http://orcid.org/0000-0002-3732-4776
Figures
Abstract
The heterotrophic microalgae Crypthecodinium cohnii was usually cultivated in complex medium containing glucose, yeast extract and sea salt. For the preparation of DHA with highest purity, a new defined medium without the yeast extract was developed. Different inoculated densities, C/N ratios, temperatures, culture volumes and glucose additions were investigated to optimize the algal growth rate and DHA production. The growth period in C. cohnii was shortened from 12–14 days to 7–8 days, the OD600 was enhanced from 2.0 to 3.0, the glucose consumption was accelerated and used up on day 3–4, and the DHA content in culture were increased from 10 to 45 nmoles/300 μl batch. It was found that C. cohnii had optimal growth and DHA accumulation in 25 °C, 0.2 inoculated density, 5–10 C/N ratio, 5:1 air/culture volume ratio. This is the first time DHA production using C.cohnii has been optimized in synthetic medium. This allows preparation of uniformly radiolabeled 13C- and 14C-DHA.
Citation: Song P, Kuryatov A, Axelsen PH (2020) A new synthetic medium for the optimization of docosahexaenoic acid production in Crypthecodinium cohnii. PLoS ONE 15(3): e0229556. https://doi.org/10.1371/journal.pone.0229556
Editor: Prakash Kumar Sarangi, Central Agricultural University, INDIA
Received: December 16, 2019; Accepted: February 6, 2020; Published: March 20, 2020
This is an open access article, free of all copyright, and may be freely reproduced, distributed, transmitted, modified, built upon, or otherwise used by anyone for any lawful purpose. The work is made available under the Creative Commons CC0 public domain dedication.
Data Availability: All relevant data are within the paper.
Funding: This work was supported by National Institutes of Health AG057197 from Dr Paul H. Axelsen; Guizhou Science and Technology Foundation of China (No. TS [2017]-2843, TJ [2017] 1143, GY [2017] 5-6) from Dr Pingping Song.
Competing interests: The authors have declared that no competing interests exist.
1. Introduction
In recent years, Docosahexaenoic acid (DHA) belonging to the ω-3 polyunsaturated fatty acid (PUFA) has become the focus of considerable attention due to its neuroprotective effects [1,2]. DHA, enhanced in phospholipids in the central nervous system and retina, is recognized to multiple roles in brain health and diseases, such as Alzheimer’s disease [3–5].
The traditional source of ω-3 fatty acids is fish oil, which contains two major PUFAs, DHA and eicosapentaenoic acid (EPA) [6]. However, the fish oil as a food additive has significant problems: its strong fishy smell, unpleasant taste and poor oxidative stability [7]. Marine micro-organisms that contain large amounts of DHA might provide this important fatty acid [8,9]. Microalgae biomass is exceptionally suitable for the extraction and isolation of individual PUFAs due to its stable and reliable contents [10]. Hence, screening of microalgae for DHA production is significant.
Crypthecodinium cohnii (C. cohnii) has been recognized as a high-volume producer of DHA amongst the marine dinoflagellate microalgae, especially in pharmaceutical and nutraceutical applications. This microalgae is exceptional in that it can accumulate a high fraction of DHA with trivial amounts of other PUFAs in cell lipids, which makes the DHA isolation very interesting, particularly for higher incorporation of glucose into DHA [11,12]. DHA-producing C. cohnii is cultivated in media containing the glucose as a sole carbon source, so the media compositions are very important to the DHA accumulation in C. cohnii.
DHA production from C. cohnii has been extensively studied and optimized [7]. High-level manufacturing of algal fatty acids is feasible by using traditional fermentation systems. Only a limited number of studies of purity of the DHA extracted from C. cohnii have been reported. In animal experiments, carbon isotope radiolabeled polyunsaturated fatty acids with high purity are usually used to explore the pathogenesis of some diseases [13]. However, the media used to grow C. cohnii are not very useful for preparing DHA samples with high isotopic purity. Here we reported a better synthetic defined medium for growing C. cohnii. The effects of various medium components and culture conditions on algal growth and DHA production were studied.
2. Materials and methods
2.1 Materials
DHA was purchased from Nu-Check Prep Inc. (Elysian, MN). d5-DHA was purchased from Cayman Chemicals (Ann Arbor, Michigan). C. cohnii (ATCC 40750) was obtained from American Type Culture Collection (Manassas, VA, USA). All other chemicals were obtained from Sigma-Aldrich (St. Louis, MO, USA).
2.2 Medium and culture conditions
C. cohnii stocks were cultivated in 4 g/L yeast extract, 12 g/L glucose, 35 g/L sea salt medium at 26°C in the dark. New cultures were inoculated to an OD600 of about 0.15. After 4–5 days OD600 reached ~1.5, and 1.5–2 ml of this culture were centrifuged at 500 g for 1 min. The supernatants were discarded and the left pellets were washed in ~5 ml of defined media (without glucose and glutamate) and centrifuged at 500 g for 1 min. After this, pellets were re-suspended in 10 ml of synthetic medium at different glutamate concentrations (1.8 g/L, 0.9 g/L, 0.6 g/L, 0.45 g/L, 0 g/L), temperatures (15°C, 20°C, 25°C, 30°C), culture volumes (5 ml, 10 ml, 15 ml, 20 ml) and additional glucoses concentrations (9 g/L, 4.5 g/L, 1.5 g/L, 0.5 g/L). The final OD600 were adjusted to 0.15–0.2, and cultures were incubated in a refrigerated incubator shaker (Edison, NJ, USA) in the dark at 200 rpm. The growth and DHA content of C. cohnii were analyzed daily.
A defined medium developed by Tuttle and Loeblich [14], were shown in following Tables 1, 2 and 3. All stock solutions were sterilized by the filtration through 0.22 μm Milex syringe filters. Variations on this defined medium were investigated in the experiments which follow.
2.3 The growth rate and glucose determination
The growth rate was determined by measuring the OD600 using a Cary 400 Bio UV-Vis spectrophotometer (Agilent, Santa Clara, CA). Glucose consumption was measured by the DNS method [15,16]. After the centrifugation of algal culture, the supernatant (25 μl) were taken and added to 275 μl water, then 300 μl DNS (1 g/L 3,5-dinitrosalicylic acid, 0.1 g/L Na2SO3, 1 g/L NaOH) were added, and incubated for 10 min at 90°C. After the incubation, 600 μl quencher (40 g/L sodium potassium tartrate) were added, and the final solution was cooled down to room temperature. Glucose concentration was measured by OD540 and analyzed by the glucose standard curve.
2.4 Lipid extraction and saponification
300 μl of algal culture in a 1.5 ml Eppendorf tube were centrifuged for 1 min at 2000 g. The supernatant was removed, and the pellet was re-suspended in 640 μl water. The suspension was subjected to three free-thaw cycles (liquid nitrogen alternating with boiling water), and cooled down on ice. 1.6 ml methanol and 800 μl dichloromethane were added and mixed, then sonicated 90 s on ice. 800 μl dichloromethane and 640 μl water were added to separate phases, which were centrifuged at 400 g for 1 min. The lower phase was withdrawn and transferred to new 13x100 mm glass tubes, and dried under argon.
Pellets were dissolved in 1.5 ml of 85% methanol in water, then 0.5ml of 1 M NaOH was added. Saponification was performed at 80°C for 1 h. Then the tubes were cooled to room temperature. The samples were acidified with 400 μl HCl (5 M). Then 1 ml of isooctane were added, vortexed and allowed to settle before the upper phase was pipetted into a glass tube. The combined upper phases were evaporated under argon. 100 μl of ethanol were added, transferred to the new vials with cap, blown with argon and then the vials were stored in a -80°C freezer.
2.5 HPLC separation and mass spectrometry analysis
An aliquot of calibrated amount of d5-DHA were added to the extracts of DHA to calculate the content. 5 μl samples were injected into a 1.0x50 mm Eclipse XD8-C18 3.5 μm column. Solvent A was 60% acetonitrile, 40% water and 0.1% formic acid. Solvent B was 100% acetonitrile and 0.1% formic acid. The mobile phase was pumped at 0.1 ml/min. From 0 to 5 min the solvent was 0% buffer B, then the composition was changed linearly from 0–100% solvent B at 5–6.5 min, 100% solvent B at 6.5–10 min, returned to 0% at 10–10.5 min, and then kept at 0% buffer B from 10.5 to 12.5 min. The eluent was alkalinized post-column with 0.15 M ammonium hydroxide in methanol flowing at 50 μl/min, and introduced into an ABI 4000 Q1 Trap tandem mass spectrometer (Sciex, Toronto, Canada) via electrospray ionization at negative polarity. The declustering potential (DP) was -70 V, the ionspray voltage (Is) was -4000 V, the temperature of drying gas (TEM) was 200°C, the collision energy (CE) was -20 V and the collision gas (CAD) was 4psi for multiple reaction monitoring (MRM) mode. The m/z transitions in MRM mode were from 327.2–283.2 for 12C-DHA with the neutral loss of CO2, 332.2–288.2 for d5-DHA.
3. Results
3.1 Growth and DHA production of C. cohnii under different conditions
3.1.1 Different inoculated densities.
When the inoculated density was 0.4, the algal cells had the highest growth rate, the maximum OD600 was 2.5, but the highest DHA content (0.1 μmole/batch) in culture was got on day 4 when the inoculated density was 0.2 (Fig 1A and 1B).
A. OD600; B, DHA content in culture, 1ml/batch.
3.1.2 Different glutamate concentrations.
In the N-deprived group, algal cells didn’t grow, the glucose was consumed very slowly, and DHA content in culture was lowest during the 7-day culture period. From the 0.45 g/L to 1.8 g/L of glutamate concentration, growth rate, glucose consumption and DHA production of C. cohnii gradually increased. At 1.8g/L glutamate concentration, the growth rate was the highest, and reached a maximum OD600 on day 5, then kept at the stable level on days 6–7 (Fig 2A). From 0.9 g/L to 1.8 g/L of glutamate concentration, the glucose consumption in culture was rapid over days 1–4, then stopped in 2 g/L on days 5–7 (Fig 2B). DHA production was the highest on day 4, then declined sharply (Fig 2C).
A, OD600; B, glucose consumption; C, DHA content in culture, 300 μl/batch.
3.1.3 Temperatures.
At 15°C, algal cells grew slowly, glucose was not consumed efficiently, and DHA production was very low during the incubation (Fig 3A–3C). At 20°C, algal cells grew faster, and reached a maximum OD600 on day 6 (Fig 3A), but the glucose consumption stopped on day 7 (Fig 3B). DHA production was highest on day 6 (Fig 3C). At 25°C, the growth rate of C. cohnii was the highest (Fig 3A). Glucose consumption was most rapid over days 1–3, then stopped at 2 g/L on days 4–7 (Fig 3B). DHA production kept at a higher level (Fig 3C). At 30°C, algal cells grew fast at first, then declined sharply after day 5 (Fig 3A). Glucose consumption stopped at 2 g/L after day 5, and DHA production was low (Fig 3B and 3C).
A, OD600; B, glucose consumption; C, DHA content in culture, 300 μl/batch.
3.1.4 Air/Culture volume ratios.
Growth rate of algal cells was highest in 9:1 and 4:1 air/culture volume ratios. Glucose consumption stopped on days 3–7. DHA production reached the highest level on day 4. In 1.5:1 air/culture volume ratio, both growth rate and DHA yield were the lowest, and glucose consumption stopped on days 5–7 (Fig 4A–4C).
5 ml (9:1), 10 ml (4:1), 15 ml (2:1), and 20 ml (1.5:1) of medium in 50 ml tubes. A, OD600; B, glucose consumption; C, DHA content in culture, 300 μl/batch.
3.1.5 Adding supplementary glucose.
DHA content of C. cohnii in culture was 0.02 μmoles/batch on day 4. After adding 9 g/L glucose, DHA accumulation reached 0.045 μmoles/batch on day 7. After adding 4.5 g/L glucose, C. cohnii had a maximum OD600 on day 5, DHA content in culture was 0.035 μmoles/batch, which was similar with 1.5 g/L glucose on day 7. After adding 0.5 g/L glucose, OD600 and DHA accumulation were both lower than other groups (Fig 5A–5C).
A, OD600; B, glucose consumption; C, DHA content in culture, 300 μl/batch.
4. Discussion
In these experiments, the growth rate and DHA production from C. cohnii in different conditions were analyzed.
Many kinds of complex media with different components have been investigated to culture the C. cohnii [17–19]. All of them used yeast extract. In our studies an optimal defined medium was found. In this medium, a metal mixture and various vitamins were added to enrich the culture. OD600 was used to analyze the algal growth. The growth period of algal cells was significantly shortened from 13–14 days to 7–8 days (data not shown). Algal cells generally entered the growth phase on day 2, reached the highest growth rate (OD600 = 2.5–3) on days 4–5, and reached the plateau phase on days 5–7.
Different inoculated densities from C. cohnii were investigated in these experiments. When the original inoculated density was about 0.2, algal cells achieved the optimal growth rate and highest DHA production (Fig 1B). Higher or lower inoculated densities were not beneficial for algal growth and DHA accumulation [20]. Considering uniformly 13C or 14C-labeled DHA experiments, the ideal inoculated density of C. cohnii was determined to 0.15–0.2.
C/N ratio plays a very important role for algal growth and DHA production [21,22]. Carbon and nitrogen are both necessary nutrient elements in the medium. When nitrogen was efficiently consumed in culture, glucose was transformed into more lipids. In our experiments, it was also found that the growth and DHA production of C. cohnii had differed depending on different glutamate concentrations (Fig 2A and 2C). Algal cells didn’t grow in N-deprived condition, glucose was consumed very slowly, and DHA content was the lowest during the culture period. Growth rate and DHA production of C. cohnii gradually increased when glutamate concentrations were raised from 0–1.8 g/L. At 0.9–1.8 g/L glutamate, glucose consumption was most rapid, so the algal cells achieved a higher OD600 and DHA yield. The optimal C/N ratio for algal growth in C. cohnii was determined to be 5–10.
Temperature is also an important factor for algal growth and DHA accumulation. At a low temperature (15°C), C. cohnii had a slow growth rate and low DHA production (Fig 3A and 3C). At a high temperature (30°C), algal growth and glucose consumption were restricted (Fig 3A and 3B). Even though the DHA production was relatively higher on day 7, the cultivation period was prolonged. 25°C was found to be the optimal temperature for growth and DHA production (Fig 3A and 3C). Algal cells grown at different temperatures may adapt by changing the proportion of polyunsaturated fatty acids in order to maintain proper membrane lipid fluidity and cell functions [23,24].
Volume ratio of air and culture was a key factor for algal growth [25]. Some reports have indicated excess culture in limited volume decreased the contact area with air and thus reduced the oxygen supply and ventilation efficiency [26]. C. cohnii was cultivated in 50 ml tube. For 5 ml and 10 ml cultures, the algal cells had higher growth rate, glucose consumption stopped on day 3, and the DHA production reached the highest level on day 4 (Fig 4A–4C). But in 20 ml cultures, the growth rate and DHA production of C. cohnii were the lowest (Fig 4A and 4C), and glucose consumption stopped two days later (Fig 4B). So, the optimal volume ratio between air and culture was 4–9.
After addition of glucose, C. cohnii had a higher growth rate, but DHA accumulation was not increased (Fig 5a and 5C). After adding extra 9 g/L glucose, DHA content in culture on day 7 was two-fold higher than on day 4, but was much lower than without glucose addition (Fig 5C). Hence, it was concluded that glucose addition can’t promote DHA accumulation in C. cohnii. Although glucose could be transformed into lipids during metabolism, excessive glucose could accelerate the algal growth and consumption of cellular lipids.
By these optimizations, optimal condition for the growth rate and DHA production in C. cohnii were established. These findings would provide optimal methods for the biosynthesis of uniformly radiolabeled 13C- and 14C-DHA, and for the research on the fate of oxidation products of DHA in Alzheimer’s disease.
Acknowledgments
The authors would like to thank Prof. Jon Lindstrom (University of Pennsylvania, Philadelphia) for proofreading and corrections of the manuscript, Dr Hiroaki Komatsu and Dr Ran Furman (University of Pennsylvania, Philadelphia) for their help with experimental technologies, and Dr Chris Moser (University of Pennsylvania, Philadelphia) for his assistance with the incubator shaker.
References
- 1. Calder PC. Docosahexaenoic acid. Annals of Nutrition and Metabolism, 2016, 69 (Suppl. 1): 8–21.
- 2. Siriwardhana N, Kalupahana NS, Moustaid-Moussa N. Health benefits of ω-3 polyunsaturated fatty acids: eicosapentaenoic acid and docosahexaenoic acid. Advances in food and nutrition research. Academic Press, 2012, 65: 211–222.
- 3. Sun GY, Simonyi A, Fritsche KL, et al. Docosahexaenoic acid (DHA): An essential nutrient and a nutraceutical for brain health and diseases. Prostaglandins, Leukotrienes and Essential Fatty Acids, 2018, 136: 3–13.
- 4. Weiser M, Butt C, Mohajeri M. Docosahexaenoic acid and cognition throughout the lifespan. Nutrients, 2016, 8 (2): 99. pmid:26901223
- 5. Harauma A, Yasuda H, Hatanaka E, et al. The essentiality of arachidonic acid in addition to docosahexaenoic acid for brain growth and function. Prostaglandins, Leukotrienes and Essential Fatty Acids, 2017, 116: 9–18.
- 6. Abdulrazaq M, Innes JK, Calder PC. Effect of ω-3 polyunsaturated fatty acids on arthritic pain: A systematic review. Nutrition, 2017, 39: 57–66. pmid:28606571
- 7. Mendes A, Reis A, Vasconcelos R, et al. Crypthecodinium cohnii with emphasis on DHA production: a review. Journal of Applied Phycology, 2009, 21 (2): 199–214.
- 8. Ummalyma SB, Sukumaran RK, Pandey A. Evaluation of Freshwater Microalgal Isolates for Growth and Oil Production in Seawater Medium. Waste and Biomass Valorization, 2018: 1–8.
- 9. Winwood RJ. Recent developments in the commercial production of DHA and EPA rich oils from microalgae. Ocl, 2013, 20 (6): D604.
- 10. Mubarak M, Shaija A, Suchithra TV. A review on the extraction of lipid from microalgae for biodiesel production. Algal Research, 2015, 7: 117–123.
- 11. Udayan A, Arumugam M, Pandey A. Nutraceuticals from algae and cyanobacteria. Algal Green Chemistry. Elsevier, 2017: 65–89.
- 12. Ziboh VA, Dreize MA, Hsia SL. Inhibition of lipid synthesis and glucose-6-phosphate dehydrogenase in rat skin by dehydroepiandrosterone. Journal of Lipid Research, 1970, 11 (4): 346–354. pmid:4394096
- 13. Furman R, Murray IVJ, Schall HE, et al. Amyloid plaque-associated oxidative degradation of uniformly radiolabeled arachidonic acid. ACS chemical neuroscience, 2016, 7 (3): 367–377. pmid:26800372
- 14. Tuttle RC, Loeblich III AR. An optimal growth medium for the dinoflagellate Crypthecodinium cohnii. Phycologia, 1975, 14 (1): 1–8.
- 15. Miller GL. Use of dinitrosalicylic acid reagent for determination of reducing sugar. Analytical Chemistry, 1959, 31 (3): 426–428.
- 16. Lee JV, Furman R, Axelsen PH. Biosynthesis of uniformly labeled 13C-and 14C-arachidonic acid in Mortierella alpina. Bioresource Technology, 2017, 227: 142–146. pmid:28013130
- 17. de Swaaf ME, de Rijk TC, Eggink G, et al. Optimisation of docosahexaenoic acid production in batch cultivations by Crypthecodinium cohnii. Progress in Industrial Microbiology. Elsevier, 1999, 35: 185–192.
- 18. Ratledge C, Kanagachandran K, Anderson AJ, et al. Production of docosahexaenoic acid by Crypthecodinium cohnii grown in a pH-auxostat culture with acetic acid as principal carbon source. Lipids, 2001, 36 (11): 1241–1246. pmid:11795857
- 19. De Swaaf ME, Sijtsma L, Pronk JT. High-cell-density fed-batch cultivation of the docosahexaenoic acid producing marine algae Crypthecodinium cohnii. Biotechnology and Bioengineering, 2003, 81 (6): 666–672. pmid:12529880
- 20. Huerlimann R, De Nys R, Heimann K. Growth, lipid content, productivity, and fatty acid composition of tropical microalgae for scale-up production. Biotechnology and Bioengineering, 2010, 107 (2): 245–257. pmid:20506156
- 21. Chi Z, Zheng Y, Jiang A, et al. Lipid production by culturing oleaginous yeast and algae with food waste and municipal wastewater in an integrated process. Applied Biochemistry and Biotechnology, 2011, 165 (2): 442–453. pmid:21567213
- 22. Benavente-Valdés JR, Aguilar C, Contreras-Esquivel JC, et al. Strategies to enhance the production of photosynthetic pigments and lipids in chlorophycae species. Biotechnology Reports, 2016, 10: 117–125. pmid:28352532
- 23. Nalley JO, O’Donnell DR, Litchman E. Temperature effects on growth rates and fatty acid content in freshwater algae and cyanobacteria. Algal Research, 2018, 35: 500–507.
- 24. Jiang Y, Chen F. Effects of temperature and temperature shift on docosahexaenoic acid production by the marine microalge Crypthecodinium cohnii. Journal of the American Oil Chemists’ Society, 2000, 77 (6): 613–617.
- 25. Singh RN, Sharma S. Development of suitable photobioreactor for algae production-A review. Renewable and Sustainable Energy Reviews, 2012, 16 (4): 2347–2353.
- 26. Pan JG, Kwak MY, Rhee JS. High density cell culture of Rhodotorulaglutinis using oxygen-enriched air. Biotechnology Letters, 1986, 8 (10): 715–718.