- Original Article
- Published:
Activity of acetyl-CoA carboxylase is not directly linked to accumulation of lipids when Chlorella vulgaris is co-immobilised with Azospirillum brasilense in alginate under autotrophic and heterotrophic conditions
Annals of Microbiology volume 65, pages 339–349 (2015)
Abstract
Activity of acetyl-CoA carboxylase (ACCase) and lipid accumulation were assayed in the microalga Chlorella vulgaris co-immobilised in alginate beads with Azospirillum brasilense, under autotrophic and heterotrophic growth conditions, with and without ammonium starvation. ACCase is a key enzyme in de novo fatty acid biosynthesis. Under the two growth conditions, co-immobilisation always enhanced the activity of ACCase and yielded a higher level of lipids when compared with immobilisation of the alga alone. The highest lipid content obtained under autotrophic conditions was with ammonium starvation. Cultivation under heterotrophic conditions without limitation of nitrogen, with or without the presence of bacteria, yielded a higher growth rate and accumulated more lipids than under autotrophic conditions. No correlation was found between total lipids and ACCase activity. Unusually, ammonium starvation significantly reduced lipid accumulation under heterotrophic conditions. Consequently, co-immobilisation, sufficient ammonium and heterotrophic growth conditions were the most significant parameters for lipid accumulation and ACCase activity in C. vulgaris where the two latter parameters are not directly linked.
Introduction
The genus Chlorella is a commonly studied unicellular, non-motile, green microalga inhabiting aquatic environments. Many microalgae have diverse applications in high-value, low-volume compounds, such as pigments for the food industry, products for the health food market, human and animal foodstuffs, applications for wastewater treatments, and, potentially, as future biofuels (Lebeau and Robert 2006; de-Bashan and Bashan 2010; Mata et al. 2010). Azospirillum spp. are bacteria with known plant growth promoters that enhance the performance of many plant and algal species, including the unicellular Chlorella spp. (Bashan et al. 2004). This enhancement occurs via many simultaneously operating mechanisms, in tandem or cascading, a process recently termed “Multiple Mechanisms Theory” (Bashan and de-Bashan 2010). Among the recorded effects of the bacteria on Chlorella spp. during co-immobilisation are increase in population (Gonzalez and Bashan 2000), increase in nitrogen and phosphorus metabolism (de-Bashan et al. 2002b; 2004; Hernandez et al. 2006; de-Bashan et al. 2008b; Perez-Garcia et al. 2010; Covarrubias et al. 2012), lipid accumulation and effects on fatty acid and pigment production (de-Bashan et al. 2002a), enhanced carbohydrate and starch accumulation (Choix et al. 2012a, b), and mitigation of negative effects of pH (de-Bashan et al. 2005) or excess tryptophan (de-Bashan and Bashan 2008).
Chlorella vulgaris grows under both autotrophic and heterotrophic conditions. Under heterotrophic conditions, glycerol (O’Grady and Morgan 2011), Na-acetate (Perez-Garcia et al. 2011), and glucose (Wan et al. 2012) can be used as carbon sources. Heterotrophic cultures of two microalgae have been used to produce polyunsaturated fatty acids (PUFAs) on a commercial scale, and five species of Chlorella produced pigments, lipids, antioxidants, L-ascorbic acid, and polysaccharides on an experimental scale (de-Bashan et al. 2002a; Bumbak et al. 2011; Choix et al. 2012b).
Immobilisation of microorganisms, including microalgae and Azospirillum (each species separately), is a common biotechnological practice for many agricultural and industrial applications (Bashan 1986, 2002; Prasad and Kadokawa 2009). Co-immobilisation of Chlorella spp. with A. brasilense has been proposed as a potential technology for wastewater treatment (de-Bashan et al. 2002b; 2004; Cruz et al. 2013) and a model to study interaction between eukaryotic and prokaryotic cells (de-Bashan and Bashan 2008; de-Bashan et al. 2011).
Cells of microalgae contain lipids in the range of 4–65 % (Gouveia and Oliveira 2009) and those of C. vulgaris within the range of 5–58 % (Mata et al. 2010). Although almost all of this is usually located in the membranes, many microalgae accumulate neutral lipids over membrane lipids under certain growth conditions. In plants (Ohlrogge and Browse 1995; Francki et al. 2002; Klaus et al. 2004), as well as in microalgae (Radakovits et al. 2010), the most abundant lipids are derived from fatty acid and glycerolipid biosynthetic pathways.
In plants and algae, ACCase is found in plastids, where primary fatty acid biosynthesis occurs, and in the cytosol, where synthesis of very long-chain fatty acids and flavonoids occurs (Liu et al. 2007; Sato and Moriyama 2007; Yu et al. 2007). Several studies have shown an association between ACCase activity and accumulation of lipids. One study demonstrates that ACCase is the control point in lipid biosynthesis in potato tubers (Klaus et al. 2004). Inhibition of ACCase leads to reduced fatty acid synthesis in lipogenic tissues in mammals (Tong and Hardwood 2006). Increase of ACCase activity in E. coli leads to greater synthesis of fatty acids (James and Cronan 2004). The rate of synthesis of fatty acids in spinach changes greatly with light and dark regimes by activating or inactivating ACCase (Sasaki and Nagano 2004). In microalgae (diatoms), ACCase activity was detected, but it was not directly correlated to accumulation of lipids (Sheehan et al. 1998).
Nitrogen starvation commonly induces accumulation of lipids in several microalgae under autotrophic conditions (Xiong et al. 2010; Tang et al. 2011; Přibyl et al. 2012), and co-immobilisation of Chlorella vulgaris and Azospirillum brasilense affects several metabolic pathways in the microalga as described above. We hypothesised, therefore, that these factors will also enhance lipid accumulation and activity of ACCase under autotrophic and heterotrophic conditions and ACCase activity is linked to accumulation of lipids. Consequently, the objectives of this study were to: (1) measure the effect of immobilisation of C. vulgaris with A. brasilense on the activity of ACCase and accumulation of lipid, (2) measure the effect of ammonium starvation on this prokaryote–eukaryote interaction, (3) determine whether growth under autotrophic (illuminated) and heterotrophic (dark) conditions affects accumulation of lipids and ACCase activity during this interaction, and (4) find whether changes in activity of ACCase is directly linked to accumulation of lipids in C. vulgaris.
Materials and methods
Microorganisms and culture conditions
Chlorella vulgaris Beijerinck (UTEX 2714, University of Texas, Austin, TX, USA) and Azospirillum brasilense Cd (DSM 1843; Leibniz-Institut DMSZ, Braunschweig, Germany) were used in all experiments. C. vulgaris was cultured for 7 days in mineral growth media (C30; Gonzalez et al. 1997) and agitated at 140 rpm in an orbital shaker, 28 ± 1 °C, and 60 μmoles photon m−2 s−1. Medium C30 composed of (in g L−1): KNO3 (25), MgSO4·7H2O (10), KH2PO4 (4), K2HPO4 (1), FeSO4·7H2O (1) and (in μg L−1): H3BO3 (2.86), MnCl2·4H2O (1.81), ZnSO4·7H2O (0.11), CuSO4·5H2O (0.09), and NaMoO4 (0.021). A. brasilense was cultured for 18 h in nutrient broth (NB; #N7519 Fluka; Sigma-Aldrich, St. Louis, MO, USA) at 37 ± 1 °C and agitated at 140 rpm.
Immobilisation of microalgae and bacteria in alginate beads
Microorganisms were immobilised using the method described by de-Bashan et al. (2004), where 40 mL C. vulgaris culture (6.0 × 106 cells mL−1) was mixed with 160 mL of a sterile, 6,000 cP 2 % alginate solution (i.e., alginate mixed at 14,000 cP and 3,500 cP), and stirred for 15 min. Using an automatic bead maker, this mixture was dropped into a 2 % CaCl2 solution under slow stirring (de-Bashan and Bashan 2010). The beads formed were stabilised for 1 h at 28 ± 1 °C and washed in sterile saline solution. Azospirillum brasilense (approximately 1.0 × 109 CFU mL−1) was immobilised similarly. The immobilisation normally reduces the number of organisms in the beads; therefore, a second incubation step was necessary (10 % NB overnight). For starvation conditions of A. brasilense, N-free OAB medium was used for the second incubation step (Bashan et al. 1993). To combine both species in the same beads, a similar procedure was performed, using 20 mL of each culture in a mixture (total of 40 mL). After the second incubation the beads were placed in 1-L Erlenmeyer flasks (40 g of beads per flask) containing 500 mL of synthetic growth medium (SGM; de-Bashan et al. (2011). SGM medium contains (in mg L−1): NaCl (7), CaCl2 (4), MgSO4·7H2O (2), K2HPO4 (217), KH2PO4 (8.5), Na2HPO4 (33.4), and NH4Cl; (191). The flasks were placed in an orbital shaker for 6 days under the same conditions as described for culturing Chlorella. In the starvation experiments using the microalgae, the N-free SGM medium was used.
Autotrophic and heterotrophic experimental conditions
For autotrophic experiments, the flasks were incubated in an orbital shaker using the same light and temperature conditions described for culturing C. vulgaris. For heterotrophic conditions, the preculture was maintained in the dark without nitrogen for 24 h (Choix et al. 2012b), and during the experiments, the culture was maintained in total darkness at 28 ± 1 °C, using 10 g L−1 of sodium acetate (#S7670; Sigma-Aldrich) as a carbon source (Choix et al. 2012a, b) and nitrogen (5 mM ammonium, 90 mg L−1) and phosphorus (phosphate, 0.44 mM or 42 mg L−1).
Samples
From each Erlenmeyer flask, 40 g of beads were taken (the beads swell when placed in the SGM) in 50-mL Corning tubes and frozen at −80 °C. These samples were used for all analyses listed below and in all experiments.
Counting microorganisms after treatment
After each experiment, beads containing microorganisms were dissolved in 4 % sodium bicarbonate solution at room temperature (∼28 °C) for ∼30 min., then microorganisms were counted. C. vulgaris was counted under a light microscope with a Neubauer hemocytometer (Gonzalez and Bashan 2000) connected to an image analyser (Image ProPlus 4.5; Media Cybernetics, Silver Spring, MD, USA). Growth rate (μ) of C. vulgaris was defined by: μ = (lnNt 1 – lnNt 0) / (t 1 – t 0), where Nt 1 is the number of cells at sampling time and Nt 0 is the number of cells at the beginning of the experiment, t 1 is the sampling time, and t 0 is the beginning of the experiment (Oh-Hama and Miyachi 1992). A. brasilense was counted after serial dilution by the plate count method on nutrient agar medium (#M7519; Sigma-Aldrich).
Quantification of lipids
Standard curve for lipids: The quantity of lipids was measured following the method described by Pande et al. (1963). Extraction of lipids followed the standard method described by Bligh and Dyer (1959) with modifications involving sonication to break down cell walls. Briefly, lipids were extracted by adding 4 mL methanol/chloroform solution (2:1, v/v) to dry beads. The beads were sonicated for 10 min (2 cycles of 5 min at 30 kHz) in an ice bath. The sonicated beads were incubated at 4 °C for 24 h in the dark and this procedure (only sonication) was repeated under the same conditions. The sample was then centrifuged (5,000 g, 20 min, 4 °C) and the supernatant was transferred to a clean tube. The rest of the analysis was done as originally described.
Quantification of lipids: Lipid assays, based on a potassium dichromate colour change reaction, were done according to Pande et al. (1963), using a calibration curve with tripalmitin (#T5888; Sigma-Aldrich), as a standard. The concentration of lipids was determined in a microplate reader (Molecular Devices, Sunnyvale, CA, USA) at 590 nm, recording the intensity of the green colour formed. Potassium dichromate has a yellow-reddish colour before the reaction and yellow-green after the reaction with lipids. The method quantified lipids in the range of 70 μg to 1.33 mg.
Enzymatic activity of ACCase
Extraction: Frozen bead aliquots were dissolved in two volumes of 4 % solution of NaHCO3 for 40 min at room temperature. Each suspension was then centrifuged (5,000 g, 10 min, 4 °C), the supernatant was discarded and the pellet was washed twice in 0.85 % NaCl and centrifuged again. The pellet was frozen with liquid nitrogen and pulverised with pestle and mortar. Preliminary analyses using sonication (5 × 1 min, 30 kHz with 1 min incubation on ice between sonications, 9 min total) yielded identical enzymatic activity results compared to the pestle and mortar technique that was generally used for convenience. For resuspension, 5 mL extraction buffer [100 mM Tris–HCl pH 8.2, 4 mM ethylenediaminetetraacetic acid (EDTA), 10 mM dithiothreitol (DTT), and 1 mM phenylmethanesulfonyl fluoride (PMSF, #P7626; Sigma-Aldrich)] was added to the pellet. This was then centrifuged for 30 min at 10,500 g at 4 °C. The pellet was discarded and the supernatant was used as a crude extract for enzymatic reactions (de-Bashan et al. 2008a).
Quantification: The reaction buffer was composed of 50 mM Tris–HCl pH 7.5, 6 μM acetyl-CoA, 2 mM ATP, 7 mM KHCO3, 8 mM MgCl2, 1 mM DTT, and 1 mg mL−1 of bovine serum albumin (BSA; #B4287; Sigma-Aldrich). The crude extract was pre-incubated (30 min, 25 °C) with 10 mM potassium citrate and 2 mg mL−1 BSA. Then, 200 μL crude extract was added to 0.8 mL of reaction buffer and the enzymatic reaction was incubated for 1 h at 30 °C. The reaction was stopped with 0.5 mL 10 % perchloric acid (PCA, #244252; Sigma-Aldrich). The total reaction mix was filtered (0.22-μm membrane filter; EMD Millipore, Billerica, MA, USA). Then, 500 μL of this mixture was transferred to a 1.5-mL glass vial and injected into the HPLC according to the method described by Levert et al. (2002), using a Zorbax Eclipse Plus C-18 column (4.6 μm and 5 × 150 mm; Agilent Technologies, Santa Clara, CA, USA). The flow rate was 1 mL min−1 and the UV detector was adjusted to 262 nm. Solution A was 10 mM KH2PO4 at pH 6.7 and solution B was absolute methanol. The analysis was done in triplicate with two controls; in both controls, the PCA solution was added at the beginning of the reaction’s development time. Using analytical software (ChemStation; Agilent Technologies), the peak areas were recorded and the quantity of acetyl-CoA was calculated using previously completed standard curves of acetyl-CoA and malonyl-CoA; hence, measuring either the disappearance of the substrate (acetyl-CoA) or the formation of the product (malonyl-CoA). Specific activity of ACCase could not be calculated because of the large quantity of unrelated proteins produced mainly by the bacterium during co-cultivation; a factor that masked all values. Therefore, activity was defined as nmoles of substrate transformed per min per one mL of sample (beads).
Determination of chlorophyll
To determine the quantity of chlorophyll a, extraction was done according to Sartory and Grobbelaar (1984) with small modifications. Quantification used the equation of Porra et al. (1989): Chl a = 16.29 (A665) – 8.54 (A652). Briefly, 10 mL 100 % methanol was added to 5 mL of freshly thawed beads and heated for 10 min at 70 °C. After cooling, the samples were incubated in the dark for 24 h at 4 °C. Then, the samples were centrifuged for 10 min (4 °C; 6,000 g) and absorbance was recorded in the supernatants at 665 and 652 nm.
Experimental design and statistical analysis
Eight individual experiments were done using a factorial design. Three variants were used: (1) Azospirillum alone, (2) Chlorella alone, and (3) co-immobilisation of Chlorella and Azospirillum. Beads without microorganisms were not routinely used because preliminary determination showed that there was no effect on the measured parameters, total lipids, and ACCase activity. Two treatments were used: (1) ammonium starvation and (2) autotrophic or heterotrophic growth conditions. The treatments were tested with either a full supply of ammonium (90 mg NH4 + L−1 or 5 mM) or ammonium starvation (0 mg NH4 + L−1), each under autotrophic (light) or heterotrophic (dark) conditions. In each treatment, three 1-L Erlenmeyer flasks containing 0.5 L SGM were used, where each flask served as a replicate. Each experiment was repeated twice and average data of both experiments were used for statistical analysis. In all eight experiments, three analyses were done: ACCase enzymatic activity, total lipids, and chlorophyll a content. Statistical analysis was done by Student’s t test at p < 0.05 (comparisons between autotrophic and heterotrophic conditions) or one-way ANOVA and LSD post-hoc analysis at p < 0.05 (comparisons among the three treatments), using Statistica 8.0 software (StatSoft, Tulsa, OK, USA).
Results
All experiments were performed when C. vulgaris was immobilised with Azospirillum brasilense in alginate beads under ammonium starvation and autotrophic and heterotrophic conditions. An optimum supply of ammonium was used in some experiments for comparison with ammonium starvation conditions. Azospirillum and Chlorella immobilised individually are also described.
Effects on total lipids
With an optimum supply of ammonium, cultures of C. vulgaris accumulated more lipids under heterotrophic than autotrophic conditions, whether cultured alone or with A. brasilense (Fig. 1a, lowercase analysis). Co-immobilisation under either type of growth cultivation produced more lipids than immobilisation of the microalgae alone (Fig. 1a, uppercase letter analysis). When cellular lipid content was calculated per cell of microalga, the cultivation conditions, autotrophic or heterotrophic, had no effect on the accumulation of lipids (Fig. 1b, lowercase analysis). Yet, each cell in the co-immobilised treatment had significantly more lipids than in other variants (Fig. 1b, uppercase letter analysis). Specific growth rates (μ; see Materials and Methods) under autotrophic conditions without starvation were 0.087 ± 005 (microalgae immobilised alone) and 0.056 ± 0.003 (co-immobilisation)for autotrophic with starvation 0.051 ± 0.002 (immobilised alone) and −0.04 ± 0.0 (co-immobilisation); for heterotrophic conditions without starvation 0.168 ± 0.002 (immobilised alone) and 0.153 ± 0.003 (co-immobilisation); for heterotrophic combined with starvation 0.023 ± 0.004 (immobilised alone) and −0.048 ± 0.004 (co-immobilisation). Growth rate of Chlorella was calculated per 6 days of growth when day 0 is immediately before the experiment started and day 6 after taking the sample. Values calculated are per day.
Under autotrophic conditions, ammonium starvation significantly enhanced lipid accumulation in all variants (microalgae and bacteria immobilised alone or co-immobilised) compared with cultivation with an optimal supply of ammonium (compare Fig. 1a and c). Contrary to conditions with an optimal supply of ammonium, cultures of C. vulgaris accumulated more lipids under autotrophic conditions (Fig. 1c, lowercase analysis), where C. vulgaris co-immobilised with A. brasilense, and cultured under autotrophic conditions combined with ammonium starvation, produced more lipids than any other variant (i.e., individually immobilised microalga or bacterium) (Fig. 1c, uppercase letter analysis). Under heterotrophic conditions, co-immobilisation did not enhance total lipid accumulation (Fig. 1c, uppercase letter analysis). This observation held true when lipid accumulation was calculated per cell (Fig. 1d, uppercase letter analysis and lowercase analysis, separately); however, it was observed that, under heterotrophic conditions, co-immobilisation produced slightly more lipids per cell than when the microalgae were immobilised alone (Fig. 1d, uppercase letter analysis).
The effect of starvation under autotrophic and heterotrophic conditions (by a t test) on accumulation of lipids per culture and per cell is presented in Table S1, employing the raw data that was used as the source for analyses presented in Fig. 1. Under autotrophic conditions, regardless of the variant (immobilisation of microalgae and bacteria alone or combined), starvation led to more total lipids in C. vulgaris. Under heterotrophic conditions, starvation reduced the amount of accumulated lipids, with the sole exception of analysis of co-immobilisation at the cell level, where no decrease was observed.
Effect on ACCase activity
Records of activities of ACCase were different, depending on the way activity was calculated, i.e., per culture or per single cell. In cultures with an optimal supply of ammonium, immobilised cultures of C. vulgaris alone cultivated heterotrophically had higher ACCase activity than under autotrophic conditions. In co-immobilised cultures, the opposite phenomenon was recorded (Fig. 2a, lowercase analysis). While similar trends were observed when activity was calculated per cell for co-immobilisation, the effect on ACCase activity in single immobilisation disappeared (Fig. 2b, lowercase analysis). Activity of ACCase was highest under autotrophic co-immobilisation (Fig. 2a, b, uppercase letter analyses).
Under conditions of ammonium starvation, the general level of ACCase activity was lower than in non-starved cultures at the culture level (compare Fig. 2a and c), but activity was mostly higher at the cell level (compare Fig. 2b and d). The effects of ammonium starvation on ACCase activity were the same regardless of whether autotrophic or heterotrophic culture conditions were used (Fig. 2c, d, lowercase analyses). ACCase activity was however, always higher in co-immobilisation, compared to single immobilisation (Fig. 2c, d, uppercase letter analyses).
The effect of starvation under autotrophic and heterotrophic conditions (by a t-test) on ACCase activity per culture and per cell is presented in Table S2, employing the raw data that was used as the source for analyses presented in Fig. 2. Under autotrophic conditions, ammonium starvation significantly decreased ACCase activity per culture and per cell. Under heterotrophic conditions at the culture level, no effect on ACCase activity was observed. But per cell ACCase activity is higher for co-immobilised Chlorella.
Effect on chlorophyll a content
Regardless of the growth conditions or starvation regime, the content of chlorophyll a in cells of C. vulgaris was always higher in co-immobilisation (Fig. 3). The highest content was recorded for non-starved autotrophic cultures (Fig. 3a). Comparable lower levels of chlorophyll a were recorded in starved cultures (autotrophic and heterotrophic) or non-starved heterotrophic cultures.
Discussion
Among the many changes in cell components and metabolism of C. vulgaris induced by immobilisation with the microalgae growth-promoting bacterium A. brasilense (under non-limited nitrogen and autotrophic growth conditions) is an increase in total lipids (de-Bashan et al. 2002a). However, the precise mechanisms for accumulating lipids in the microalgae in the combined and singly immobilised systems are unknown. This work is built upon this initial observation and measures the effects of ammonium starvation, combined with either autotrophic or heterotrophic growth conditions, on lipid accumulation and ACCase activity and the possible link between the two. ACCase is a key enzyme in de novo synthesis and in regulating fatty acid synthesis rate (Hu et al. 2008).
From all the tested parameters, co-immobilisation and heterotrophic growth conditions were the main factors affecting accumulation of lipids in C. vulgaris. A general analysis of the data obtained from the eight experiments is presented in Table 1. Under autotrophic and heterotrophic conditions, co-immobilisation always yielded higher amounts of lipids. The main factor that enhances accumulation of lipids in Chlorella spp. under autotrophic conditions is nitrogen starvation (Xiong et al. 2010; Tang et al. 2011; Přibyl et al. 2012). Our findings regarding autotrophic growth and nitrogen starvation are in accordance with this paradigm; the highest lipid content in this study under autotrophic conditions was obtained with ammonium starvation, but only when the microalga was co-immobilised with the bacterium. An unusual event that was detected was that under heterotrophic conditions ammonium starvation reduced lipid accumulation. Cultivation under heterotrophic conditions without limitation of nitrogen, however, and with or without the presence of bacteria, accumulated more lipids than under autotrophic conditions. A similar result was reported for single species cultivation where an increase of up to 900 % in lipid content in heterotrophic cultures of Chlorella zofingiensis fed 30 g L−1 glucose was found (Liu et al. 2011). In our study, therefore, it is unlikely that accumulation of lipids in C. vulgaris primarily results from limited N. While nitrogen starvation is a universal pre-requisite for lipid over-expression in most microalgae under autotrophic conditions, this study showed that A. brasilense clearly and strongly contributes to this effect.
Under co-immobilisation conditions with A. brasilense, accumulation of lipids differs between the quantity of lipids each cell accumulates in a specific culture and the total lipid accumulation capacity of a culture. This depends mainly on the size of developing microalgal population in each culture. This was demonstrated earlier for nitrogen uptake (de-Bashan et al. 2005) and carbohydrate and starch accumulation (Choix et al. 2012a, b) with our system of co-immobilisation. This phenomenon can be explained by the growth conditions of this co-culture. de-Bashan et al. (2005) and Choix et al. (2012a, b) demonstrate that culturing conditions have a significant effect on the metabolism of Chlorella spp. Small populations can uptake large quantities of nitrogen or accumulate more carbohydrate and starch, whereas larger populations were less efficient. In this study we demonstrated that this also occurred for lipid accumulation.
As a key enzyme in fatty acid synthesis, ACCase has been studied in several plants, including maize leaves (Egli et al. 1993; Herbert et al. 1996), pea leaves (Alban et al. 1994), rice seedlings (Hayashi and Satoh 2006) , and in microalgae (Sukenik and Livne 1991; Livne and Sukenik 1992; Khozin-Goldberg and Cohen 2011). In our study, ACCase activity at the culture level was variable; however, high activity was obtained with non-starved autotrophic cultures or with co-immobilisation, sufficient ammonium, and autotrophic growth conditions. At the cellular level, the highest activity was obtained when there was co-immobilisation (3 out of 4 analyses) and the best regime, either in cultures or in cells, was autotrophic (Table 1).
Although many major efforts have been made to improve production of lipids in photosynthetic microorganisms, mainly for biofuels production (Radakovits et al. 2010; Rawat et al. 2013), nonetheless, ACCase activity has not been directly correlated to lipid production in diatoms (Roessler and Ohlrogge 1993; Dunahay et al. 1996; Sheehan et al. 1998). Yet, the association between fatty acid accumulation and ACCase activity has been demonstrated (James and Cronan 2004; Klaus et al. 2004; Sasaki and Nagano 2004; Tong and Hardwood 2006). One of the most significant findings of our study is that we did not find a correlation between total lipid content and ACCase activity regardless of the variables tested. It is worth emphasising, however, that co-immobilisation under autotrophic and heterotrophic conditions (the former with and the latter without starvation) generally increased ACCase activity. We propose three plausible explanations of why there is no direct correlation between total lipid content and ACCase activity. The first explanation might be connected to the common method we used to quantify total lipids. This method quantifies other cellular components, such as chlorophyll, carotenoid, sterol, and some vitamins whose structures are lipid in nature (Pande et al. 1963), and whose synthesis is not directly controlled by ACCase, in contrast to the case for common fatty acids. Some of these compounds are enhanced in C. vulgaris when co-immobilised with A. brasilense (de-Bashan et al. 2002a; this study). This may have the strongest effect on our results in cultures with co-immobilisation, where we showed that chlorophyll a contents were always higher compared with individual immobilisation. These side effects may distort the values of lipids attributed to the production of total lipids from fatty acids by ACCase. The second explanation, strongly supporting our results with C. vulgaris, is based on intensive studies to increase production of lipids in diatoms (Sheehan et al. 1998). These studies concluded that the plausible reason for there being no increase in lipid production, despite performing successful ACCase over-expression, is because the lipid biosynthesis pathway may be subjected to feedback inhibition. Therefore, the increased activity of ACCase is compensated for by other pathways within the cell. The third explanation might be that, although ACCase is the unique enzyme in the pathway of formation of fatty acids which leads to production of lipids, lipids in the plant cell can also be produced by other pathways such as the isoprenoid pathway (Ohlrogge and Browse 1995). Thus, an increase or decrease in ACCase activity does not necessarily translate into an increase or decrease in lipid production.
At this stage of our investigations, one needs to add a reservation regarding the separation of the activities of microalgal ACCase and bacterial ACCase, which were both present in the co-immobilisation experiments. The analyses cannot separate the contribution to enzymatic activity of the prokaryotic partner, A. brasilense, to the mix. While this contribution is small regarding accumulation of lipids, the bacterium has about the same level of enzymatic activity as microalga immobilised alone under autotrophic conditions, but far lower than in the co-immobilisation treatment.
This study confirmed two observations regarding cultivation of C. vulgaris and A. brasilense when immobilised together. First, under some conditions, the growth rate of C. vulgaris, when co-immobilised with the bacterium, is lower than when the microalga is immobilised alone (Choix et al. 2012b). This demonstrated that the effect of Azospirillum is not necessarily on cell multiplication, but rather on metabolic activity, as reported previously (de-Bashan et al. 2005; 2008a). Secondly, sodium acetate is an effective carbon source for heterotrophic studies of this interaction.
In summary, when the eukaryotic–prokaryotic model (microalga–bacterium) is used, the effect exerted by A. brasilense on C. vulgaris can be quantified as an increase in total lipids and increased ACCase activity. Heterotrophic growth conditions were favourable for production of lipids, ACCase activity, and population growth of C. vulgaris, but its enhanced activity of ACCase is not linked to enhanced accumulation of lipids.
References
Alban C, Baldet P, Douce R (1994) Localization and characterization of two structurally different forms of acetyl-CoA carboxylase in young pea leaves, of which one is sensitive to aryloxyphenoxypropionate herbicides. Biochem J 300:557–565
Bashan Y (1986) Alginate beads as synthetic inoculant carriers for the slow release of bacteria that affect plant growth. Appl Environ Microb 51:1089–1098
Bashan Y, de-Bashan LE (2010) How the plant growth-promoting bacterium Azospirillum promotes plant growth-a critical assessment. Adv Agron 108:77–136
Bashan Y, Holguin G, Lifshitz R (1993) Isolation and characterization of plant growth-promoting rhizobacteria. In: Glick B, Thompson JE (eds) Methods in plant molecular biology and biotechnology. CRC, Boca Raton, pp 331–345
Bashan Y, Hernandez JP, Leyva LA, Bacilio M (2002) Alginate microbeads as inoculant carrier for plant growth-promoting bacteria. Biol Fert Soils 35:359–368
Bashan Y, Holguin G, de-Bashan LE (2004) Azospirillum-plant relationships: physiological, molecular, agricultural, and environmental advances (1997–2003). Can J Microbiol 50:521–577
Bligh GE, Dyer JW (1959) A rapid method f total lipid extraction and purification. Can J Biochem Physiol 37:911–917
Bumbak F, Cook S, Zachleder V, Hauser S, Kovar K (2011) Best practices in heterotrophic high-cell-density microalgal processes: achievements, potential and possible limitations. Appl Microbiol Biotechnol 91:31–46
Choix FJ, de-Bashan LE, Bashan Y (2012a) Enhanced accumulation of starch and total carbohydrates in alginate-immobilized Chlorella spp. induced by Azospirillum brasilense. I. Autotrophic conditions. Enzym Microb Technol 51:294–299
Choix FJ, de-Bashan LE, Bashan Y (2012b) Enhanced accumulation of starch and total carbohydrates in alginate-immobilized Chlorella spp. induced by Azospirillum brasilense. II. Heterotrophic conditions. Enzyme Microb Technol 51:300–309
Covarrubias SA, de-Bashan LE, Moreno M, Bashan Y (2012) Alginate beads provide a beneficial physical barrier against native microorganisms in wastewater treated with immobilized bacteria and microalgae. Appl Microbiol Biotechnol 93:2669–2680
Cruz I, Bashan Y, Hernàndez-Carmona G, de-Bashan LE (2013) Biological deterioration of alginate beads containing immobilized microalgae and bacteria during tertiary wastewater treatment. Appl Microbiol Biotechnol 97:9847–9858
de-Bashan LE, Bashan Y (2008) Joint immobilization of plant growth-promoting bacteria and green microalgae in alginate beads as an experimental model for studying plant-bacterium interactions. Appl Environ Microb 74:6797–6802
de-Bashan LE, Bashan Y (2010) Immobilized microalgae for removing pollutants: review of practical aspects. Bioresource Technol 101:1611–1627
de-Bashan LE, Bashan Y, Moreno M, Lebsky VK, Bustillos JJ (2002a) Increased pigment and lipid content, lipid variety, and cell and population size of the microalgae Chlorella spp. when coimmobilized in alginate beads with the microalgae-growth-promoting bacteria Azospirillum brasilense. Can J Microbiol 48:514–521
de-Bashan LE, Moreno M, Hernandez JP, Bashan Y (2002b) Removal of ammonium and phosphorus ions from synthetic wastewater by the microalgae Chlorella vulgaris coimmobilized in alginate beads with the microalage growth-promoting bacterium Azospirillum brasilense. Water Res 36:2941–2948
de-Bashan LE, Hernandez JP, Morey T, Bashan Y (2004) Microalgae growth-promoting bacteria as helpers for microalgae: a novel approach for removing ammonium and phosphorus from municipal wastewater. Water Res 38:466–474
de-Bashan LE, Antoun H, Bashan Y (2005) Cultivation factors and population size control uptake of nitrogen by the microalgae Chlorella vulgaris when interacting with the microalgae growth-promoting bacterium Azospirillum brasilense. FEMS Microbiol Ecol 54:197–203
de-Bashan LE, Magallon P, Antoun H, Bashan Y (2008a) Role of glutamate dehydrogenase and glutamine synthetase in Chlorella vulgaris during assimilation of ammonium when jointly immobilized with the microalgae-growth-promoting bacterium Azospirillum brasilense. J Phycol 44:1188–1196
de-Bashan LE, Trejo A, Huss VAR, Hernandez JP, Bashan Y (2008b) Chlorella sorokiniana UTEX 2805, a heat and intense, sunlight-tolerant microalgae with potential for removing ammonium from wastewater. Bioresource Technol 99:4980–4989
de-Bashan LE, Schmid M, Rothballer M, Hartmann A, Bashan Y (2011) Cell-cell interaction in the eukaryote-prokaryote model using the microalgae Chlorella vulgaris and the bacterium Azospirillum brasilense immobilized in polymer beads. J Phycol 47:1350–1359
Dunahay TG, Jarvis EE, Dais SS, Roessler PG (1996) Manipulation of microalgal lipid production using genetic engineering. Appl Biochem Biotechnol 57(58):223–231
Egli MA, Gengenbach BG, Gronwald JW, Somers DA, Wyse DL (1993) Characterization of maize acetyl-Coenzyme A carboxylase. Plant Physiol 101:499–506
Francki M, Whitaker P, Smith P, Atkins C (2002) Differential expression of a novel gene during seed triacylglycerol accumulation in lupin species (Lupinus angustifolius L. and L. mutabilis L.). Funct Integr Genom 2:292–300
Gonzalez LE, Bashan Y (2000) Growth promotion of the microalga Chlorella vulgaris when coimmobilized and cocultured in alginate beads with the plant-growth-promoting bacterium Azospirillum brasilense. Appl Environ Microb 66:1527–31
Gonzalez LE, Cañizares RO, Baena S (1997) Efficiency of ammonia and phosphorus removal from a Colombian agroindustrial wastewater by the microalgae Chlorella vulgaris and Scenedesmus dimorphus. Bioresource Technol 60:259–262
Gouveia L, Oliveira AC (2009) Microalgae as raw material for biofuels production. J Ind Microbiol Biot 36:269–274
Hayashi O, Satoh K (2006) Determination of acetyl-CoA and Malonyl-CoA in germinating rice seeds using the LC-MS/MS Technique. Biosci Biotech Biochem 70:2676–2681
Herbert D, Price L, Alban C, Dehaye L, Job D, Cole D, Pallet K, Hardwood J (1996) Kinetic studies on two isoforms of acetyl-CoA carboxylase from maize leaves. Biochem J 318:997–1006
Hernandez JP, de-Bashan LE, Bashan Y (2006) Starvation enhances phosphorus removal from wastewater by the microalga Chlorella spp. co-immobilized with Azospirillum brasilense. Enzyme Microb Tech 38:190–198
Hu Q, Sommerfeld M, Jarvis E, Ghirardi M, Posewitz M, Seibert M, Darzins A (2008) Microalgal triacylglycerols as feedstocks for biofuels production: perspectives and advances. Plant J 54:621–639
James ES, Cronan JE (2004) Expression of two Escherichia coli acetyl-CoA carboxylase subunits is autoregulated. J Biol Chem 279:2520–2527
Khozin-Goldberg I, Cohen Z (2011) Unraveling algal lipid metabolism: recent advances in gene identification. Biochimie 93:91–100
Klaus D, Ohlrogge J, Ekkerhard Neuhaus H, Dörmann P (2004) Increased fatty acid production in potato by engineering of Acetyl-CoA carboxylase. Planta 219:389–396
Lebeau T, Robert JM (2006) Biotechnology of immobilized micro algae: a culture technique for the future? In: Rao S (ed) Algal cultures, analogues of blooms and applications. Science Publishers, Enfield, pp 801–837
Levert KL, Waldrop GL, Stephens JM (2002) A biotin analogue inhibits acetyl CoA carboxylase activity and adipogenesis. J Biol Chem 277:16347–16350
Liu W, Harrison DK, Chalupska D, Gornicki P, O’Donnell C, Adkins S, Haselkorn R, Williams R (2007) Single-site mutations in the carboxyltransferase domain of plastid acetyl-CoA carboxylase confer resistance to grass-specific herbicides. Proc Natl Acad Sci USA 104:3627–3632
Liu J, Huang J, Sun Z, Zhong Y, Jiang Y, Chen F (2011) Differential lipid and fatty acid profiles of photoautotrophic and heterotrophic Chlorella zofingiensis: assessment of algal oils for biodiesel production. Bioresource Technol 102:106–110
Livne A, Sukenik A (1992) Lipid synthesis and abundance of acetyl-CoA carboxylase in Isochrysis galbana (Prymnesiophyceae) following nitrogen starvation. Plant Cell Physiol 33:1175–1181
Mata TM, Martins AA, Caetano NS (2010) Microalgae for biodiesel production and other applications: a review. Renew Sust Energ Rev 14:217–232
O’Grady J, Morgan A (2011) Heterotrophic growth and lipid production of Chlorella protothecoides on glycerol. Bioprocess Eng 34:121–125
Oh-Hama T, Miyachi S (1992) Chlorella. In: Borowitzka MA, Borowitzka LJ (eds) Micro-algae biotechnology. Cambridge University Press, Cambridge, pp 3–26
Ohlrogge J, Browse J (1995) Lipid biosynthesis. Plant Cell 7:957–970
Pande SV, Parvin RK, Venkitasubramanian TA (1963) Microdetermination of lipids and serum total fatty acids. Anal Biochem 6:415–423
Perez-Garcia O, de-Bashan LE, Hernandez JP, Bashan Y (2010) Efficiency of growth and nutrient uptake from wastewater by heterotrophic, autotrophic, and mixotrophic cultivation of Chlorella vulgaris immobilized with Azospirillum brasilense. J Phycol 46:800–812
Perez-Garcia O, Bashan Y, Puente ME (2011) Organic carbon supplementation of sterilized municipal wastewater is essential for heterotrophic growth and removing ammonium by the microalga Chlorella vulgaris. J Phycol 47:190–199
Porra RJ, Thomson WA, Kriedemann PA (1989) Determination of accurate extinction coefficients and simultaneous equations for assaying chlorophylls a and b extracted with four different solvents: verification of the concentrations of chlorophyll standards by atomic absorption spectroscopy. Biochim Biophys Acta 975:384–394
Prasad K, Kadokawa JI (2009) Alginate-based blends and nano/microbeads. Microbiol Monogr 13:175–210
Přibyl P, Cepák V, Zachleder V (2012) Production of lipids in 10 strains of Chlorella and Parachlorella, and enhanced lipid productivity in Chlorella vulgaris. Appl Microbiol Biotechnol 94:549–561
Radakovits R, Jinkerson RE, Darzins A, Pasewitz C (2010) Genetic engineering of algae for enhanced biofuel production. Eukaryot Cell 9:486–501
Rawat I, Ranjith Kumar R, Mutanda T, Bux F (2013) Biodiesel from microalgae: a critical evaluation from laboratory to large scale production. Appl Energ 103:444–467
Roessler PG, Ohlrogge JB (1993) Cloning and characterization of the gene that encodes acetyl-coenzyme A carboxylase in the alga Cyclotella cryptica. J Biol Chem 268:19254–19259
Sartory D, Grobbelaar J (1984) Extraction of chlorophyll a from freshwater phytoplankton for spectrophotometric analysis. Hydrobiologia 114:177–187
Sasaki Y, Nagano Y (2004) Plant acetyl-CoA carboxylase: structure, biosynthesis, regulation and gene manipulation for plant breeding. Biosci Biotechnol Biochem 68:1175–1184
Sato N, Moriyama T (2007) Genomic and biochemical analysis of lipid biosynthesis in the unicellular rhodophyte Cyanidioschyzon merolae: lack of plastidic desaturation pathway results in the coupled pathway of galactolipid synthesis. Eukariot Cell 6:1006–1017
Sheehan J, Dunahay T, Benemann J, Roessler PG (1998) US Department of Energy’s Office of Fuels Development. A look back at the US Department of Energy’s aquatic species program – biodiesel from algae, close Out Report TP-580-24190. National Renewable Energy Laboratory, Golden
Sukenik A, Livne A (1991) Variations in lipid and fatty acid content in relation to acetyl CoA carboxylase in the marine Prymnesiophyte Isochrysis galbana. Plant Cell Physiol 32:371–378
Tang H, Chen M, Garcia MED, Abunasser N, Simon Ng KY, Salley SO (2011) Culture of microalgae Chlorella minutissima for biodiesel feedstock production. Biotechnol Bioeng 108:2280–2287
Tong L, Hardwood HJ (2006) Acetyl-coenzyme A carboxylases: versatile targets for drug discovery. J Cell Biochem 99:1476–1488
Wan M, Wang R, Xia J, Rosenberg J, Nie Z, Kobayashi N, Oyler G, Betenbaugh M (2012) Physiological evaluation of a new Chlorella sorokiniana isolate for its biomass production and lipid accumulation in photoautotrophic and heterotrophic cultures. Biotechnol Bioeng 109:1958–1964
Xiong W, Gao CF, Yan D, Wu C, Wu QY (2010) Double CO2 fixation in photosynthesis–fermentation model enhances algal lipid synthesis for biodiesel production. Bioresource Technol 101:2287–2293
Yu Q, Collavo A, Zheng M, Owen M, Sattin M, Powles S (2007) Diversity of acetyl-Coenzyme A carboxylase mutations in resistant Lolium populations: evaluation using clethodim. Plant Physiol 145:547–558
Acknowledgments
At CIBNOR, we thank Manuel Moreno for technical support, Ira Fogel for editorial improvements, Fernando Garcia-Carreño for free use of the HPLC, and Mariana Diaz- Tenorio of Instituto Tecnologico de Sonora, Cd. Obregon, Mexico, for help in enzymatic analysis. This study was supported by the Secretaria de Medio Ambiente y Recursos Naturales, (SEMARNAT contract 23510) and Consejo Nacional de Ciencia y Tecnologia of Mexico (CONACYT-Basic Science-2009, contracts 130656 and 164548). Time for writing was provided by The Bashan Foundation, USA. L.A.L. was mainly supported by a graduate fellowship (CONACYT #48487) and additional periodic grants from The Bashan Foundation.
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This study is dedicated to the memory of the Italian microbiologist Prof. Franco Favilli (1933–2012) of the University of Florence, Italy, one of the pioneers of Azospirillum studies
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Leyva, L.A., Bashan, Y. & de-Bashan, L.E. Activity of acetyl-CoA carboxylase is not directly linked to accumulation of lipids when Chlorella vulgaris is co-immobilised with Azospirillum brasilense in alginate under autotrophic and heterotrophic conditions. Ann Microbiol 65, 339–349 (2015). https://doi.org/10.1007/s13213-014-0866-3
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DOI: https://doi.org/10.1007/s13213-014-0866-3