials

Restriction enzymes, Phusion polymerase, and Taq ligase were purchased from New England Biolabs (Beverly, MA, USA), and T5 exonuclease was purchased from Epicenter Biotechnologies (Madison, WI, USA). Plasmid miniprep kits, PCR purification kits, and gel extraction kits were purchased from Axygen (Alameda, CA, USA). All primers were synthesized by GENEWIZ (Suzhou, China). Fatty acid standards were purchased from TCI (Shanghai, China), and all the other reagents were purchased from Sigma-Aldrich (St. Louis, MO, USA).

Plasmid and strain construction

Table 2 shows all plasmids used in this study. The sequences of all primers used in PCRs are listed in Table 3. The sequences of synthesized genes are listed in Additional file 7.
Table 2

Plasmids used in this study

Plasmids

Replication origin

Overexpressed genes

Resistance

Reference

pDG16

pBR322

PT7: alsS

Kan

This study

pDG17

pBR322

PT7: ilvC

Kan

This study

pDG18

pBR322

PT7: ilvD

Kan

This study

pDG19

pBR322

PT7: ilvC and ilvD

Kan

This study

pDG20

pBR322

PT7: alsS, ilvC, and ilvD

Kan

This study

pDG102

pBR322

PT7: aro10, adh2, ws/dgat, and fadD

Kan

Reference [31]

pDG104

pBR322

PT7: ws/dgat, aro10, adh2, fadD, alsS, ilvC, and ilvD

Kan

This study

pTL30

pBR322

PT7: tesA’

Kan

Reference [14]

pXC002

pSC101

PT7

Amp

Not published

pDG105

pSC101

PT7: tesA’

Amp

This study

pDG25

pBBR1

PT7: bckd

Cam

This study

pDG110

pBBR1

PT7: fabHB and bckd

Cam

This study

pDG10

pBR322

PGAP: his4

G418 and His

This study

pDG11

pBR322

PGAP: ws/dgat

G418

This study

pDG12

pBR322

PGAP: aro10

G418

This study

pDG13

pBR322

PGAP: adh2

G418

This study

pDG14

pBR322

PGAP: ws/dgat

G418 and His

This study

pDG15

pBR322

PGAP: ws/dgat and aro10

G418 and His

This study

pDG103

pBR322

PGAP: ws/dgat, aro10, and adh2

G418 and His

This study

Table 3

Primers used for PCR amplification of genes

Primer name

Primer sequence (5′-3′)

ilvC-XbaI

GTATCTAGAAAGAGGAGATATAATGGCTAACTACTTCAATACACTGAATCTG

ilvC-SpeI-BamHI

ACTGGATCCACTAGTTTAACCCGCAACAGCAATACGTT

ilvD-XbaI

GTATCTAGAAAGAGGAGATATAATGCCTAAGTACCGTTCCGCCA

ilvD-SpeI-BamHI

ACTGGATCCACTAGTTTAACCCCCCAGTTTCGATTTATCG

BCKD-SacI

AGATGAGCTCATGGCAACTGAGTATGACGTAGTCATTC

BCKD-SpeI

AGTACTAGTTTAGTAAACAGATGTCTTCTCGTCAATCG

fabHB-BamHI

ACTGGATCCAAGAAGGAGATATAATGTCAAAAGCAAAAATTACAGCTATCGG

fabHB-XhoI

TGTCTCGAGTTACATCCCCCATTTAATAAGCAATCCTG

WS/DGAT-SfuI

AGGTTTCGAAATGAGACCATTACACCCTATTGATTTC

WS/DGAT-EcoRI

GACGAATTCTTAGTTGGCAGTCTTAATGTCTTCTTG

HIS4-BamHI

AATGGATCCCTCGCAGCTGATGAATATCTTGTG

HIS4-BglII

CAAGGATCCACCGATACCAGGATCTTGCCAT

ARO10-SfuI

GCGTTCGAAATGGCACCTGTTACAATTGAAAAGTTC

ARO10-EcoRI

CCGTCTAGACTATTTTTTATTTCTTTTAAGTGCCGCTG

ADH2-SfuI

CCGTTCGAAATGTCTATTCCAGAAACTCAAAAAGCC

ADH2-EcoRI

GCGGAATTCTTATTTAGAAGTGTCAACAACGTATCTACCAG

Plasmids for FAIBE and FAIAE production

The alsS gene [GenBank: 936852] from B. subtilis was synthesized using GenScript (Nanjing, China) with the sequence of the ribosome binding site (rbs) and cloned into the XbaI-BamHI sites of the plasmid pET28a (+), yielding pDG16. The ilvC [GenBank: 948286] and ilvD [GenBank: 948277] genes were amplified from E. coli genomic DNA with primers ilvC-XbaI/ilvC-SpeI-BamHI and ilvD-XbaI/ilvD-SpeI-BamHI, and the PCR products were cloned into pET28a (+), yielding pDG17 and pDG18, respectively. The XbaI-SalI fragment from pDG17 was cloned into pDG18 yielding pDG19. Subsequently, the XbaI-SalI fragment of pDG19 was cloned into pDG16 yielding pDG20. The XbaI-SalI fragment of pDG20 was cloned into the NheI-XhoI sites of pDG102 [31], yielding pDG104. The truncated tesA’ gene [GenBank: 945127] from pTL30 [14] was cloned under the control of T7 promoter of pXC002 with a pSC101 replication origin, yielding pDG105.

Plasmids for BFA production

The bckd [GenBank: CP010052] and fabHB [GenBank: 939306] genes were amplified from B. subtilis genomic DNA with the primers fabHB-BamHI/fabHB-XhoI and BCKD-SacI/BCKD-SpeI. The bckd fragment was inserted into the SacI-SpeI sites of pBBR1MCS1, yielding pDG25. The PCR fragment of the fabHB gene was digested by SacI-SpeI and inserted into the BamHI-XhoI sites of pDG25, yielding pDG110.

Plasmids for FABCE production in P. pastoris

First, a constitutive expression vector that can express multiple genes under the control of GAP promoter in P. pastoris was constructed as follows: The his4 gene [GenBank: 850327] was amplified from the plasmid pPIC3.5k with the primers HIS4-BamHI and HIS4-BglII. The PCR fragment was inserted into the BamHI site of pGAPZα A, yielding pDG10, which can constitutively overexpress multiple genes in P. pastoris. Then, the synthesized ws/dgat gene [GenBank: 5984342] was amplified with the primers WS/DGAT-SfuI/WS/DGAT-EcoRI and cloned into the SfuI-EcoRI sites of pGAPZα A, yielding pDG11. The aro10 [GenBank: 851987] and adh2 [GenBank: 855349] genes from S. cerevisiae YPH499, coding 2-keto acid decarboxylase and alcohol dehydrogenase, were amplified from genomic DNA with the primers ARO10-SfuI/ARO10-EcoRI and ADH2-SfuI/ADH2-EcoRI and cloned into the SfuI-EcoRI sites of pGAPZα A, yielding pDG12 and pDG13, respectively. The BamHI-BglII fragment from pDG11 was inserted into the BamHI site of pDG10, resulting in the plasmid pDG14. Similarly, the BamHI-BglII fragment from pDG12 was inserted into the BamHI site of pDG14, yielding pDG15. A similar strategy was used to clone the adh2 gene into pDG15, yielding pDG103.

Shake-flask cultures

Table 4 shows all the strains used in this study. For E. coli, the corresponding plasmids were transformed into BL21 (DE3) or TL101 competent cells with suitable antibiotics, respectively, and several single colonies were pre-cultivated in a 10 mL LB medium in 50-mL flasks with proper antibiotics at 30 °C for 12 h. Cells were collected and resuspended with 100 mL modified M9 medium as described previously [31] in 500-mL flasks and shaken in a rotary shaker at 220 rpm and 30 °C. When OD600 reached 0.8, IPTG was added to a final concentration of 0.1 mM. Cells were harvested 28 h after induction. All experiments were performed in triplicate. For P. pastoris, pDG103 was linearized using SacI and transformed into competent cells of P. pastoris GS115 via electroporation. The positive transformants harboring chromosomal integration of ws/dgat, adh2, and aro10 expression cassettes were preliminarily selected on SC-His plates supplemented with G418. Single colonies of harboring expression cassettes were used to inoculate 10 ml YPD medium in 50-mL flasks at 30 °C for 12 h. Cells were collected and resuspended with 100 mL YPD medium in 500-mL flasks and shaken in a rotary shaker at 220 rpm and 30 °C. Cells were harvested after 28 h. All experiments were performed in triplicate.
Table 4

Strains used in this study

Strains

Description

Reference

BL21(DE3)

E. coli B dcm ompT hsdS(r B ˉm B ˉ)gal

Invitrogen

TL101

E. coli BL21(DE3): ΔfadE

Reference [17]

BL21/pDG104

BL21(DE3) derivative;{pDG104}

This study

BL21/pDG104/pDG105

BL21(DE3) derivative;{pDG104, pDG105}

This study

TL101/pDG104/pDG105

BL21(ΔfadE) derivative;{pDG104, pDG105}

This study

BL21/pDG110

BL21(DE3) derivative;{pDG110}

This study

TL101/pDG110

BL21(ΔfadE) derivative;{pDG110}

This study

TL101/pDG104/pDG105/pDG110

BL21(ΔfadE) derivative;{pDG104, pDG105, pDG110}

This study

GS115

his4, Mut +

Biovector

P. pastoris/pDG103

GS115 derivative;{pDG103}

This study

Analysis methods

GC-MS analysis of fatty acid esters and branched-chain alcohols

Fatty acid esters were extracted using a previously published method [31]. GC-MS analysis of fatty acid esters dissolved in hexane phase was performed and quantified using a TRACE Ultra gas chromatograph connected to a TSQ Quantum XLS triple quadrupole mass spectrometer (GC-MS, Thermo Scientific Inc., San Jose, CA, USA). The hexane phase was analyzed on a TR-WAXMS capillary column (30 m × 0.25 mm × 0.25 μm), following a 1-μL injection with an auto-sampler (AI/AS 3000). Injections were performed in split mode with a split ratio of 20:1. Helium was used as the carrier gas with a flow rate of 1 mL/min. The inject inlet and ion source temperatures were 220 and 240 °C, respectively. The temperature sequence was programmed as follows: 100 °C as an initial temperature for 5 min, then a 6 °C/min ramp to 240 °C, held at 240 °C for 10 min. For identification of fatty acid esters, each fatty acid ester standard was synthesized by esterification of individual fatty acids with corresponding alcohols. For quantification, methyl pentadecanoic acid was used as an internal standard in all samples.

The branched-chain alcohol content of the shake-flask samples was extracted by hexane and analyzed by GC-MS as described previously [31]. Authentic standards were used to quantify isobutanol and isoamylol.

Abbreviations

ACP: 

Acyl carrier protein

BFAs: 

Branched fatty acids

BCKD: 

Branched-chain α-keto acid dehydrogenase complex

BFABCEs: 

Branched fatty acid branched-chain esters

CoA: 

Coenzyme A

DCW: 

Dry cell weight

FABCEs: 

Fatty acid branched-chain esters

FabH: 

β-ketoacyl-ACP synthase III

FAEEs: 

Fatty acid ethyl esters

FAIAEs: 

Fatty acid isoamyl esters

FAIBEs: 

Fatty acid isobutyl esters

FAME: 

Fatty acid methyl ester

FASEs: 

Fatty acid short-chain esters

GC-MS: 

Gas chromatography–mass spectrometry

IPTG: 

Isopropyl β-d-thiogalactopyranoside

LB: 

Luria-Bertani

rbs: 

Ribosome binding site

OD600 : 

Optical cell densities at 600 nm

TIC: 

Total ion chromatogram

WS/DGAT: 

Wax ester synthase

YPD: 

Yeast extract peptone dextrose medium

Declarations

Acknowledgements

This research was supported by grants from the 863 (2012AA02A701) and 973 (2011CBA00800, 2012CB721000) Project from the Ministry of Science and Technology of China and the National Natural Science Foundation of China (31170096, 31222002), as well as the Project supported by Science and Technology Department of Hubei Province and by J1 Biotech Co. Ltd. (2014091610010595).

Authors’ Affiliations

(1)
Key Laboratory of Combinatorial Biosynthesis and Drug Discovery, Ministry of Education and Wuhan University School of Pharmaceutical Sciences, Wuhan, 430071, China
(2)
Hubei Engineering Laboratory for Synthetic Microbiology, Wuhan Institute of Biotechnology, Wuhan, 430075, China
(3)
State Key Laboratory of Microbial Metabolism, School of Life Sciences and Biotechnology, Shanghai Jiao Tong University, 800 Dongchuan Road, Shanghai, 200240, China
(4)
Hubei Provincial Cooperative Innovation Center of Industrial Fermentation, Wuhan, 430068, China

References

  1. Hill J, Nelson E, Tilman D, Polasky S, Tiffany D. Environmental, economic, and energetic costs and benefits of biodiesel and ethanol biofuels. Proc Natl Acad Sci U S A. 2006;103:11206–10. doi:10.1073/pnas.0604600103.View ArticleGoogle Scholar
  2. Atsumi S, Liao JC. Metabolic engineering for advanced biofuels production from Escherichia coli. Curr Opin Biotechnol. 2008;19:414–9. doi:10.1016/j.copbio.2008.08.008.View ArticleGoogle Scholar
  3. Peralta-Yahya PP, Zhang F, Del Cardayre SB, Keasling JD. Microbial engineering for the production of advanced biofuels. Nature. 2012;488:320–8. doi:10.1038/nature11478.View ArticleGoogle Scholar
  4. Dunn RO, Knothe G. Alternative diesel fuels from vegetable oils and animal fats. J Oleo Sci. 2001;50:415–26.View ArticleGoogle Scholar
  5. Knothe G, Matheaus AC, Ryan III TW. Cetane numbers of branched and straight-chain fatty esters determined in an ignition quality tester. Fuel. 2003;82:971–5.View ArticleGoogle Scholar
  6. Steen EJ, Kang Y, Bokinsky G, Hu Z, Schirmer A, McClure A, et al. Microbial production of fatty-acid-derived fuels and chemicals from plant biomass. Nature. 2010;463:559–62. doi:10.1038/nature08721.View ArticleGoogle Scholar
  7. Janßen HJ, Steinbüchel A. Fatty acid synthesis in Escherichia coli and its applications towards the production of fatty acid based biofuels. Biotechnol Biofuels. 2014;7:7.View ArticleGoogle Scholar
  8. Zhang F, Rodriguez S, Keasling JD. Metabolic engineering of microbial pathways for advanced biofuels production. Curr Opin Biotechnol. 2011;22:775–83. doi:10.1016/j.copbio.2011.04.024.View ArticleGoogle Scholar
  9. De Jong B, Siewers V, Nielsen J. Systems biology of yeast: enabling technology for development of cell factories for production of advanced biofuels. Curr Opin Biotechnol. 2012;23:624–30. doi:10.1016/j.copbio.2011.11.021.View ArticleGoogle Scholar
  10. Nielsen J, Larsson C, van Maris A, Pronk J. Metabolic engineering of yeast for production of fuels and chemicals. Curr Opin Biotechnol. 2013;24:398–404. doi:10.1016/j.copbio.2013.03.023.View ArticleGoogle Scholar
  11. Liu Q, Wu K, Cheng Y, Lu L, Xiao E, Zhang Y, et al. Engineering an iterative polyketide pathway in Escherichia coli results in single-form alkene and alkane overproduction. Metab Eng. 2015;28:82–90.View ArticleGoogle Scholar
  12. Li X, Guo D, Cheng Y, Zhu F, Deng Z, Liu T. Overproduction of fatty acids in engineered Saccharomyces cerevisiae. Biotechnol Bioeng. 2014;111:1841–52. doi:10.1002/bit.25239.View ArticleGoogle Scholar
  13. Lu X, Vora H, Khosla C. Overproduction of free fatty acids in E. coli: implications for biodiesel production. Metab Eng. 2008;10:333–9. doi:10.1016/j.ymben.2008.08.006.View ArticleGoogle Scholar
  14. Liu T, Vora H, Khosla C. Quantitative analysis and engineering of fatty acid biosynthesis in E. coli. Metab Eng. 2010;12:378–86. doi:10.1016/j.ymben.2010.02.003.View ArticleGoogle Scholar
  15. Ruffing AM, Jones HD. Physiological effects of free fatty acid production in genetically engineered Synechococcus elongatus PCC 7942. Biotechnol Bioeng. 2012;109:2190–9.View ArticleGoogle Scholar
  16. Handke P, Lynch SA, Gill RT. Application and engineering of fatty acid biosynthesis in Escherichia coli for advanced fuels and chemicals. Metab Eng. 2011;13:28–37. doi:10.1016/j.ymben.2010.10.007.View ArticleGoogle Scholar
  17. Yu X, Liu T, Zhu F, Khosla C. In vitro reconstitution and steady-state analysis of the fatty acid synthase from Escherichia coli. Proc Natl Acad Sci. 2011;108:18643–8.View ArticleGoogle Scholar
  18. Dellomonaco C, Clomburg JM, Miller EN, Gonzalez R. Engineered reversal of the beta-oxidation cycle for the synthesis of fuels and chemicals. Nature. 2011;476:355–9. doi:10.1038/nature10333.View ArticleGoogle Scholar
  19. Xu P, Gu Q, Wang W, Wong L, Bower AG, Collins CH, et al. Modular optimization of multi-gene pathways for fatty acids production in E coli. Nat Commun. 2013;4:1409. doi:10.1038/ncomms2425.View ArticleGoogle Scholar
  20. Kalscheuer R, Uthoff S, Luftmann H, Steinbüchel A. In vitro and in vivo biosynthesis of wax diesters by an unspecific bifunctional wax ester synthase/acyl-CoA:diacylglycerol acyltransferase from acinetobacter Calcoaceticus ADP1. Eur J Lipid Sci Technol. 2003;105:578–84. doi:10.1002/ejlt.200300840.View ArticleGoogle Scholar
  21. Stöveken T, Kalscheuer R, Malkus U, Reichelt R, Steinbüchel A. The wax ester synthase/acyl coenzyme A: diacylglycerol acyltransferase from Acinetobacter sp. strain ADP1: characterization of a novel type of acyltransferase. J Bacteriol. 2005;187:1369–76. doi:10.1128/JB.187.4.1369-1376.2005.View ArticleGoogle Scholar
  22. Kalscheuer R, Stolting T, Steinbüchel A. Microdiesel: Escherichia coli engineered for fuel production. Microbiology. 2006;152:2529–36. doi:10.1099/mic.0.29028-0.View ArticleGoogle Scholar
  23. Duan Y, Zhu Z, Cai K, Tan X, Lu X. De novo biosynthesis of biodiesel by Escherichia coli in optimized fed-batch cultivation. PLoS ONE. 2011;6, e20265. doi:10.1371/journal.pone.0020265.View ArticleGoogle Scholar
  24. Zhang F, Carothers JM, Keasling JD. Design of a dynamic sensor-regulator system for production of chemicals and fuels derived from fatty acids. Nat Biotechnol. 2012;30:354–9. doi:10.1038/nbt.2149.View ArticleGoogle Scholar
  25. Thompson RA, Trinh CT. Enhancing fatty acid ethyl ester production in Saccharomyces cerevisiae through metabolic engineering and medium optimization. Biotechnol Bioeng. 2014;111:2200–8. doi:10.1002/bit.25292.View ArticleGoogle Scholar
  26. Shi S, Valle-Rodriguez JO, Khoomrung S, Siewers V, Nielsen J. Functional expression and characterization of five wax ester synthases in Saccharomyces cerevisiae and their utility for biodiesel production. Biotechnol Biofuels. 2012;5:7. doi:10.1186/1754-6834-5-7.View ArticleGoogle Scholar
  27. Shi S, Valle-Rodriguez JO, Siewers V, Nielsen J. Engineering of chromosomal wax ester synthase integrated Saccharomyces cerevisiae mutants for improved biosynthesis of fatty acid ethyl esters. Biotechnol Bioeng. 2014;111:1740–7. doi:10.1002/bit.25234.View ArticleGoogle Scholar
  28. Rodriguez GM, Tashiro Y, Atsumi S. Expanding ester biosynthesis in Escherichia coli. Nat Chem Biol. 2014;10:259–65. doi:10.1038/nchembio.1476.View ArticleGoogle Scholar
  29. Layton DS, Trinh CT. Engineering modular ester fermentative pathways in Escherichia coli. Metab Eng. 2014;26C:77–88. doi:10.1016/j.ymben.2014.09.006.View ArticleGoogle Scholar
  30. Tai YS, Xiong M, Zhang K. Engineered biosynthesis of medium-chain esters in Escherichia coli. Metab Eng. 2015;27:20–8. doi:10.1016/j.ymben.2014.10.004.View ArticleGoogle Scholar
  31. Guo D, Zhu J, Deng Z, Liu T. Metabolic engineering of Escherichia coli for production of fatty acid short-chain esters through combination of the fatty acid and 2-keto acid pathways. Metab Eng. 2014;22:69–75. doi:10.1016/j.ymben.2014.01.003.View ArticleGoogle Scholar
  32. Lee I, Johnson LA, Hammond EG. Use of branched-chain esters to reduce the crystallization temperature of biodiesel. J Am Oil Chem Soc. 1995;72:1155–60.View ArticleGoogle Scholar
  33. Knothe G. Dependence of biodiesel fuel properties on the structure of fatty acid alkyl esters. Fuel Process Technol. 2005;86:1059–70. doi:10.1016/j.fuproc.2004.11.002.View ArticleGoogle Scholar
  34. Knothe G. Improving biodiesel fuel properties by modifying fatty ester composition. Energy Environ Sci. 2009;2:759. doi:10.1039/b903941d.View ArticleGoogle Scholar
  35. Dunn R, Bagby M. Low-temperature properties of triglyceride-based diesel fuels: transesterified methyl esters and petroleum middle distillate/ester blends. J Am Oil Chem Soc. 1995;72:895–904.View ArticleGoogle Scholar
  36. Atsumi S, Hanai T, Liao JC. Non-fermentative pathways for synthesis of branched-chain higher alcohols as biofuels. Nature. 2008;451:86–9. doi:10.1038/nature06450.View ArticleGoogle Scholar
  37. Connor MR, Liao JC. Engineering of an Escherichia coli strain for the production of 3-methyl-1-butanol. Appl Environ Microbiol. 2008;74:5769–75. doi:10.1128/AEM.00468-08.View ArticleGoogle Scholar
  38. Cann AF, Liao JC. Production of 2-methyl-1-butanol in engineered Escherichia coli. Appl Microbiol Biotechnol. 2008;81:89–98. doi:10.1007/s00253-008-1631-y.View ArticleGoogle Scholar
  39. Atsumi S, Wu TY, Eckl EM, Hawkins SD, Buelter T, Liao JC. Engineering the isobutanol biosynthetic pathway in Escherichia coli by comparison of three aldehyde reductase/alcohol dehydrogenase genes. Appl Microbiol Biotechnol. 2010;85:651–7. doi:10.1007/s00253-009-2085-6.View ArticleGoogle Scholar
  40. Howard TP, Middelhaufe S, Moore K, Edner C, Kolak DM, Taylor GN, et al. Synthesis of customized petroleum-replica fuel molecules by targeted modification of free fatty acid pools in Escherichia coli. Proc Natl Acad Sci. 2013;110:7636–41.View ArticleGoogle Scholar
  41. Haushalter RW, Kim W, Chavkin TA, The L, Garber ME, Nhan M, et al. Production of anteiso-branched fatty acids in Escherichia coli; next generation biofuels with improved cold-flow properties. Metab Eng. 2014;26C:111–8. doi:10.1016/j.ymben.2014.09.002.View ArticleGoogle Scholar
  42. Jiang W, Jiang Y, Bentley GJ, Liu D, Xiao Y, Zhang F. Enhanced production of branched‐chain fatty acids by replacing β‐ketoacyl‐(acyl‐carrier‐protein) synthase III (FabH). Biotechnol Bioeng. 2015. doi:10.1002/bit.25583.Google Scholar
  43. Cho H, Cronan JE. Defective export of a periplasmic enzyme disrupts regulation of fatty acid synthesis. J Biol Chem. 1995;270:4216–9.View ArticleGoogle Scholar
  44. Zhang X, Li M, Agrawal A, San KY. Efficient free fatty acid production in Escherichia coli using plant acyl-ACP thioesterases. Metab Eng. 2011;13:713–22. doi:10.1016/j.ymben.2011.09.007.View ArticleGoogle Scholar
  45. Zheng Y, Li L, Liu Q, Qin W, Yang J, Cao Y, et al. Boosting the free fatty acid synthesis of Escherichia coli by expression of a cytosolic Acinetobacter baylyi thioesterase. Biotechnol Biofuels. 2012;5:76–88.View ArticleGoogle Scholar
  46. Choi K-H, Heath RJ, Rock CO. β-ketoacyl-acyl carrier protein synthase III (FabH) is a determining factor in branched-chain fatty acid biosynthesis. J Bacteriol. 2000;182:365–70.View ArticleGoogle Scholar
  47. Kaneda T. Fatty acids of the genus Bacillus: an example of branched-chain preference. Bacteriol Rev. 1977;41:391.Google Scholar
  48. Voelker TA, Davies HM. Alteration of the specificity and regulation of fatty acid synthesis of Escherichia coli by expression of a plant medium-chain acyl-acyl carrier protein thioesterase. J Bacteriol. 1994;176:7320–7.Google Scholar
  49. Runguphan W, Keasling JD. Metabolic engineering of Saccharomyces cerevisiae for production of fatty acid-derived biofuels and chemicals. Metab Eng. 2014;21:103–13. doi:10.1016/j.ymben.2013.07.003.View ArticleGoogle Scholar
  50. Valle-Rodríguez JO, Shi S, Siewers V, Nielsen J. Metabolic engineering of Saccharomyces cerevisiae for production of fatty acid ethyl esters, an advanced biofuel, by eliminating non-essential fatty acid utilization pathways. Appl Energy. 2014;115:226–32. doi:10.1016/j.apenergy.2013.10.003.View ArticleGoogle Scholar
  51. Macauley-Patrick S, Fazenda ML, McNeil B, Harvey LM. Heterologous protein production using the Pichia pastoris expression system. Yeast. 2005;22:249–70. doi:10.1002/yea.1208.View ArticleGoogle Scholar
  52. Yan J, Zheng X, Du L, Li S. Integrated lipase production and in situ biodiesel synthesis in a recombinant Pichia pastoris yeast: an efficient dual biocatalytic system composed of cell free enzymes and whole cell catalysts. Biotechnol Biofuels. 2014;7:55.View ArticleGoogle Scholar
  53. Foglia TA, Nelson LA, Dunn RO, Marmer WN. Low-temperature properties of alkyl esters of tallow and grease. J Am Oil Chem Soc. 1997;74:951–5.View ArticleGoogle Scholar
  54. Zhang Y, Van Gerpen JH. Combustion analysis of esters of soybean oil in a diesel engine: SAE Technical Paper 1996. doi:10.4271/960765Google Scholar
  55. Bennett BD, Kimball EH, Gao M, Osterhout R, Van Dien SJ, Rabinowitz JD. Absolute metabolite concentrations and implied enzyme active site occupancy in Escherichia coli. Nat Chem Biol. 2009;5:593–9. doi:10.1038/nchembio.186.View ArticleGoogle Scholar
  56. Stöveken T, Steinbüchel A. Bacterial acyltransferases as an alternative for lipase-catalyzed acylation for the production of oleochemicals and fuels. Angew Chem Int Ed. 2008;47:3688–94. doi:10.1002/anie.200705265.View ArticleGoogle Scholar
  57. Wältermann M, Stöveken T, Steinbüchel A. Key enzymes for biosynthesis of neutral lipid storage compounds in prokaryotes: properties, function and occurrence of wax ester synthases/acyl-CoA: diacylglycerol acyltransferases. Biochimie. 2007;89:230–42. doi:10.1016/j.biochi.2006.07.013.View ArticleGoogle Scholar
  58. Barney BM, Mann RL, Ohlert JM. Identification of a residue affecting fatty alcohol selectivity in wax ester synthase. Appl Environ Microbiol. 2013;79:396–9. doi:10.1128/AEM.02523-12.View ArticleGoogle Scholar
  59. Li Y, Zhao Z, Bai F. High-density cultivation of oleaginous yeast Rhodosporidium toruloides Y4 in fed-batch culture. Enzyme Microb Technol. 2007;41:312–7. doi:10.1016/j.enzmictec.2007.02.008.View ArticleGoogle Scholar
  60. Moser BR. Biodiesel production, properties, and feedstocks. Vitro Cell Dev Biol Plant. 2009;45:229–66. doi:10.1007/s11627-009-9204-z.View ArticleGoogle Scholar

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