- Open Access
Co-production of single cell oil and gluconic acid using oleaginous Cryptococcus podzolicus DSM 27192
Biotechnology for Biofuels volume 12, Article number: 127 (2019)
The co-production of single cell oil (SCO) with value-added products could improve the economic viability of industrial SCO production. The newly isolated oleaginous yeast Cryptococcus podzolicus DSM 27192 was able to co-produce SCO intracellularly and gluconic acid (GA) extracellularly. In this study, the metabolic regulation of carbon distribution between SCO and GA through process optimization was comprehensively investigated.
The carbon flow distribution between SCO and GA was significantly influenced by the cultivation conditions, such as nitrogen sources, glucose concentration and dissolved oxygen concentration. It was found that organic nitrogen sources were beneficial for SCO accumulation, while GA production was decreased. Dissolved oxygen concentration (DOC) was found to enhance SCO accumulation, while high glucose concentration was more favorable for GA accumulation. Hence, a two-stage DOC or glucose concentration-controlled strategy was designed to improve cell growth and direct carbon distribution between SCO and GA. Moreover, C. podzolicus DSM 27192 could degrade its stored lipids to synthesize GA in the late stationary phase, although considerable amounts of glucose remained unconsumed in the culture medium, indicating the importance of fermentation time control in co-production systems. All these observations provide opportunity to favor either the production of SCO or GA or rather their simultaneous production.
Co-production of SCO and GA by C. podzolicus DSM 27192 can improve the economical value for microbial lipid-derived biodiesel production. Moreover, the results of the proposed co-production strategy might give guidance for other co-production systems.
Driven by the foreseeable depletion of crude oil and the highly controversial “food-or-fuel” discussion regarding plant-based biodiesel production, single cell oil (SCO) has been considered as an intriguing alternative for biodiesel production and oleochemical industries . To unlock the economical competitiveness of SCO hindered by its relatively high production cost and low yield [2, 3], many efforts have been made on the utilization of low-cost feedstocks, optimization of fermentation conditions and genetic modification of lipid synthesis pathways in microbes [4,5,6]. However, the improvement is still limited, as the lipid yield and productivity are still too low [7,8,9,10]. Currently, the practical yield of SCO from glucose is only ~ 0.22 g lipid/g glucose, since high amounts of carbon are used for the production of biomass and other metabolites .
The production of some metabolites is inevitable for the maintenance of metabolism; alternatively, an effective co-production system may be more beneficial than the repression or deletion of genes related to by-products synthesis, as it may prevent metabolic imbalances . In addition, the co-production of the main metabolic products, e.g., SCO with value-added chemicals, may make full use of nutrients in the cultivation medium, improving the techno-economics of microbial lipid technology . Successful precedents have been established for the co-production of PHA with proteins, alcohols and biosurfactants ; β-galactosidase with ethanol ; erythritol with lipase ; lactic acid with chitin , etc. Currently, a number of co-production systems of SCO with other chemicals have also been reported, most of which have focused on the co-production with bioethanol , proteins  and some liposoluble products, such as carotenoid, fucoxanthin and pigments [20,21,22]. However, only little attention has been paid to the co-production of SCO with other bulk chemicals.
In our previous study, the oleaginous yeast Cryptococcus podzolicus DSM 27192 was isolated and identified. Preliminary fermentation results showed that it can accumulate high amounts of gluconic acid (GA) as a by-product when growing on glucose . GA (C6H12O7) is an oxidation product of glucose, which has been widely used in the food, medicine and cement industries for over 50 years [24, 25]. Especially, the favorable effects of GA on human and animal health have boosted its use as a prebiotic in food production recently . Due to its multiple applications in different aspects, the demand for GA has been steadily increasing globally. At present, the production of GA and its derivatives has been estimated to be approximately 60,000 ton/year, with production costs ranging from 1.20 to 8.50 US$/kg, which restricts its application in many cases . Hence, developing an effective and economically viable system for GA production is urgent.
In this study, the co-production of SCO and GA by using C. podzolicus DSM 27192 was investigated. The influence of nitrogen source, dissolved oxygen, glucose concentration as well as fermentation time on the production of SCO and GA was comprehensively analyzed. Furthermore, biochemical and technological considerations concerning the microbial behavior were assessed and critically discussed, which will provide more guidance for further lipid co-production strategies.
Results and discussion
According to literature, the production of GA and SCO is mainly influenced by three factors: (1) an excess of carbon; (2) nutrient limitation, e.g., nitrogen limitation; and (3) continuous aeration to ensure sufficient supply with oxygen. Therefore, these parameters were investigated accordingly [11, 24].
Regulation of carbon flow between SCO and GA using different nitrogen sources
It is known that cell growth and distribution of metabolites are strongly affected by nitrogen sources during microbial fermentation . In a previous shake flask study, SCO accumulation in C. podzolicus DSM 27192 was found to be similar in both YM and mineral salt medium. Furthermore, 1.8 g/L of GA was produced in mineral salt medium, while no GA was detected in YM medium (data not shown). A major difference between these two media was the nitrogen source. To further explore the effect of nitrogen sources on carbon flow distribution, different nitrogen sources including (NH4)2SO4, YM-based nitrogen (peptone, yeast extract and malt extract) and yeast extract were investigated in bioreactor experiments to ensure optimal aeration and pH control. To be able to compare the influence of different nitrogen sources, the C/N ratio was kept similar in all experiments as described by Li et al.  and Bellou et al. .
As shown in Fig. 1a, when (NH4)2SO4 was used as the nitrogen source, 17.5 g/L of GA was produced by C. podzolicus DSM 27192, while considerably lower GA concentrations of 4.8 g/L, 4.6 g/L and 6.0 g/L were obtained in YM-based nitrogen, yeast extract medium and YM medium, respectively, suggesting a possible inhibition of organic nitrogen sources on GA production in contrast to inorganic ones. However, yeast extract is a complex mixture of nitrogenous compounds, carbon, sulfur, trace nutrients, vitamin B complex and other important growth factors. Thus, it is difficult to conclude which element(s) resulted in this phenomenon. In a previous study, some metals such as Cu2+ and Fe2+ in yeast extract have been reported to repress key enzyme activities, such as glucose oxidase (GO) in the GA production pathway [31,32,33]. However, the results are inconsistent with other studies, in which organic nitrogen sources, such as peptone and yeast extract, were found to have a stimulating effect on GO activity .
In terms of SCO production, organic nitrogen sources, such as yeast extract, were found to be favorable to improve the lipid content, since 49.9% and 39.6% were obtained in YM-based nitrogen and yeast extract medium, respectively. 40.1% was obtained by using YM medium, while a slightly lower lipid content of 36.3% was produced in (NH4)2SO4 medium (Fig. 1b). However, when (NH4)2SO4 was used as the nitrogen source, the highest biomass production (40.6 g/L) was detected (Fig. 1c), while YM medium, YM-based nitrogen and yeast extract medium resulted in 22.4 g/L, 18.6 g/L, and 24.3 g/L of cell mass, respectively. These results imply that inorganic and organic nitrogen play different roles in biomass production and lipid accumulation in the fermentation process, and that inorganic nitrogen sources are more beneficial for biomass accumulation, but less suitable for SCO production, while organic nitrogen sources improve lipid accumulation, but are less suitable for cell growth. These findings are consistent with the results reported by Bellou et al. . Specifically, by measuring the enzyme activity of malic enzyme (ME) during Yarrowia lipolytica fermentation with different nitrogen sources, Bellou et al. found that ME may not be implicated in lipid biosynthesis in this yeast, and NADPH may be provided by the pentose phosphate pathway (PPP). The presence of organic nitrogen in low concentrations during lipogenesis was also required for NADPH supply of the lipogenic machinery in Y. lipolytica.
Effect of glucose feeding on cell growth and carbon distribution
Excess carbon source is a prerequisite for SCO accumulation, and high glucose concentrations also induce the expression of GO. Accordingly, different glucose concentrations ranging from 9 to 15% were adopted to investigate the effect of glucose dosage on SCO accumulation and GA production. As seen in Fig. 2, 21.7 g/L of GA was produced when adding 15% glucose, with a yield of 0.16 g/g from glucose, corresponding to an increase of 24% compared with 9% glucose addition. However, an increased GA production due to higher glucose concentration might also cause more hydrogen peroxide accumulation in the medium, resulting in a severe damage on cell growth . As observed in our experiment, the biomass did decrease by 35.5% when the glucose concentration was increased from 9 to 15%. In addition, cells generally tend to grow better at lower initial glucose concentration, since a high carbon source concentration might result in higher oxygen requirements during microbial cell growth, leading to a subsequent lower dissolved oxygen concentration (DOC) in the medium, which would force cells to enter the stationary growth phase prematurely .
With regard to the production of lipids, a content of 51.3% was obtained when the glucose concentration was increased from 9 to 15%, leading to a 41.3% improvement (Fig. 2). However, an increase in lipid content does not necessarily mean an increased lipid production in total. Since SCO is accumulated intracellularly, lower biomass concentration does discount SCO yield. As observed in this study, only 13.4 g/L of SCO was produced when 15% glucose was added, i.e., a 9% decrease compared to SCO production with 9% glucose. In conclusion, a high glucose concentration is more favorable for lipid accumulation rather than SCO production.
As expected, fatty acid composition was not affected markedly by varying the glucose concentration. The major fatty acids of C. podzolicus DSM 27192 were still palmitic acid (C16:0, ~ 20%) and oleic acid (C18:1, ~ 62%) (Table 1). Exceptionally, linoleic acid (C18:2) content did increase by 14.3%, from 7.7 to 8.8% in total lipids. A similar phenomenon was also reported for Y. lipolytica. When Y. lipolytica was cultivated with high initial glucose concentration, the concentration of cellular oleic acid decreased, while linoleic acid slightly increased . This could be caused by an increased desaturation of oleic acid by Δ12desaturase within the fatty acid elongation cycle . Therefore, optimizing the initial glucose concentration might be an easy way to upgrade SCO value by enhancing the content of polyunsaturated fatty acids in C. podzolicus DSM 27192 and other oleaginous yeasts.
Effect of DOC on cell growth and SCO–GA co-production
Dissolved oxygen concentration reflects the real-time state of cell growth and glucose uptake under a given agitation and aeration rate. In the early phase of C. podzolicus DSM 27192 cultivation, the DOC decreased rapidly to zero and remained zero throughout the exponential phase, suggesting that oxygen supply was a limiting factor for cell growth and lipid production, which was also observed when using other yeasts [35, 38]. Likewise, oxygen pressure was also proven to play a key role in GA production . Therefore, further research regarding DOC influence on the production of SCO and GA was conducted.
The growth curve of C. podzolicus DSM 27192 cultivated with DOC above 40% as well as the production of SCO and GA is illustrated in Fig. 3. After 40 h of cultivation, the agitation speed was increased gradually from 600 rpm up to 930 rpm to keep DOC above 40%. The increased agitation resulted in a slight damage to cell growth, as 12% decrease in cell mass was found when compared with that under a constant agitation of 600 rpm. However, the negative influence of the increased agitation on GA production was more pronounced than on cell growth. GA production was maintained at a sluggish rate under high agitation condition, even after more glucose was supplemented. Only 9.6 g/L of GA was obtained after 145 h, with a GA yield of only 0.06 g/g glucose (Table 2), showing a 45% decrease compared with that under a constant agitation of 600 rpm. The reason could be that the activity of GO dropped sharply due to the increase in agitation speed as reported by Petruccioli et al. .
In contrast, the increased DOC had a positive effect on SCO accumulation, as a noticeable increase from 36.3 to 47.8% in lipid content was observed, corresponding to an increased lipid yield of 0.11 g/g glucose. This may be attributed to the upregulation of ATP-citrate lyase and malic enzyme at high DOC, which participate in lipid synthesis while the activity of NAD+-dependent isocitrate dehydrogenase was also found to decrease during the transition from low to high DOC in that study, usually a prerequisite for lipid accumulation . Besides from Y. lipolytica and Rhodotorula glutinis, high DOC was beneficial for cell growth, but unfavorable for lipid accumulation in other studies [41, 42].
The changes of overall fatty acid composition under different DOC conditions were negligible (Table 1). For example, under constant agitation, the main fatty acids are palmitic acid (C16:0) 20.0%, stearic acid (C18:0) 5.5%, oleic acid (C18:1) 62.9%, and linoleic acid (C18:2) 7.7%. A nearly identical composition was obtained, when DOC was kept above 40% (21.1%, 5.5%, 61.5%, and 8.1% of C16:0, C18:0, C18:1 and C18:2, respectively). In contrast to Lipomyces starkeyi , an increased DOC did not decrease the saturation degree of fatty acids. Speculatively, the amount of oxygen required for the unsaturation is negligible when compared to cell propagation, energy metabolism, and total lipid biosynthesis in this yeast under current conditions.
SCO and GA accumulation under high DOC and high glucose feeding at different fermentation stages
Taken together, high DOC is favorable for SCO production, while high glucose concentration is favorable for GA production (Table 2). To explore the comprehensive effect of high DOC and high glucose addition on both cell growth and metabolites mainly SCO and GA production, experiments with high glucose feeding rate and high DOC above 40% were conducted. As expected, the growth of C. podzolicus DSM 27192 was severely inhibited by the increased glucose concentration and high agitation (Fig. 4). Only 21.8 g/L of cell mass was obtained after 142 h, resulting in the lowest lipid production of 11.7 g/L (Table 2). In addition, the neutralization caused by the high DOC and high glucose addition resulted in only 15.4 g/L of GA production.
It was found that cells grew fast during the growth phase, accumulating little SCO, with nearly no GA production. When the fermentation process entered the oleaginous phase after nitrogen depletion, glucose was channeled mainly to SCO accumulation, as relatively small amounts of GA were formed. At the end of the oleaginous phase, the cellular stored lipids were gradually degraded and presumably used for GA production, although glucose was still available in the medium (Fig. 4). By this strategy, it was possible to separate the production phases of both metabolites. Similar phenomena were also observed by using other oleaginous microorganisms. For example, when Aspergillus niger was cultivated on waste glycerol medium derived from the biodiesel industry, stored lipids were used to produce significant amounts of oxalic acid even under high glycerol concentration . Also, stored lipids in Y. lipolytica were degraded and citric acid was produced despite high amounts of glycerol . Generally, degradation of lipids for the production of other compounds occurs when carbon sources are completely exhausted [45, 46], or when the carbon source uptake rate cannot satisfy the anabolic activities inside the cell . Especially during lipid accumulation, the uptake and metabolism of glucose are very slow when nitrogen is depleted . Thereby, nitrogen limitation would induce lipid accumulation in the first growth stage, while the GA biosynthesis pathway was not completely activated. Afterward, stored lipids were degraded to synthesize GA due to the restriction in glucose transportation and metabolism. However, further analysis of the metabolic balance between SCO and GA using transcriptomics or proteomics is needed for future studies.
Different factors influencing the carbon flow between SCO and GA production, namely nitrogen source, dissolved oxygen, glucose concentration and cultivation time, have been studied using C. podzolicus DSM 27192. The carbon distribution between SCO and GA was found susceptible to cultivation conditions. In detail, the GA production pathway was severely inhibited by organic nitrogen sources; high glucose addition greatly stimulated GA production, and both high glucose addition and high DOC were proven to promote SCO accumulation. However, either high glucose addition or high DOC had negative effects on cell mass growth, especially high glucose addition, which discounted the total SCO production. Hence, a two-stage DOC or glucose concentration control strategy was needed to improve cell growth and distribute carbon between SCO and GA. Moreover, the fermentation time is important for lipid production, since stored lipids will be degraded and used for the production of non-lipid metabolites in the late stationary phase. All these observations give the opportunity to favor either the production of SCO or GA or rather their simultaneous production. More importantly, this study might give more guidance for other co-production systems. Further studies should be focused on developing more efficient SCO co-production systems, improving the total product yield, amending the SCO production pathway, and enhancing specific high-value fatty acid production.
Microorganisms and medium
Cryptococcus podzolicus DSM 27192 used in this study was deposited at DSMZ culture collection in Braunschweig, Germany. The glycerol stocks were stored at − 80 °C in the in-house culture collection. Yeast colonies were maintained at 4 °C on Yeast Malt (YM) Agar plates (g/L): yeast extract 3.0, malt extract 3.0, peptone 5.0, glucose 10.0, agar 20.0, pH 6.2. For SCO production, a mineral salt medium was used as described by Ines Schulze et al. . 50 g/L of glucose was used initially, from the 2nd day the glucose was replenished to a maximum concentration of 90 g/L after determining the actual concentration.
The nitrogen content was around 8–12% in yeast extract, 10–13% in peptone, and < 1% in malt extract used in this study. In the experiment of nitrogen influence study, to keep the C/N condition similar to the mineral salt medium, 12.1 g/L of YM nitrogen (3.3 g/L of yeast extract, 5.5 g/L of peptone, and 3.3 g/L of malt extract) and 10 g/L of yeast extract were used, respectively, to replace (NH4)2SO4 as the nitrogen source.
Batch fermentation in bioreactor
A loopful of cells from YM agar plates was used to inoculate 20 mL of mineral salt medium (50 g/L of glucose as the carbon source) in a baffled shake flask and incubated in a gyratory shaker at 20 °C and 130 rpm for approximately 24 h. A second pre-culture was carried out using the same conditions. The second pre-culture was prepared from the first pre-culture in 200 mL culture medium in 2 L shake flasks with an initial OD600 of 1.0.
Fermentation was performed in a 2.5 L fermenter (Infors HT, Bottmingen, Switzerland; Minifors fermenter) with working volume of 1.2 L, an initial OD600 of 0.5–1.0 at 600 rpm, and 1 vvm aeration rate without control of dissolved oxygen level (pO2). The pO2 value was measured constantly by a probe. The control of pH to 6.0 was done automatically by the addition of 4 M H3PO4 and 4 M NaOH. In each fermenter, Contraspum A 4050 HAC (Zschimmerund Schwarz GmbH und Co KG, Lahnstein, Germany) was applied as antifoam agent. Each day, 20 mL of salt solution and 20 mL of trace element solution were fed into the medium.
All experiments were done in independent duplicates under the same condition.
Determination of cell mass
The cell concentration in the culture medium was determined by the optical density at 600 nm (OD600) with the initial culture medium as blank. All samples were diluted to an optical density of 0.2–0.8 at 600 nm for measurement.
Cell dry biomass (CDW) was analyzed gravimetrically. 1 mL aliquot of the culture broth was transferred into a pre-dried and pre-weighed 1.5 mL reaction tube and centrifuged at 13,000 rpm for 5 min. The supernatant was collected and used for the determination of glucose, GA, and acetic acid. The cell pellet was washed with 1 mL saline (0.9% NaCl), dried at 60 °C for 24 h and weighed. For each sample, all parameters were measured in duplicate.
Determination of glucose and GA
For glucose determination, 45 µL 4 M NH3Cl and 100 µL 1.2 M MgSO4 were added to 1 mL pure supernatant and subsequently centrifuged for 5 min at 20,000×g after 5 min of incubation. 500 µL supernatant was then transferred to 500 µL 0.1 M H2SO4, mixed, and incubated for 15 min. After the final centrifugation step of 15 min at 20,000×g, the supernatant was used for HPLC analysis. The analysis was performed with a standard HPLC device (Agilent 1100 Series, Agilent, Germany) with a Rezex ROA organic acid H+ (8%) column (300 by 7.8 mm, 8 m; Phenomenex) protected by a Rezex ROA organic acid H+ (8%) guard column (50 by 7.8 mm). Separation was performed under isocratic conditions at 50 °C (column temperature) for 45 min with 5 mM H2SO4 as the mobile phase at a constant flow rate of 0.4 mL/min. Detection of carbohydrate was achieved via an Agilent 1200 series refractive index detector at 50 °C.
For GA analysis, the untreated supernatant was collected and diluted to an appropriate concentration using 20 mM KH2PO4 (pH 2.5). The analysis was performed with a standard HPLC device (Agilent1100 Series, Agilent Technologies Deutschland GmbH, Böblingen, Germany) equipped with a 150 × 4.6 mm HPLC column Synergi™ 4 μm Fusion-RP 80 Å (Phenomenex, Aschaffenburg, Germany; 00 F-4424-E0) at 30 °C column temperature. 20 mM KH2PO4 (pH 2.5) (A) and 100% methanol (B) were used as eluents to drive the following temporal gradient: 0–0.5 min 100% eluent A, 0.5–10 min increase of eluent B from 0 to 10%,10–12 min decrease of eluent B from 10% back to 0% and 12–14 min again 100% eluent A. 10 μL sample was injected, a flow rate of 1 mL/min was adjusted, and peaks were detected via UV at 220 nm.
Lipid extraction and determination of fatty acid methyl esters
20 mL aliquot of the culture broth was centrifuged (4700 rpm, 5 min), the pellet was resuspended in saline (0.9% NaCl). and centrifuged (4700 rpm, 5 min) again. The supernatant was discarded and the pellet was freeze dried (− 30 °C, 0.370 mbar). Sample preparation for the quantitative and qualitative gas chromatographic analysis was done in a one-step-procedure of direct esterification coupled with extraction. A portion (20 mg) of freeze-dried biomass was weighed into a 15 mL glass Falcon with Teflon cap. 1.5 mL of hexane and 0.5 mL of 2.0 mg/mL internal standard (methyl benzoate dissolved in hexane) were added as solvent for lipid extraction. In addition, 2 mL 15% H2SO4 in methanol was added for esterification. Then, the sample was heated up to 100 °C for 2 h with continuous shaking. After cooling on ice, 1 mL demineralized water was added, and the mixture was centrifuged for 5 min with 2500 rpm at 4 °C. Afterward, 1 μL of the upper phase was analyzed via chromatography (Agilent Technologies, 6890 N Network GC-System). The instrument was equipped with a DBWax column (Length: 30 m, diam: 0.25 mm, film: 0.25 μm; Agilent Technologies Deutschland GmbH, Böblingen, Germany; 122-7032) and a flame ionization detector and worked with a pressure of 1.083 bar and initial temperature of 40 °C. The column temperature was increased from 40 to 250 °C at a rate of 8 °C/min. The temperature was held at 250 °C for 10 min before cooling down to 40 °C. The total fatty acid content and the identification of fatty acids were obtained using the standard RM3 FAME Mix (Sigma Aldrich, Taufkirchen, Germany; 07256-1AMP) and Marine FAME Mix (Acid Methyl Ester Marine Oil FAME Mix) (Restek GmbH, Bad Homburg, Germany; 35066). Fatty acids which represented less than 1% of total fatty acids were combined to “trace fatty acids”.
Availability of data and materials
The information about accession numbers is given in the manuscript.
single cell oil
dissolved oxygen concentration
Huang C, Chen XF, Xiong L, Chen XD, Ma LL, Chen Y. Single cell oil production from low-cost substrates: the possibility and potential of its industrialization. Biotechnol Adv. 2013;31:129–39.
Qin L, Liu L, Zeng AP, Wei D. From low-cost substrates to single cell oils synthesized by oleaginous yeasts. Bioresour Technol. 2017;245:1507–19.
Carsanba E, Papanikolaou S, Erten H. Production of oils and fats by oleaginous microorganisms with an emphasis given to the potential of the nonconventional yeast Yarrowia lipolytica. Crit Rev Biotechnol. 2018;38:1230–43.
Ochsenreither K, Glück C, Stressler T, Fischer L, Syldatk C. Production strategies and applications of microbial single cell oils. Front Microbiol. 2016;7:1539.
Muniraj IK, Uthandi SK, Hu ZH, Xiao LW, Zhan XM. Microbial lipid production from renewable and waste materials for second-generation biodiesel feedstock. Environ Technol Rev. 2015;4:1–16.
Qiao KJ, Abidi SHI, Liu HJ, Zhang HR, Chakraborty S, Watson N, et al. Engineering lipid overproduction in the oleaginous yeast Yarrowia lipolytica. Metab Eng. 2015;29:56–65.
Poontawee R, Yongmanitchai W, Limtong S. Efficient oleaginous yeasts for lipid production from lignocellulosic sugars and effects of lignocellulose degradation compounds on growth and lipid production. Process Biochem. 2017;53:44–60.
Calvey CH, Su Y-K, Willis LB, McGee M, Jeffries TW. Nitrogen limitation, oxygen limitation, and lipid accumulation in Lipomyces starkeyi. Bioresour Technol. 2016;200:780–8.
Friedlander J, Tsakraklides V, Kamineni A, Greenhagen EH, Consiglio AL, MacEwen K, et al. Engineering of a high lipid producing Yarrowia lipolytica strain. Biotechnol Biofuels. 2016;9:77.
Fei Q, Wewetzer SJ, Kurosawa K, Rha C, Sinskey AJ. High-cell-density cultivation of an engineered Rhodococcus opacus strain for lipid production via co-fermentation of glucose and xylose. Process Biochem. 2015;50:500–6.
Jin MJ, Slininger PJ, Dien BS, Waghmode S, Moser BR, Orjuela A, et al. Microbial lipid-based lignocellulosic biorefinery: feasibility and challenges. Trends Biotechnol. 2015;33:43–54.
Liang QF, Qi QS. From a co-production design to an integrated single-cell biorefinery. Biotechnol Adv. 2014;32:1328–35.
Zhang CL, Shen HW, Zhang XB, Yu X, Wang H, Xiao S, et al. Combined mutagenesis of Rhodosporidium toruloides for improved production of carotenoids and lipids. Biotechnol Lett. 2016;38:1733–8.
Li T, Elhadi D, Chen GQ. Co-production of microbial polyhydroxyalkanoates with other chemicals. Metab Eng. 2017;43:29–36.
You SP, Zhang JY, Yin QD, Wei Q, Su RX, He ZM. Development of a novel integrated process for co-production of β-galactosidase and ethanol using lactose as substrate. Bioresour Technol. 2017;230:15–23.
Liu XY, Yu XJ, Lv JS, Xu JX, Xia J, Wu Z, et al. A cost-effective process for the coproduction of erythritol and lipase with Yarrowia lipolytica M53 from waste cooking oil. Food Bioprod Process. 2017;103:86–94.
Liu Y, Liao W, Chen S. Co-production of lactic acid and chitin using a pelletized filamentous fungus Rhizopus oryzae cultured on cull potatoes and glucose. J Appl Microbiol. 2010;105:1521–8.
Kim I, Seo YH, Kim GY, Han JI. Co-production of bioethanol and biodiesel from corn stover pretreated with nitric acid. Fuel. 2015;143:285–9.
Halim R, Webley PA, Martin GJO. The CIDES process: fractionation of concentrated microalgal paste for co-production of biofuel, nutraceuticals, and high-grade protein feed. Algal Res. 2016;19:299–306.
Saenge C, Cheirsilp B, Suksaroge TT, Bourtoom T. Potential use of oleaginous red yeast Rhodotorula glutinis for the bioconversion of crude glycerol from biodiesel plant to lipids and carotenoids. Process Biochem. 2011;46:210–8.
Gao BY, Chen AL, Zhang WY, Li AF, Zhang CW. Co-production of lipids, eicosapentaenoic acid, fucoxanthin, and chrysolaminarin by Phaeodactylum tricornutum cultured in a flat-plate photobioreactor under varying nitrogen conditions. J Ocean Univ China. 2017;16:916–24.
Bai MD, Cheng CH, Wan HM, Lin YH. Microalgal pigments potential as byproducts in lipid production. J Taiwan Inst Chem Eng. 2011;42:783–6.
Schulze I, Hansen S, Großhans S, Rudszuck T, Ochsenreither K, Syldatk C, et al. Characterization of newly isolated oleaginous yeasts—Cryptococcus podzolicus, Trichosporon porosum and Pichia segobiensis. AMB Express. 2014;4:24.
Ramachandran S, Fontanille P, Pandey A, Larroche C. Gluconic acid: properties, applications and microbial production. Food Technol Biotechnol. 2006;44:185–95.
Qi PY, Chen SS, Chen J, Zheng JW, Zheng XL, Yuan YZ. Catalysis and reactivation of ordered mesoporous carbon-supported gold nanoparticles for the base-free oxidation of glucose to gluconic acid. ACS Catal. 2015;5:2659–70.
Cañete-Rodríguez AM, Santos-Dueñas IM, Jiménez-Hornero JE, Ehrenreich A, Liebl W, García-García I. Gluconic acid: properties, production methods and applications—an excellent opportunity for agro-industrial by-products and waste bio-valorization. Process Biochem. 2016;51:1891–903.
Pal P, Kumar R, Banerjee S. Manufacture of gluconic acid: a review towards process intensification for green production. Chem Eng Process. 2016;104:160–71.
da Cruz SH, Batistote M, Ernandes JR. Effect of sugar catabolite repression in correlation with the complexity of the nitrogen source on yeast growth and fermentation. J Struct Inst Brew. 2015;109:349–55.
Li Y, Chen J, Liang D-F, Lun S-Y. Effect of nitrogen source and nitrogen concentration on the production of pyruvate by Torulopsis glabrata. J Biotechnol. 2000;81:27–34.
Bellou S, Triantaphyllidou I-E, Mizerakis P, Aggelis G. High lipid accumulation in Yarrowia lipolytica cultivated under double limitation of nitrogen and magnesium. J Biotechnol. 2016;234:116–26.
Dubey MK, Zehra A, Aamir M, Meena M, Ahirwal L, Singh S, et al. Improvement strategies, cost effective production, and potential applications of fungal glucose oxidase (GOD): current updates. Front Microbiol. 2017;8:1032.
Wong CM, Wong KH, Chen XD. Glucose oxidase: natural occurrence, function, properties and industrial applications. Appl Microbiol Biotechnol. 2008;78:927–38.
Gunny AAN, Arbain D, Ahmad MS, Tompang MF. Screening of medium components for glucose oxidase production by Aspergillus terreus UniMAP AA-1. In: International conference on food engineering and biotechnology, IPCBEE, IACSIT press, Singapore. vol. 9. 2011. p. 73–6.
Bankar SB, Bule MV, Singhal RS, Ananthanarayan L. Optimization of Aspergillus niger fermentation for the production of glucose oxidase. Food Bioprocess Technol. 2009;2:344–52.
Bellou S, Makri A, Triantaphyllidou I-E, Papanikolaou S, Aggelis G. Morphological and metabolic shifts of Yarrowia lipolytica induced by alteration of the dissolved oxygen concentration in the growth environment. Microbiology. 2014;160:807–17.
Papanikolaou S, Chatzifragkou A, Fakas S, Galiotou-Panayotou M, Komaitis M, Nicaud JM, et al. Biosynthesis of lipids and organic acids by Yarrowia lipolytica strains cultivated on glucose. Eur J Lipid Sci Technol. 2009;111:1221–32.
Lee J-E, Vadlani PV, Min D. Sustainable production of microbial lipids from lignocellulosic biomass using oleaginous yeast cultures. J Sustain Bioenergy Syst. 2017;7:36–50.
Galafassi S, Cucchetti D, Pizza F, Franzosi G, Bianchi D, Compagno C. Lipid production for second generation biodiesel by the oleaginous yeast Rhodotorula graminis. Bioresour Technol. 2012;111:398–403.
Tan XS, Deng WP, Liu M, Zhang QH, Wang Y. Carbon nanotube-supported gold nanoparticles as efficient catalysts for selective oxidation of cellobiose into gluconic acid in aqueous medium. Chem Commun. 2009;41:7179–81.
Petruccioli M, Fenice M, Piccioni P, Federici F. Effect of stirrer speed and buffering agents on the production of glucose oxidase and catalase by Penicillium variabile (P16) in benchtop bioreactor. Enzyme Microb Technol. 1995;17:336–9.
Papanikolaou S, Chevalot I, Komaitis M, Marc I, Aggelis G. Single cell oil production by Yarrowia lipolytica growing on an industrial derivative of animal fat in batch cultures. Appl Microbiol Biotechnol. 2002;58:308–12.
Yen HW, Zhang ZY. Effects of dissolved oxygen level on cell growth and total lipid accumulation in the cultivation of Rhodotorula glutinis. J Biosci Bioeng. 2011;112:71–4.
André A, Diamantopoulou P, Philippoussis A, Sarris D, Komaitis M, Papanikolaou S. Biotechnological conversions of bio-diesel derived waste glycerol into added-value compounds by higher fungi: production of biomass, single cell oil and oxalic acid. Ind Crops Prod. 2010;31:407–16.
Makri A, Fakas S, Aggelis G. Metabolic activities of biotechnological interest in Yarrowia lipolytica grown on glycerol in repeated batch cultures. Bioresour Technol. 2010;101:2351–8.
Papanikolaou S, Aggelis G. Lipids of oleaginous yeasts. Part I: biochemistry of single cell oil production. Eur J Lipid Sci Technol. 2011;113:1031–51.
Dourou M, Aggeli D, Papanikolaou S, Aggelis G. Critical steps in carbon metabolism affecting lipid accumulation and their regulation in oleaginous microorganisms. Appl Microbiol Biotechnol. 2018;102:2509–23.
Palma M, Madeira SC, Mendes-Ferreira A, Sá-Correia I. Impact of assimilable nitrogen availability in glucose uptake kinetics in Saccharomyces cerevisiae during alcoholic fermentation. Microb Cell Fact. 2012;11:99.
This work was supported by the National Natural Science Foundation of China (No. 21706125, No. 21706124) and the Jiangsu Province Natural Science Foundation for Youths (BK20170993).
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Qian, X., Gorte, O., Chen, L. et al. Co-production of single cell oil and gluconic acid using oleaginous Cryptococcus podzolicus DSM 27192. Biotechnol Biofuels 12, 127 (2019) doi:10.1186/s13068-019-1469-9
- Single cell oil (SCO)
- Gluconic acid (GA)
- Carbon flow