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Lipid Production by a <TEX>$CO_2$</TEX>-Tolerant Green Microalga, Chlorella sp. MRA-1
Lipid Production by a $CO_2$-Tolerant Green Microalga, Chlorella sp. MRA-1
Journal of Microbiology and Biotechnology. 2014. May, 24(5): 683-689
Copyright © 2014, The Korean Society For Microbiology And Biotechnology
  • Received : August 19, 2013
  • Accepted : January 25, 2014
  • Published : May 28, 2014
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About the Authors
Yanlin Zheng
College of Science, Shandong University of Science and Technology, Qingdao 266510, P. R. China
Cheng Yuan
Qingdao Institute of Bioenergy and Bioprocess Technology, Chinese Academy of Sciences, Qingdao 266101, P. R. China
Junhan Liu
Qingdao Institute of Bioenergy and Bioprocess Technology, Chinese Academy of Sciences, Qingdao 266101, P. R. China
Guangrong Hu
Qingdao Institute of Bioenergy and Bioprocess Technology, Chinese Academy of Sciences, Qingdao 266101, P. R. China
Fuli Li
Qingdao Institute of Bioenergy and Bioprocess Technology, Chinese Academy of Sciences, Qingdao 266101, P. R. China
lifl@qibebt.ac.cn

Abstract
Since CO 2 concentrations in industrial flue gases are usually 10%-20%, one of the prerequisites for efficient CO 2 removal by algae is the level of tolerance of microalgal species to exposure to high concentrations of CO 2 . A newly isolated microalgal strain, Chlorella sp. MRA-1, could retain growth with high concentrations of CO 2 up to 15%. The highest lipid productivity for Chlorella sp. MRA-1 was 0.118 g/l/day with a 5% CO 2 concentration. Octadecenoic acid and hexadecanoic acid, the main components of biodiesel, accounted for 70% of the total fatty acids. A lipid content of 52% of dry cell weight was achieved with limited amounts of nitrogen. Chlorella sp. MRA-1 seems to be an ideal candidate for biodiesel production when cultured with high concentrations of CO 2 .
Keywords
Introduction
Biodiesel derived from soybean, windmill palm, rapeseed, and other oil plants has proved eminently suitable as a transport fuel and, because of its nontoxicity, biodegradability, and renewability, continues to generate widespread interest [20 , 22] . Nevertheless, a major obstacle to increasing biodiesel production using these oil plants is their relatively high cost. In addition, growing these plants requires the allocation of large amounts of land and energy resources. Although oil plants already provide a small fraction of the liquid fuel demanded by our transportation systems, biodiesel production from oil plants still faces stiff competition from entrenched fossil fuel industries [16 , 22] .
Because of its higher lipid productivity and photosynthetic efficiencies in comparison with oil plants, microalgal lipids are currently regarded as the third-generation feedstock for sustainable biodiesel production [6 , 7] . Furthermore, microalgae cultivation does not compete with food sources and can generate valuable co-products [31 , 33] . Generally, phototrophic microalgal growth requires CO 2 as a carbon source. In recent years, bioregenerative methods, particularly those using microalgae photosynthesis, have been implemented to reduce atmospheric CO 2 to ensure a safe and reliable living environment [11 , 24] . Absorption of CO 2 using microalgae could convert CO 2 into microalgae biomass [24 , 30] , and producing 100 tons of algal biomass fixes roughly 183 tons of CO 2 [6] . At the same time, flue gases from power plants contain 10%-20% (v/v) CO 2 , which may provide a carbon source for large-scale microalgal cultivation [36] . Direct utilization of flue gas reduces the cost of pretreatment, but imposes extreme conditions on microalgae–such as high concentrations of CO 2 . Although most microalgae grow well under conditions of CO 2 concentrations from 1% to 5%, only a few highly CO 2 -tolerant species able to withstand high CO 2 concentrations (> 5%) have been found [1 , 8 , 15 , 33] .
For biodiesel production, the lipid content is another important factor in selecting microalgae species. Many microalgae can accumulate lipids due to excess photosynthesis, and some species can accumulate large amounts of lipids from heterotrophic or environmental stress factors, such as nutrient deficiency [28] . In this study, the newly isolated microalgal strain Chlorella sp. MRA-1 was evaluated for its CO 2 tolerance, and the effects of CO 2 and nitrogen concentrations on growth and lipid accumulation were investigated.
Materials and Methods
- Strain and Culturing Conditions
Chlorella sp. MRA-1 was isolated from a wastewater pond in Qingdao, China, and conserved at the China General Microbiological Culture Collection Center (CGMCC 4652; China). The strain was cultivated in a 500 ml glass bubble column (30 mm in diameter) containing 300 ml of BG-11 medium with 1.5 g/l NaNO 3 . The columns were maintained at 25 ± 2℃, bubbled with sterile gas composed of air supplemented with varying CO 2 concentrations (5%-30%). Trichromatic lamps (Y228-T5; NVC Lighting Technology Corporation, China), with spectra ranging from 380 to 780 nm, were used as light sources. Microalgal cells were grown under low illumination (50 μmol photons m -2 s -1 ) for 3 days, and then subjected to high illumination (220 μmol photons m -2 s -1 ) for another 10 days [19] .
To assess the effects of different nitrogen concentrations on the growth and lipid accumulation of microalgae, we prepared four samples with an initial NaNO 3 concentration of 0.375, 2.5, 5, and 10 g/l; and blowing air supplemented with a 5% CO 2 concentration. The growth of microalgae was monitored using a UV/VIS spectrophotometer at 750 nm (UNICO 2600, Shanghai, China), and the final biomass was determined by measuring the dry cell weight (DCW). After 13 days, a 5 ml microalgae sample was taken and filtered through preweighted 0.8 μm microporous filter paper. The filter paper was oven-dried for 6 h at 105℃. The difference between the final weight and the weight of the paper before filtration was taken as the DCW.
- Lipid Extraction
Microalgal cells were harvested by centrifugation at 3,000 rpm for 10 min. A freeze-drying procedure was performed using a vacuum freeze dryer (Alpha1-2LD plus; Martin Christ GmbH, Osterode, Germany) to get dry algal powder. The lipids were extracted as previously described [3] , with modifications. Four milliliters of chloroform and 2 ml of methanol were added to a glass tube containing 50 mg of dry algal powder. The mixture was shaken at 180 rpm at 30℃ for 12 h, and then centrifuged at 3,000 rpm for 10 min. The supernatant was transferred to a new glass tube, and 2 ml of methanol and 3.6 ml of water were added to make the final ratio of chloroform:methanol:water to be 10:10:9 (v/v/v). Further centrifugation of this mixture at 3,000 rpm for 10 min produced two distinct layers. The chloroform layer was transferred into a preweighted glass tube and removed at 60℃ under the protection of N 2 . The lipid was dried in a vacuum-drying oven (Liantian DZF-6050, Hangzhou, China) at 0.09 Mpa, 60℃, for 2 h. The final weight was measured using an electronic balance (0.01 mg: XS105 DualRange; Mettler Toledo, Zurich, Switzerland). Extraction was performed in duplicate for each sample.
- Analysis of Fatty Acid Composition
Transesterification was performed by incubating the total lipids sample in 2 ml of methanol containing 2% (v/v) H 2 SO 4 for 2.5 h at 85℃. After cooling to room temperature, 1 ml of HPLC-grade hexane and 1 ml of saturated NaCl solution were added. The mixture was centrifuged for 10 min at 3,000 rpm, and the upper layer containing fatty acid methyl esters (FAMEs) was obtained for further analysis. FAME analysis was performed with a gas chromatograph (Varian 450-GC; Varian Inc., USA) using a fused CP-WAX 58 column (25 m × 0.25 mm). The carried gas was helium, and 1 μl of methyl ester sample solution was injected for analysis. The split ratio was 1:30. The temperature program was as follows: column temperature was maintained at 100℃ for 2min and then elevated to 250℃ at a rate of 10℃/min and maintained for a further 3 min. The injector temperature was set at 250℃. The flame-ionization detector temperature was set at 280℃. Fatty acids were identified by comparing the retention time obtained with the analytical standard FAME mixture C8-C24 (Sigma-Aldrich, Shanghai, China).
- Elemental Analysis
The elemental composition (C, H, N, and S) of microalgae biomass under different conditions was analyzed using Vario EL (Elementar Analysensysteme GmbH, Hanau, Germany) with helium as the carrier gas. The combustion temperature and oxygen pressure were 1,150℃ and 0.25 MPa, respectively.
- Carbon Dioxide Fixation Rate
The carbon dioxide fixation rate of microalgae can be calculated by the following equation [35] :
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where X max and X o represent maximum dry cell weight and initial inoculated dry cell weight (mg/l); t stands for the time required to reach the maximum dry cell weight; and C is the carbon content of the dry cell biomass per the element analyzer found in Table 2 . M CO2 and M C represent the molecular weight of CO 2 and elemental carbon, respectively.
Results
- Cultivation and Lipid Production of Chlorella sp. MRA-1 with Different Concentrations of CO2
Chlorella sp. MRA-1 could grow in the presence of 5% to 20% CO 2 and reached a stationary stage after 10 days ( Fig. 1 ). The maximum biomass concentration of 4.48 ± 0.30 g/l was achieved with 5% CO 2 . With 10% and 20% CO 2 , biomasses of 3.52 ± 0.17 and 3.20 ± 0.29 g/l were obtained, respectively. After 13 days, the lipid contents and lipid yields of strain MRA-1 (grown with different CO 2 concentrations) were compared ( Fig. 2 ). The highest lipid yield of 1.53 g/l was obtained when cultured with 5% CO 2 . When the CO 2 concentration was increased, the lipid yield decreased greatly ( Fig. 2 ). Lipid yields of the cells grown with CO 2 concentrations of 10% and 20% were 1.26 and 0.79 g/l, respectively.
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Growth of Chlorella sp. MRA-1 under different CO2 concentrations in BG-11 medium with 1.5 g/l NaNO3.
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Algae biomass, lipid yield, and lipid content of Chlorella sp. MRA-1 in BG-11 medium with 1.5 g/l NaNO3 under different CO2 concentrations
- Effects of Different Nitrogen Concentrations on the Growth and Lipid Accumulation of Chlorella sp. MRA-1
To improve the lipid productivity, the effects of different nitrogen concentrations on the growth and lipid accumulation of Chlorella sp. MRA-1 were investigated ( Fig. 3 ). The maximum biomass concentration of 4.14 ± 0.31 g/l was achieved in 13 days when the alga was grown in BG-11 medium with 5 g/l NaNO 3 . Microalgal cells were collected, and extractable lipid contents (% DCW) were determined by the gravimetric method. The lipid contents and productivities of Chlorella sp. MRA-1, grown with different concentrations of NaNO 3 , are shown in Fig. 4 . Strain MRA-1 showed the highest lipid content of 52.1% DCW with 0.375 g/l NaNO 3 . The lipid contents of the cells grown with 2.5, 5, and 10 g/l NaNO 3 were significantly lower than with 0.375 g/l NaNO 3 . As has been shown, nitrogen limitation can stimulate lipid accumulation in Chlorella sp. MRA-1. In this study, the maximum lipid yield of 1.87 g/l was achieved with a nitrogen limitation of 0.375 g/l NaNO 3 .
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Growth of Chlorella sp. MRA-1 with different nitrogen concentrations in BG-11 medium with 5% CO2.
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Algae biomass, lipid yield, and lipid content of Chlorella sp. MRA-1 grown in BG-11 medium with different concentrations of NaNO3 with 5% CO2.
- Fatty Acid Composition of Chlorella sp. MRA-1 Grown with Different CO2and NaNO3Concentrations
The fatty acid composition of Chlorella sp. MRA-1 grown with different CO 2 and NaNO 3 concentrations was analyzed using GC ( Table 1 ). The major fatty acid components for all cells grown under different conditions were octadecenoic acid and hexadecanoic acid, constituting 70% of the total fatty acid content. The fatty acid profiles of total lipids were similar for Chlorella sp. MRA-1 grown with different concentrations of NaNO 3 . However, the proportion of monounsaturated fatty acids that included C16:1, C18:1, and C20:1 reached 60.43% of the total lipid composition when strain MRA-1 was cultured with 10 g/l NaNO 3 . This amount was 11%-14% higher than for the cells grown with 0.375, 2.5, and 5 g/l NaNO 3 .
Fatty acid composition ofChlorellasp. MRA-1 grown with different CO2and NaNO3concentrations.
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Fatty acid composition of Chlorella sp. MRA-1 grown with different CO2 and NaNO3 concentrations.
- Element Analysis and Carbon Dioxide Fixation Rate
The levels of carbon, nitrogen, hydrogen, and sulfur in Chlorella sp. MRA-1 grown with different CO 2 and NaNO 3 concentrations were analyzed ( Table 2 ). The carbon content was 53.72% ± 1.30% when grown with 0.375 g/l NaNO 3 , which was higher than that found in cells grown with sufficient nitrogen. Cultivation with high concentrations of CO 2 (10% and 20%) also led to microalgae cells exhibiting a carbon content greater than 56%. However, the highest C/N ratio of 21.78 ± 1.51 was obtained when the cells were cultured with 0.375 g/l NaNO 3 . This indicated that nitrogen deficiency could induce Chlorella sp. MRA-1 to produce more lipid than CO 2 stress.
Elemental analysis ofChlorellasp. MRA-1 grown with different CO2and NaNO3concentrations.
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Data are reported as means ± standard deviation of triplicates.
Tolerable concentration of CO2and biomass yield by microalgae.
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NA: not available.
The carbon dioxide fixation rate was compared when this strain was cultured with different CO 2 concentrations ( Table 4 ). The maximum CO 2 fixation rate of Chlorella sp. MRA-1 was 710.7 mg/l/day when cultured with 5% CO 2 . The CO 2 fixation rate declined when higher levels of CO 2 were supplied.
Carbon dioxide fixation rate ofChlorellasp. MRA-1 in this work.
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Carbon dioxide fixation rate of Chlorella sp. MRA-1 in this work.
Discussion
Waste gases from thermal power stations contain 10%-20% (v/v) CO 2 , which may provide a carbon source for microalgae cultivation. Several microalgal species have been tested with high CO 2 concentrations ( Table 3 ). Chlorococcum littorale could grow with 60% CO 2 using the stepwise adaptation technique [5] . Another high CO 2 -tolerant species is Euglena gracilis whose growth was enhanced under 5%-45% of CO 2 . Scenedesmus sp. could grow with 80% CO 2 , but maximum cell mass was observed with 10%-20% CO 2 [13] . It is also reported that some species such as Chlorella sp. and Cyanidium sp. could even grow with 100% CO 2 [2 , 21] .
Hu et al . [14] summarized the total lipid contents of oleaginous green algae reported in the literature, which showed an average total lipid content of 25.5% DCW. Mata et al . [23] suggested Chlorella sp. to be a good option for biodiesel production, according to a wide range of literature. In a previous study reported by Demorais and Costa [9] , Chlorella kessleri isolated from a coal-fired thermoelectric power plant showed a maximum biomass productivity of 0.087 g/l/day with 6% CO 2 , even growing in a medium containing up to 18% CO 2 . Tang et al . [29] reported that a lipid content of 20.65% DCW was achieved by a CO 2 -tolerant microalga, Chlorella sorokiniana CS-01, when cultured with 5% CO 2 [29] . The lipid content of Chlorella vulgaris grown with 10% CO 2 was found to be less than 11.92% DCW [32] . In the present study, it was shown that Chlorella sp. MRA-1 could grow with 5%-20% CO 2 , with the best growth (0.34 g/l/day) achieved at 5% CO 2 . The highest CO 2 fixation rate was achieved when the strain was grown with 5% CO 2 . Lipid content and lipid productivity of Chlorella sp. MRA-1, when cultured with 5% CO 2 , were 34.1% DCW and 116 mg/l/day, respectively.
A high content of algal lipid increases the process yield coefficient and reduces the cost of extraction and purification per unit product [4] . Algal lipids respond to nitrogen deprivation stress and CO 2 enrichment in a heterogeneous fashion. Pratt and Johnson [25] proposed that lipid synthesis was promoted at high CO 2 levels in Chlorella . In this study, we also found that a higher lipid content was achieved with higher CO 2 concentrations. On the other hand, it is known that nitrogen deprivation promotes lipid accumulation [17] . In the present study, Chlorella sp. MRA-1 accumulated more lipid through nitrogen limitation; the highest lipid content of 52.1% DCW was obtained when cells were grown in BG-11 medium with 0.375 g/l NaNO 3 -one-fourth the normal nitrogen concentration.
The unsaturation degree of fatty acids in Chlorella vulgaris was inversely related to the CO 2 concentration. Tsuzuki et al . [30] reported that the unsaturation levels of fatty acids in C. vulgaris were greater in low-CO 2 cells than in high-CO 2 cells, indicating a shift of the relative content of saturated and unsaturated fatty acids with a change in CO 2 concentrations. In this study, we also found that the contents of unsaturated fatty acid (monounsaturated fatty acids and polyunsaturated fatty acids) were greater in low-CO 2 cells than in high-CO 2 cells in Chlorella sp. MRA-1. Moreover, the contents of monounsaturated fatty acids in lipids were lower under nitrogen starvation conditions, which is similar to Tetraselmis subcordiformis in previous reports where the major increase in fatty acids under nitrogen deprivation conditions was of the monounsaturated type [26] . An additional characteristic of oleaginous microalgae is the suitability of lipids for biodiesel in terms of the type and amount produced by a microalgal species ( e.g ., chain length, degree of saturation) [12] . This study confirms that the major components of the lipids from Chlorella sp. MRA-1 are suitable for biodiesel production.
In conclusion, the newly isolated strain Chlorella sp. MRA-1, with its tolerance to high concentrations of CO 2 and high lipid productivity, could efficiently exploit flue gases for biodiesel production. We also found that nitrogen deficiency effectively induced the strain to produce more lipid than CO 2 stress. Chlorella sp. MRA-1 seems to be an ideal candidate for biodiesel production when cultured with high concentrations of CO 2 .
Acknowledgements
This study was supported by grants from the National Science Foundation of China (U1232126) and the Key Research Program of Shandong Province (2012GSF12123).
References
Andersen T , Andersen F 2006 Effects of CO2concentration on growth of filamentous algae and Littorella uniflora in a Danish softwater lake. Aquat. Bot. 84 267 - 271    DOI : 10.1016/j.aquabot.2005.09.009
Arancibia-Avila P , Coleman JR , Russin WA , Wilcox LW , Graham JM , Graham LE 2000 Effects of pH on cell morphology and carbonic anhydrase activity and localization in bloom-forming Mougeotia (Chlorophyta, Charophyceae). Can. J. Bot. 78 1206 - 1214
Bligh EG , Dyer WJ 1959 A rapid method of total lipid extraction and purification. Can. J. Biochem. Physiol. 377 911 - 917    DOI : 10.1139/o59-099
Borowitzka MA 1992 Algal biotechnology products and processes - matching science and economics. J. Appl. Phycol. 4 267 - 279    DOI : 10.1007/BF02161212
Chihara M , Nakayama T , Inouye I , Kodama M 1994 Chlorococcum littorale, a new marine green coccoid alga (Chlorococcales, Chlorophyceae). Arch. Protistenkunde 144 227 - 235    DOI : 10.1016/S0003-9365(11)80133-8
Chisti Y 2007 Biodiesel from microalgae. Biotechnol. Adv. 25 294 - 306    DOI : 10.1016/j.biotechadv.2007.02.001
Chisti Y 2008 Biodiesel from microalgae beats bioethanol. Trends Biotechnol. 26 126 - 131    DOI : 10.1016/j.tibtech.2007.12.002
Chiu S , Kao C , Tsai M , Ong S , Chen C , Lin C 2009 Lipid accumulation and CO2utilization of Nannochloropsis oculata in response to CO2aeration. Bioresour. Technol. 100 833 - 838    DOI : 10.1016/j.biortech.2008.06.061
Demorais M , Costa J 2007 Isolation and selection of microalgae from coal fired thermoelectric power plant for biofixation of carbon dioxide. Energ. Convers. Manage. 48 2169 - 2173    DOI : 10.1016/j.enconman.2006.12.011
Doucha J , Straka F , Livansky K 2005 Utilization of flue gas for cultivation of microalgae (Chlorella sp.) in an outdoor open thin-layer photobioreactor. J. Appl. Phycol. 17 403 - 412    DOI : 10.1007/s10811-005-8701-7
Fernandez FGA , Gonzalez-Lopez CV , Sevilla JMF , Grima EM 2012 Conversion of CO2into biomass by microalgae: how realistic a contribution may it be to significant CO2removal? Appl. Microbiol. Biotechnol. 96 577 - 586    DOI : 10.1007/s00253-012-4362-z
Griffiths MJ , Harrison STL 2009 Lipid productivity as a key characteristic for choosing algal species for biodiesel production. J. Appl. Phycol. 21 493 - 507    DOI : 10.1007/s10811-008-9392-7
Hanagata N , Takeuchi T , Fukuju Y , Barnes DJ , Karube I 1992 Tolerance of microalgae to high CO2and hightemperature. Phytochemistry 31 3345 - 3348    DOI : 10.1016/0031-9422(92)83682-O
Hu Q , Sommerfeld M , Jarvis E , Ghirardi M , Posewitz M , Seibert M , Darzins A 2008 Microalgal triacylglycerols as feedstocks for biofuel production: perspectives and advances. Plant J. 54 621 - 639    DOI : 10.1111/j.1365-313X.2008.03492.x
Jiang LL , Luo SJ , Fan XL , Yang ZM , Guo RB 2011 Biomass and lipid production of marine microalgae using municipal wastewater and high concentration of CO2. Appl. Energy 88 3336 - 3341    DOI : 10.1016/j.apenergy.2011.03.043
Lang X , Dalai AK , Bakhshi NN , Reaney MJ , Hertz PB 2001 Preparation and characterization of bio-diesels from various bio-oils. Bioresour. Technol. 80 53 - 62    DOI : 10.1016/S0960-8524(01)00051-7
Larson TR , Rees TAV 1996 Changes in cell composition and lipid metabolism mediated by sodium and nitrogen availability in the marine diatom Phaeodactylum tricornutum (Bacillariophyceae). J. Phycol. 32 388 - 393    DOI : 10.1111/j.0022-3646.1996.00388.x
Lee JS , Sung KD , Kim MS , Park SC , Lee KW 1996 Current aspects of carbon dioxide fixation by microalgae in Korea. Abstr. Pap. Am. Chem Soc. 212 119 -
Liu J , Yuan C , Hu G , Li F 2012 Effects of light intensity on the growth and lipid accumulation of microalga Scenedesmus sp. 11-1 under nitrogen limitation. Appl. Biochem. Biotechnol. 166 2127 - 2137    DOI : 10.1007/s12010-012-9639-2
Liu ZH , Shao HB 2010 Comments: main developments and trends of international energy plants. Renew. Sustain. Energy Rev. 14 530 - 534    DOI : 10.1016/j.rser.2009.08.009
Maeda K , Owada M , Kimura N , Omata K , Karube I 1995 CO2fixation from the flue-gas on coal-fired thermal powerplant by microalgae. Energy Convers. Manage. 36 717 - 720    DOI : 10.1016/0196-8904(95)00105-M
Mandal S , Mallick N 2009 Microalga Scenedesmus obliquus as a potential source for biodiesel production. Appl. Microbiol. Biotechnol. 84 281 - 291    DOI : 10.1007/s00253-009-1935-6
Mata TM , Martins AA , Caetano NS 2010 Microalgae for biodiesel production and other applications: a review. Renew. Sustain. Energy Rev. 14 217 - 232    DOI : 10.1016/j.rser.2009.07.020
Miron AS , Garciia MCC , Gomez AC , Camacho FG , Grima EM , Chisti Y 2003 Shear stress tolerance and biochemical characterization of Phaeodactylum tricornutum in quasi steady-state continuous culture in outdoor photobioreactors. Biochem. Eng. J. 16 287 - 297    DOI : 10.1016/S1369-703X(03)00072-X
Pratt R , Johnson E 1964 Lipid content of Chlorella “aerated” with a CO2-nitrogen versus a CO2-air mixture. J. Pharm. Sci. 53 1135 - 1136    DOI : 10.1002/jps.2600530942
Huang XX , Huang ZZ , Wen W , Yan JQ 2013 Effects of nitrogen supplementation of the culture medium on the growth, total lipid content and fatty acid profiles of three microalgae (Tetraselmis subcordiformis, Nannochloropsis oculata and Pavlova viridis). J. Appl. Phycol. 25 129 - 137    DOI : 10.1007/s10811-012-9846-9
Sydney EB , Sturm W , de Carvalho JC , Thomaz-Soccol V , Larroche C , Pandey A , Soccol CR 2010 Potential carbon dioxide fixation by industrially important microalgae. Bioresour. Technol. 101 5892 - 5896    DOI : 10.1016/j.biortech.2010.02.088
Takagi M , Karseno , Yoshida T 2006 Effect of salt concentration on intracellular accumulation of lipids and triacylglyceride in marine microalgae Dunaliella cells. J. Biosci. Bioeng. 101 223 - 226    DOI : 10.1263/jbb.101.223
Tang DH , Han W , Li PL , Miao XL , Zhong JJ 2011 CO2biofixation and fatty acid composition of Scenedesmus obliquus and Chlorella pyrenoidosa in response to different CO2levels. Bioresour. Technol. 102 3071 - 3076    DOI : 10.1016/j.biortech.2010.10.047
Tsuzuki M , Ohnuma E , Sato N , Takaku T , Kawaguchi A 1990 Effects of CO2concentration during growth on fattyacid composition in microalgae. Plant Physiol. 93 851 - 856    DOI : 10.1104/pp.93.3.851
Wang B , Li Y , Wu N , Lan CQ 2008 CO2bio-mitigation using microalgae. Appl. Microbiol. Biotechnol. 79 707 - 718    DOI : 10.1007/s00253-008-1518-y
Yoo C , Jun SY , Lee JY , Ahn CY , Oh HM 2010 Selection of microalgae for lipid production under high levels of carbon dioxide. Bioresour. Technol. 101 S71 - S74    DOI : 10.1016/j.biortech.2009.03.030
Yuan C , Liu J , Fan Y , Ren X , Hu G , Li F 2011 Mychonastes afer HSO-3-1 as a potential new source of biodiesel. Biotechnol. Biofuels 4 47 -    DOI : 10.1186/1754-6834-4-47
Yue L , Chen W 2005 Isolation and determination of cultural characteristics of a new highly CO2tolerant fresh water microalgae. Energy Convers. Manage. 46 1868 - 1876    DOI : 10.1016/j.enconman.2004.10.010
Yun YS , Lee SB , Park JM , Lee CI , Yang JW 1997 Carbon dioxide fixation by algal cultivation using wastewater nutrients. J. Chem. Technol. Biotechnol. 69 451 - 455
Zeiler KG , Heacox DA , Toon ST , Kadam KL , Brown LM 1995 The use of microalgae for assimilation and utilization of carbon-dioxide from fossil fuel-fired power-plant flue-gas. Energy Convers. Manage. 36 707 - 712    DOI : 10.1016/0196-8904(95)00103-K
Zhang K , Miyachi S , Kurano N 2001 Evaluation of a vertical flat-plate photobioreactor for outdoor biomass production and carbon dioxide bio-fixation: effects of reactor dimensions, irradiation and cell concentration on the biomass productivity and irradiation utilization efficiency. Appl. Microbiol. Biotechnol. 55 428 - 433    DOI : 10.1007/s002530000550