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Oxidative Stress Is a Mediator for Increased Lipid Accumulation in a Newly Isolated Dunaliella salina Strain

  • Kaan Yilancioglu,

    Affiliation Faculty of Engineering and Natural Sciences, Sabanci University, Orhanlı, Istanbul, Turkey

  • Murat Cokol,

    Affiliations Faculty of Engineering and Natural Sciences, Sabanci University, Orhanlı, Istanbul, Turkey, Sabanci University Nanotechnology Research and Application Center, Orhanlı, Istanbul, Turkey

  • Inanc Pastirmaci,

    Affiliation Faculty of Engineering and Natural Sciences, Sabanci University, Orhanlı, Istanbul, Turkey

  • Batu Erman,

    Affiliation Faculty of Engineering and Natural Sciences, Sabanci University, Orhanlı, Istanbul, Turkey

  • Selim Cetiner

    cetiner@sabanciuniv.edu

    Affiliation Faculty of Engineering and Natural Sciences, Sabanci University, Orhanlı, Istanbul, Turkey

Oxidative Stress Is a Mediator for Increased Lipid Accumulation in a Newly Isolated Dunaliella salina Strain

  • Kaan Yilancioglu, 
  • Murat Cokol, 
  • Inanc Pastirmaci, 
  • Batu Erman, 
  • Selim Cetiner
PLOS
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Abstract

Green algae offer sustainable, clean and eco-friendly energy resource. However, production efficiency needs to be improved. Increasing cellular lipid levels by nitrogen depletion is one of the most studied strategies. Despite this, the underlying physiological and biochemical mechanisms of this response have not been well defined. Algae species adapted to hypersaline conditions can be cultivated in salty waters which are not useful for agriculture or consumption. Due to their inherent extreme cultivation conditions, use of hypersaline algae species is better suited for avoiding culture contamination issues. In this study, we identified a new halophilic Dunaliella salina strain by using 18S ribosomal RNA gene sequencing. We found that growth and biomass productivities of this strain were directly related to nitrogen levels, as the highest biomass concentration under 0.05 mM or 5 mM nitrogen regimes were 495 mg/l and 1409 mg/l, respectively. We also confirmed that nitrogen limitation increased cellular lipid content up to 35% under 0.05 mM nitrogen concentration. In order to gain insight into the mechanisms of this phenomenon, we applied fluorometric, flow cytometric and spectrophotometric methods to measure oxidative stress and enzymatic defence mechanisms. Under nitrogen depleted cultivation conditions, we observed increased lipid peroxidation by measuring an important oxidative stress marker, malondialdehyde and enhanced activation of catalase, ascorbate peroxidase and superoxide dismutase antioxidant enzymes. These observations indicated that oxidative stress is accompanied by increased lipid content in the green alga. In addition, we also showed that at optimum cultivation conditions, inducing oxidative stress by application of exogenous H2O2 leads to increased cellular lipid content up to 44% when compared with non-treated control groups. Our results support that oxidative stress and lipid overproduction are linked. Importantly, these results also suggest that oxidative stress mediates lipid accumulation. Understanding such relationships may provide guidance for efficient production of algal biodiesels.

Introduction

The idea of using biofuels has gained prominence, since they provide a cleaner alternative to the currently used fossil fuels. It has recently been estimated that utilization of biofuels will result in a 30% decrease in CO2 emissions in the United States. Biofuels can be derived from different kinds of resources including microalgae, animal fats, soybeans, corns and other oil crops. While none of these options currently has the efficiency to produce the required amounts of biofuel [1], microalgae are considered the most promising venue of biofuel production due to their ease of cultivation, sustainability, and compliance in altering their lipid content resulting in higher biofuel production.

High lipid accumulation and biomass productivity are the two manifestly desired phenotypes in algae for biodiesel production. However, various studies conducted under nutrient depleted conditions have demonstrated that biomass productivity and lipid accumulation are negatively related [2]. These studies have established that stress conditions, which by definition reduce the biomass production, increase lipid content of algae. This problem was addressed by using a two-stage reactor where algal species such as Oocysti sp. and amphora sp. are grown in optimal conditions for maximum biomass, followed by stress conditions for maximum lipid accumulation [3]. Within this context, nitrogen depletion can be still considered as a strategy for increasing lipid accumulation since it has been still defined as one of the best lipid accumulator stress condition in algae to date. However the mechanistic insights of this phenomenon are still needed.

Nitrogen deprivation as a stress condition is known to maximize the lipid content up to 90% [4]. However, underlying mechanisms have not been well described in terms of its physiological and molecular aspects. Despite the fact that oxygen itself is not harmful for cells, the presence of reactive oxygen species (ROS) may lead to oxidative damage to the cellular environment, ultimately leading to toxicity resulting from excessive reactive oxygen stress [5]. Redox reactions of the reactive forms of oxygen including hydrogen peroxide (H2O2), superoxide (O2) or hydroxyl (OH) radicals with cellular lipids, proteins, and DNA result in oxidative stress [6]. A previous study showed that nitrogen depletion results in the co-occurrence of ROS species and lipid accumulation in diatoms [7]. Association of increased reactive oxygen species levels and cellular lipid accumulation under different environmental stress conditions was also shown in green microalgae [8] ROS is known to be an important factor in cellular response and it is well established that ROS increases when microalgae are exposed to various stresses. However, a mechanistic understanding of the connection between ROS increase and increased lipid accumulation in algae species requires further investigation [9].

Nitrogen depleted conditions trigger reactive oxygen species accumulation, increased cellular lipid content and protein production impairment. However, the temporal order and the causal links between these events are yet to be explored. Here, we aimed at finding the relationship between oxidative stress and increased cellular lipid content under nitrogen depleted conditions in a hypersaline green alga in order to have a better understanding of this phenomenon.

Dunaliella genus [10] is one of the microalgae genus that has been considered for lipid production. Dunaliella species are particularly attractive due to their strong resistance characteristics to various unfavourable environmental conditions such as high salinity. Obtaining such strong algal species for lipid production under conditions that are otherwise not useful is an important economical consideration in terms of biodiesel production. In addition, cultivation of algae species in freshwaters may not be feasible due to the limited supply and population expansion. Understanding the mechanisms behind increased lipid accumulation in halophilic Dunaliella in response to different stress conditions, especially nitrogen depletion, is crucial to enable key manipulations at the genetic, biochemical and physiological level for decreasing biodiesel production costs.

Materials and Methods

Organism and Culture Conditions

Dunaliella tertiolecta (D.t. #LB999) and Chlamydomonas reinhardtii (C.r. #90) were obtained from UTEX, Collection Culture of Algae, USA and cultivated artificial sea water medium and soil extract medium as instructed by the culture collection protocols respectively. The alga used in this study was isolated from the hypersaline lake “Tuz”, which is located in Middle Anatolia, Turkey with the research permission of Republic of Turkey Ministry of Food, Agriculture and Livestock (Permit issue: B.12.0.TAG.404.03.10.03.03–1607). Field studies did not involve endangered or protected species. Collection of water samples was done and isolation location was recorded using a GPS device as 39°4′23.97″K - 33°24′33.11″E at the southern east part of Sereflikochisar province. 10 ml water samples were collected and enriched with the same volume of Bold’s Basal Medium (BBM) modified by addition of 5% NaCl. BBM was pH 7.4 and consisted of 5 mM NaNO3 along with CaCl2·2H2O 0.17 mM, MgSO4·7H2O 0.3 mM, K2HPO4 0.43 mM, KH2PO4 1.29 mM, Na2EDTA·2H2O 2 mM, FeCl3·6H2O 0.36 mM, MnCl2·4H2O 0.21 mM, ZnCl2 0.037 mM, CoCl2·6H2O 0.0084 mM, Na2MoO4·2H2O 0.017 mM, Vitamin B12 0.1 mM and 5 mM NaCO3 was supplied as carbon source.

Water samples were plated on petri dishes with modified BBM 5% NaCl and 1% bacteriological agar, while same water samples were also subjected to dilutions with fresh modified BBM 5% NaCl in 48-well plates (1∶2, 1∶4, 1∶8, 1∶16, 1∶32, 1∶64) to obtain monocultures. After 2 and 4 weeks cultivation periods of 48-well plate liquid cultures and petri dishes, respectively, clones were isolated. These clones were transferred to fresh mediums in 100 ml canonical flasks in a final volume of 25 ml for obtaining cell stocks at 25°C under continuous shaking and photon irradiance of 80 rpm and 150 μEm−2s−1.

All experiments were carried out under same cultivation conditions in 250 ml batch cultures but different nitrogen concentrations, 0.05, 0.5 and 5 mM NaNO3 were used for low, medium and high nitrogen concentrations, respectively. Concentrations ranging between 200 uM and 8 mM were used for H2O2 experiments.

Isolation and Purification of DNA and Amplification of 18S rRNA Encoding Gene

DNA isolation was done by using DNeasy Plant Mini Kit (Qiagen) as instructed by the manufacturer. Quantification of the genomic DNA obtained and assessment of its purity was done on a Nanodrop Spectrophotometer ND-1000 (Thermo Scientific) and on 1% agarose gel elecrophoresis. MA1 [5′-CGGGATCCGTAGTCATATGCTTGTCTC-3′] and MA2 [5-GGAATTCCTTCTGCAGGTTCACC-3′] were designed from 18S rDNA genes and were previously reported by Olmos et al [11]. PCR reactions were carried out in a total volume of 50 μl containing 50 ng of chromosomal DNA in dH2O and 200 ng MA1 and MA2 conserved primers. The amplification was carried out using 30 cycles in a MJ Mini Personal Thermal Cycler (BioRad), with a Tm of 52°C for all reactions. One cycle consisted of 1 minute at 95°C, 1 minute at 52°C and 2 minutes at 72°C.

Sequencing and Phylogenetic Analysis

MA1–MA2 PCR products were utilized to carry out sequencing reactions after purification with a QIAquick PCR purification kit (Qiagen). The sequencing reactions were run by MCLAB (San Francisco, CA), employing primers MA1–MA2 in both reverse and forward directions. DNA sequences were imported to BLAST for identification and to search for phylogenetic relationship correlations between other 18S rDNA gene sequences of Dunaliella species/strains deposited in NCBI Gene Bank. Dendrogram data generated by BLAST was converted into newick format and submitted to Phyfi [12] for generating phylogenetic tree.

Growth Analysis

Specific growth rate and biomass productivity was calculated according to the equation; where and , biomass at time1 and time2 respectively [13]. Divisions per day and the generation (doubling) time were calculated according to the equations below:

Extraction and Measurements of Lipid Contents and Fluorescence Microscopy

Lipid was extracted according to Bligh and Dyer wet extraction method. Briefly, to a 15 ml glass vial containing 100 mg dried algal biomass, 2 ml methanol and 1 ml chloroform were added and kept for 24 h at 25°C. The mixture was then vortexed and sonicated for 10 minutes. One milliliter of chloroform was again added, and the mixture shaken vigorously for 1 min. Subsequently, 1.8 ml of distilled water was added and the mixture vortexed again for 2 min. The aqueous and organic phases were separated by centrifugation for 15 min at 2,000 rpm. The lower (organic) phase was transferred into a previously weighed clean vial (V1). Evaporation occurred in a thermo-block at 95°C, and the residue was further dried at 104°C for 30 min. The weight of the vial was again recorded (V2). Lipid content was calculated by subtracting V1 from V2, and expressed as dcw %. The correspondence between Nile Red fluorescence intensity and % lipid content was determined by plotting relative fluorescence units against % cellular lipid content obtained from triplicate samples. For fluorescence microscopy analysis of Nile Red, cells were stained with 5 μl 0.5 mg/mL Nile Red (Sigma, USA) stock solution after fixing cells with 5% paraformaldehyde and imaged by epi-fluorescence microscopy with a Leica DMR microscope (Leica Microsystems).

Spectrofluorometric Microplate Analysis for Determination of Lipid and Reactive Oxygen Species Accumulation

Nile red, 9-diethylamino-5H-benzo[alpha]phenoxazine-5-one was first reported that is an excellent vital stain for the detection of intracellular lipid droplets by fluorescence microscopy and flow cytoflourometry [14] and it has been widely used for measuring and comparing cellular lipid content in various organisms in numerous studies [15][19]. A stock solution of Nile Red (NR) (Sigma, 72485) was prepared by adding 5 mg of NR to 10 ml of acetone. The solution was kept in a dark colored bottle and stored in the dark at −20°C. 1 ml of algal cells from a culture of 250 ml glass erlenmeyer flasks containing 100 ml growth media with different nitrogen concentrations were transferred to 1.5 ml eppendorf tubes for 5 min centrifugation at 5,000 rpm, washed twice with fresh medium, and measured in a spectrophotometer at 600 nm. Each sample was adjusted to an OD600 of 0.3 in a 1 ml final volume by dilution with fresh medium. 5 μl of Nile Red solution was added to each tube and mixed well, followed by 20 min incubation in the dark. Finally, cellular neutral lipids were quantified using a 96-well microplate spectrofluorometry (SpectraMAX GEMINI XS) with an excitation wavelength of 485 nm and an emission wavelength of 612 nm.

Dichloro-dihydro-fluorescein diacetate (DCFH-DA) is the most widely used fluorometric probe for detecting intracellular oxidative stress. This probe is cell-permeable and is hydrolyzed intracellularly to the DCFH carboxylate anion. Two-electron oxidation of DCFH results in the formation of a dichlorofluorescein (DCF) as a fluorescent product. The amount of this fluorescent product is highly correlated with the cellular oxidation/oxidative stress level. Investigators have routinely used DCFH-DA to measure intracellular generation of reactive oxidants in cells in response to intra- or extracellular activation with oxidative stimulus [20]. Determination of ROS production related to oxidative stress was done by using DCFH-DA (Sigma, USA). Vital staining for determination of cell survival under H2O2 treatment was done by using fluorescein diacetate (FDA) (Sigma, USA). FDA is incorporated into live cells and it is converted into fluorescein by cellular hydrolysis [21]. 0.5 mg/ml stock solutions for both stains were prepared in acetone and the same protocol was used for FDA (Sigma, USA) and DCFH-DA (Sigma, USA) staining as described above for Nile Red staining. Data were recorded as relative fluorescence units [22] for all spectrofluorometric staining experiments.

Flow Cytometric Analysis for Determination of Lipid and Reactive Oxygen Species Accumulation

5 μl of Nile Red (Sigma, USA) from stock solution (0.5 mg/mL) was added to 1 ml of a cell suspension at an OD600 of 0.3 after washing cells twice with fresh medium. This mixture was gently vortexed and incubated for 20 minutes at room temperature in dark. Nile Red uptake was determined using a BD-FACS Canto flow cytometer (Becton Dickinson Instruments) equipped with a 488 nm argon laser. Upon excitation by a 488 nm argon laser, NR exhibits intense yellow-gold fluorescence when dissolved in neutral lipids. The optical system used in the FACS Canto collects yellow and orange light (560–640 nm, corresponding to neutral lipids). Approximately 10,000 cells were analysed using a log amplification of the fluorescent signal. Non-stained cells were used as an autofluorescence control. Nile Red fluorescence was measured using a 488 nm laser and a 556 LP+585/42 band pass filter set on a FACS Canto Flow Cytometer. Data were recorded as mean fluorescence intensity (MFI).

DCFH-DA (Sigma, USA) from stock solution (0.5 mg/ml) was used as described above for flow-cytometric microplate Nile Red staining method in order to analyze cellular oxidative stress status. Briefly, 1 ml of algal cells in different nitrogen concentrations were transferred into 1.5 ml eppendorf tubes, centrifuged 5 min at 5,000 rpm, washed twice with fresh medium, and measured in a spectrophotometer at 600 nm. Each sample was adjusted to an OD600 of 0.3 in a 1 ml final volume by dilution with fresh medium. 5 μl of dye solution was added to each tube and mixed well, followed by 20 min incubation in the dark and analyzed. Nonfluorescent DCFH-DA is taken up and converted into diclorodihydrofluorescein (DCF) by the action of cellular esterases. Fluorescence from oxidized DCF was measured using a 488 nm laser and a 556/Long Pass filter set on a BD-FACS Canto Flow Cytometer. Data were expressed as mean fluorescence intensity (MFI). The data of both staining methods were evaluated using Flowjo Ver. 7.6.1 (Tree Star, Inc.).

Protein, Chlorophyll, Carotenoid, TBARS Analyses and Enzymatic Assays

Total protein isolation was done according to Barbarino et al. [23]. Protein content was determined following the method described by Bradford [24]. Cellular chlorophyll and carotenoid isolations were done using the methanol extraction method. Calculation of chlorophyll and carotenoid contents were carried out using the formula for methanol extraction described by Wellburn [25]. Lipid peroxidation analysis upon different nitrogen concentration regimes was analysed by using thiobarbituric acid reactive substances (TBARS) method described by Sabatini et al [26]. For superoxide dismutase (SOD) analysis 50 mg biomass was homogenized in 2 ml 0.5 M phosphate buffer (pH 7.5) and centrifuged at 13,000 rpm for 10 min at 4°C. SOD activity was determined in the supernatant by inhibition of nitroblue tetrazolium (NBT) using a reaction mixture of 1.5 ml Na2CO3 (1 M), 200 μl methionine (200 mM), 100 μl NBT (2.25 mM), 100 μl EDTA (3 mM), 100 μl riboflavin (60 ?M) and 1.5 ml phosphate buffer (pH 7.8, 0.1 M). The absorbance was recorded at 560 nm. One unit of SOD per gram of protein was defined as the amount causing 50% inhibition of photochemical reduction of NBT [27]. For catalase (CAT) analysis, 50 mg biomass was homogenized in 2 ml phosphate buffer (0.5 M, pH 7.5), centrifuged at 12,000 rpm at 4°C for 30 min and supernatant was taken for CAT activity. A reaction mixture containing 1.6 ml phosphate buffer (pH 7.3), 100 μl EDTA (3 mM), 200 μl H2O2 (0.3%) and 100 μl supernatant (containing enzyme extract) was taken in a cuvette and CAT activity in supernatant was determined by monitoring the disappearance of H2O2, by measuring a decrease in absorbance at 240 nm against a blank of same reaction mixture without 0.3% H2O2 [28]. For analysis of ascorbate peroxidase (APX), 50 mg biomass was homogenized in 2 ml phosphate buffer (0.5 M, pH 7.5) and centrifuged at 12,000 rpm at 4°C for 30 min. The supernatant was taken for APX activity. A reaction mixture containing 1 ml phosphate buffer (pH 7.3), 100 μl EDTA (3 mM), 1 ml ascorbate (5 mM), 200 μl H2O2 (0.3%) and 100 μl supernatant (containing enzyme extract) was prepared in a cuvette. The reaction was followed for 3 min at a wavelength of 290 nm against a blank of same reaction mixture without 0.3% H2O2 [29].

Results and Discussion

Isolation and Identification of the New Dunaliella salina Strain

We isolated a new hypersaline microalga from the biggest salt lake of Turkey located in the Middle Anatolian region in July 2011. The microalga, which is unicellular, biflagellate and tolerant up to 20% NaCl was identified as Dunaliella salina based on the morphological characterization prior to molecular identification. We observed that cell color was green under normal conditions and the color changed to red under stress conditions. Morphologically, ovoid, spherical and cylindrical cell shapes were observed. Stigma was not clearly visible or diffuse. Large pyrenoid with distict amylosphere was observed and refractile granules are absent. Cellular size was measured as ∼20 μm. These observed characteristics were consistent with previous morphological characteristics of Dunaliella salina.

This strain was deposited in −196°C ultra freeze conditions at Sabanci University algae culture collection as Dunaliella salina strain Tuz_KS_01. Molecular identification was based on 18S rDNA gene sequence amplification and sequencing. A single 18S rDNA PCR amplicon was about ∼1800 bp in size, in accordance with Olmos et al. [11]. The partial sequence of the 18S rDNA encoding gene was submitted to National Center for Biotechnology Information (NCBI) GeneBank database as Dunaliella salina strain Tuz_KS_01 (GeneBank accession no. JX880083). According to Basic Local Aligment Search Tool (BLAST) analysis, the isolated sequence had very high percentage of identity with other deposited 18S rDNA sequences of Dunaliella species shown in the phylogenetic tree plotted in Figure 1. Molecular identification showed a high percentage identity to Dunaliella salina strains (Identity 93%, Query Coverage 70%).

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Figure 1. Phylogenetic analysis of Dunaliella salina strain Tuz_KS_01 (GeneBank accession no. JX880083).

Dendrogram was generated using the neighbor-joining analysis based on 18S rDNA gene sequences. The phylogenetic tree shows the position of Dunaliella salina strain Tuz_KS_01 (GeneBank accession no. JX880083) relative to other species and strains of Dunaliella deposited in NCBI GeneBank.

https://doi.org/10.1371/journal.pone.0091957.g001

Growth Analysis of the New Dunaliella Strain Under Different Nitrogen Concentrations

The newly isolated halotolerant Dunaliella salina strain was cultivated under different nitrogen concentrations for growth analysis. 0.05 mM, 0.5 mM and 5 mM NaNO3 concentrations were considered as low, medium and high nitrogen concentrations. Specific growth rates and/or average biomass productivities (ABP) were found to be 370 mg/dayL, 430 mg/dayL, 520 mg/dayL for low, medium and high nitrogen groups respectively. The highest biomass concentration under low nitrogen regimes was 495 mg/l, compared with 994 mg/l and 1409 mg/l for medium and high nitrogen regimes shown in Figure 2. Other kinetic growth data including doubling time/generation time and division per day were also calculated. Doubling times were calculated as 1.84, 1.59, and 1.32 whereas division of cells per day was calculated as 0.54, 0.62, and 0.75 for low, medium and high nitrogen concentration groups respectively.

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Figure 2. Effects of different nitrogen concentrations on the growth and biomass productivity of Dunaliella salina strain Tuz_KS_01 (GeneBank accession no. JX880083).

0.053 are referred as low, medium and high nitrogen concentrations respectively. Shown OD600 optical density and biomass values are the means of three replicates. The error bars correspond to ±1 SD of triplicate optical density measurements.

https://doi.org/10.1371/journal.pone.0091957.g002

Biomass productivity is one of the most important parameters for the feasibility of utilizing algal oil for biodiesel production. Hence, numerous studies have been conducted in various algal species. Tang et al. (2011) demonstrated that Dunaliella tertiolecta had a highest biomass concentration of ∼400 mg/l [30]. In another study conducted by Ho et al. (2010) the optimal biomass productivity of freshwater alga Scenedesmus obliquus were found to be 292.50 mg/dayL [31]. Griffiths et al. (2012) studied 11 different algal species including freshwater, marine and halotolerant species and demonstrated their biomass productivities [32]. Compared to the reported biomass productivities in previous studies, both the highest biomass concentration and average biomass productivity of isolated Dunaliella salina strain Tuz_KS_01 showed very good potential, eventhough small batch cultivation process was utilized instead of using more sophisticated and efficient cultivation systems.

Lipid Accumulation Analysis of the New Dunaliella salina Strain Under Different Nitrogen Concentrations

Experimental groups were subjected to flow cytometric Nile red analysis for measuring lipid accumulation at single cell level in stationary growth phase. Cell populations were chosen according to cellular size and granulation as quantified by forward and side scatter values of populations, respectively which is demonstrated in Figure 3A. Figure 3B shows a representative flow cytometric analysis of lipid contents under different nitrogen concentrations, indicating high lipid content under low nitrogen condition. Figure 3C shows the mean and standard error for three biological replicates, clearly exhibiting a negative relationship between lipid accumulation and nitrogen levels. Therefore, cultivation under low nitrogen conditions stimulates lipid accumulation in Dunaliella salina strain Tuz_KS_01, in agreement with previous studies [33], [34].

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Figure 3. Lipid content analysis of Dunaliella salina strain Tuz_KS_01 under different nitrogen conditions.

A) Zebra-plot of SSC (Side Scatter) and FSC (Forward Scatter) expressing cellular granulation and cellular size, respectively, under a representative nitrogen depletion condition (0.05 mM). B) A representative histogram of flow-cytometric analysis of lipid contents under different nitrogen concentrations C) Mean fluorescent intensities (MFI) of flow cytometric analysis. D) Fluorometric microplate Nile Red analysis of early logarithmic, late logarithmic and stationary growth phases. Data represent the mean values of triplicates. Standard error for each triplicate is shown as tilted lines for clarity, where the minimum and maximum y values of each line corresponds to ±1 SE.

https://doi.org/10.1371/journal.pone.0091957.g003

In addition, we measured lipid accumulation of the green alga under different nitrogen levels using spectrofluorophotometer [35] at early-logarithmic, late-logarithmic and stationary growth phases. While the cellular lipid accumulation in early and late logarithmic phases did not show a drastic change, we observed a marked increase of lipid content in the stationary phase, which was significantly higher under low nitrogen cultivation conditions shown in Figure 3D.

Nitrogen depletion is well known to result in increased lipid accumulation in algal species [36], eventhough its association with other related factors has not been well defined. To demonstrate the oxidative stress under nitrogen limited cultivation conditions, fluorometric DCFH-DA and related TBARS lipid peroxidation assays were utilized. According to these results, increased ROS production (Figure 4A) and lipid peroxidation (Figure 4B) were both observed under nitrogen limited conditions, in association with increased lipid accumulation especially at stationary phase shown in Figure 4C.

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Figure 4. Oxidative stress and lipid accumulation under different nitrogen concentrations.

A) Fluorometric microplate DCFH-DA analysis under different nitrogen concentrations. B) TBARS analysis for lipid peroxidation under different nitrogen concentrations. C) Fluorometric microplate Nile-Red analysis under different nitrogen concentrations. Data represent the mean values of triplicates ±1 SE.

https://doi.org/10.1371/journal.pone.0091957.g004

Antioxidant Enzyme Activities, Pigment Composition and Protein Analyses Under Different Nitrogen Concentrations

ROS accumulation is prevented by a powerful intrinsic antioxidant system in photosynthetic organisms, involving enzymes such as superoxide dismutase (SOD), catalase (CAT), ascorbate peroxidase (APX) [37]. Next, we analyzed these three oxidative stress indicator antioxidant enzymes to demonstrate the effect of nitrogen depletion on the intracellular oxidative stress status as also supplementary to DCFH-DA measurements.

Intracellular SOD converts O2 to O2 and H2O2, acting as the first line of defence against oxidative stress [38]. We observed that SOD activity of cells increased under low nitrogen concentrations, especially at stationary growth phase. This data suggests that superoxides may be elevated under nitrogen depleted conditions, necessitating increased SOD activity (Figure 5A). CAT is a heme-containing enzyme that catalyzes the conversion of H2O2 into oxygen and water [37]. APX is involved in the ascorbate-glutathione cycle occuring in chloroplasts, cytoplasm, mitochondria and perixisomes [39]. We observed elevated levels of CAT and APX activity under nitrogen depleted conditions (Figure 5B, 5C). These data strongly indicate that oxidative stress is induced under nitrogen depletion in Dunaliella salina strain Tuz_KS_01.

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Figure 5. Antioxidant enzyme activities under different nitrogen concentrations.

A–C) Spectrophotometric enzymatic assays for catalase (CAT), ascorbate peroxidase (APX) and superoxide dismutase (SOD). Data demonstrate the mean values of triplicates ±1 SE.

https://doi.org/10.1371/journal.pone.0091957.g005

Next, we analyzed the chlorophyll, carotenoid and protein content change in response to nitrogen depletion in Dunaliella salina strain Tuz_KS_01. Chlorophyll content is an indicator of photosynthetic efficiency, rate and nitrogen [40] status. Carotenoids can perform an essential role in photoprotection by quenching the triplet chlorophyll and scavenging singlet oxygen and other reactive oxygen species [41]. We observed that chlorophyll A and B levels sharply declined in low nitrogen conditions, as expected (Figure 6A). In contrast, we observed no decrease in total carotenoid contents under nitrogen depletion conditions. This observation suggests that cells increase caroteoid content to overcome with oxidative stress induced by singlet oxygens, similar to SOD activity increase discussed above (Figure 6A).

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Figure 6. Pigment and protein contents of Dunaliella salina strain under different nitrogen concentrations.

A) Chlorophyll A, B and total carotenoid contents under different nitrogen concentrations. B) Protein contents of Dunaliella salina strain Tuz_KS_01 cells cultivated under different nitrogen concentrations Data demonstrate the mean values of triplicates ±1 SE.

https://doi.org/10.1371/journal.pone.0091957.g006

Upon nitrogen starvation, algal cells reduce the synthesis of protein and nucleic acid synthesis and carbon flow is directed from protein synthesis to fatty acid and carbonhydrate synthesis [42]. We found that neutral lipids increase while the protein content of algal cells was reduced under nitrogen depletion conditions (Figure 6B). This indicates that carbon flow direction is to fatty acid synthesis under nitrogen limitation at stationary phase, in accordance with the literature [43].

Reactive Oxygen Species (ROS) Production Induces Lipid Accumulation

Our analysis thus far hints that lipid accumulation might be partially triggered by ROS accumulation and oxidative stress under nitrogen depleted condition (Figure 4). In order to test this hypothesis, we used H2O2, a well-known oxidative stress inducer [44]. We treated cells at exponential growth phase in high nitrogen containing media (5 mM) with different concentrations of H2O2 and we measured ROS, via using flowcytometric DCFH-DA method, a robust fluorescent assay [45]. In addition, cell viability was measured by using FDA fluorescent assay while using Nile red staining method for determination of lipid contents under different H2O2 concentrations. Although cellular size and granularity under H2O2 treated conditions were similar to previous experimental conditions (Figure 7A and 3A), cell survival under higher H2O2 concentrations were observed significantly reduced due to the oxidative stress induction (Figure 7B–7C). Although reduction of cell survival is to ∼20% at 4 mM H2O2 concentration, at this high concentration of H2O2, new isolate Dunaliella salina strain Tuz_KS_01 showed highly tolerant characteristics to oxidative stress (Figure 7D).

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Figure 7. Effect of H2O2, a known oxidative stress inducer, on Dunaliella salina strain Tuz_KS_01.

A) Zebra-plot of SSC (Side Scatter) and FSC (Forward Scatter) expressing cellular granulation and cellular size under a representative H2O2 condition (4 mM). B) Histogram of flow-cytometric analysis of ROS accumulation under different H2O2 concentrations. C) Percentage increase of ROS production based on flow-cytometric DCFH-DA analysis. D) Fluorometric microplate fluorescent diacetate (FDA) survival analysis cultivated under different H2O2 concentrations. E) Fluorometric microplate Nile-Red analysis under different H2O2 concentrations. Data represent the mean values of triplicates ±1 SE.

https://doi.org/10.1371/journal.pone.0091957.g007

Lipid accumulation of algae is known to increase by various factors including temperature, excessive light, and pH, which may also related to oxidative stress induced by ROS accumulation [33], [46]. We used fluorometric Nile red analysis for analysis of lipid accumulation under different H2O2 treatments. We observed increased lipid accumulation with increasing concentrations of H2O2 (Figure 7E). This result supports that the lipid accumulation observed under nitrogen depletion conditions is at least partly mediated by oxidative stress. Importantly, this result also suggests a method for obtaining high lipid from green alga, namely by growing cells in high nitrogen (optimal) conditions followed by oxidative stress induction at stationary phase. Such a method may be economically more feasible than two stage reactors described above.

We next wished to visually observe the effect of nitrogen depletion and H2O2 treatment on lipid accumulation. After cultivation, we collected and stained cells with Nile red and observed with fluorescence microscopy. We used three different conditions: 1) control, 2) 0.05 mM nitrogen and 3) 4 mM H2O2. Microscopy results were in strong agreement with our previous results, as lipid accumulation (increased size and number of cytoplasmic lipid droplets) after nitrogen depletion or H2O2 treatment was higher than the control (Figure 8A–8B–8C).

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Figure 8. Fluorescence microphotographs of Dunaliella salina strain Tuz_KS_01 stained with Nile-Red fluorescence dye and screened under 400X magnification.

A) Control group, 5 mM nitrogen concentration cultivation condition. B) Nitrogen limitation group, 0.05 mM nitrogen condentration cultivation condition C) Oxidative stress group, 4 mM H2O2 cultivation condition. Gravimetric lipid content analysis and Nile-Red fluorescence measurement correlation D) Gravimetric and fluorometric Nile-Red lipid content analysis of Dunaliella salina strain Tuz_KS_01 under 0.05 mM nitrogen and 4 mM H2O2 cultivation conditions. Data represent the mean values of triplicates ±1 SE E) Correlation plot of gravimetric and fluorometric Nile-Red lipid content analysis (r2 = 0.82).

https://doi.org/10.1371/journal.pone.0091957.g008

Moreover, in order to validate the lipid increasing effect of nitrogen limitation and H2O2 induced oxidative stress, solvent extraction gravimetric lipid analysis in nitrogen depleted (0.05 mM) and H2O2 containing media (4 mM) were done. We found that, nitrogen limitation led to increased lipid accumulation up to 35%, and H2O2 induced oxidative stress led to increased lipid accumulation up to 44% as shown in Figure 8D. We also measured the lipid content by Nile red fluorescence analysis for each of these conditions. Consistent with previous studies, we found that gravimetric and fluorometric measurements were correlated (r2 = 0.82) (Figure 8E) [17]. These data suggest that exogenously induced oxidative stress triggered by the application of H2O2 resulted to increased lipid accumulation. Therefore, as previously shown by the fluorometric analyses above, oxidative stress and increased lipid accumulation association is coupled under nitrogen limitation conditions. Induction of lipid accumulation by applying exogeneous oxidative stress inducers such as H2O2 may assist more effective lipid production compared with biomass production lowering nitrogen starvation strategy.

ROS production resulting from various stress factors is known to affect nearly all cellular processes by impairing the structural stability of functional macromolecules including DNA, proteins and structural lipids. Since the green algae life-cycle is reliant on its photosynthetic activity and cellular integrity, it is crucial to protect against oxidative stress. Otherwise cells can not tolerate oxidative damage and eventually die [47][49]. Even though there is limited explanation about the correlation between ROS production and lipid accumulation in algae cultivated under nitrogen depleted conditions. Our results indicate that nitrogen depletion results in ROS accumulation and lipid peroxidation especially at stationary growth phase. This relationship might also be related to survival response of the alga against excessive oxidative stress conditions [7].

Although a few recent studies have suggested an association of ROS levels and cellular lipid accumulation [7], [8], underlying mechanistic principles are not clear. ROS is well demonstrated to modify cellular responses against different stressors in corresponding signal transduction pathways. ROS levels increase in microalgae cells when exposed to the different environmental stresses [9]. In a recent study, nitrogen depletion was shown to correlate with increased ROS accumulation and increased cellular lipid accumulation in a freshwater algae. This study showed that increased MDA concentration is an indicator of membrane peroxidation which implied increased ROS levels. It was suggested that H2O2 induced exogenous oxidative stress was an effective factor for neutral lipid induction in C. sorokiniana C3 [50].

Microalgae can modify its photosynthetic system under stress, resulting in a decrease in the gene expression of various proteins forming up the photosystem complexes I and II [51]. Such adjustments are thought to occur for minimizing oxidative stress via decreasing photosynthesis rate [52]. Nitrogen deprivation is closely associated with the degradation of ribulose-1,5-bisphosphate carboxylase oxygenase to recycle nitrogen [53]. Degradation of this protein may result in alterations in photosynthesis rate, which is consistent with the observed decrease in chlorophyll content under nitrogen depleted condition [54]. As a result of decreased photosynthesis rate, overall anabolic reaction flux is severely constrained. In this context, algae cells may favor storage of energetic molecules, such as lipids, instead of consumption.

Effects of H2O2 Induced Oxidative Stress on Lipid Accumulation in Dunaliella tertiolecta and Chlamydomonas reinhardtii

Green algae, Dunaliella tertiolecta and Chlamydomonas reinhardtii were chosen for further investigation and confirmation of the H2O2 induced oxidative stress effects on cellular lipid accumulation. We cultivated cells in high nitrogen containing media (5 mM) with different concentrations of H2O2 as described for Dunaliella salina strain Tuz_KS_01. We measured ROS by using the DCFH-DA method, cell viability by using the FDA fluorescent assay, and lipid content by using the fluorometric Nile Red method, as described above. Dunaliella tertiolecta cells were found to be more tolerant to H2O2; therefore higher concentrations of H2O2 were used to demonstrate the cellular response. Chlamydomonas reinhardtii cells were treated within the range from 200 μM to 4 mM H2O2 concentrations while Dunaliella tertiolecta cells were treated within the range of 2 mM to 8 mM H2O2 concentrations. As shown in Figure 9, we found that in response to H2O2 in both species ROS accumulation and lipid contents increased, while cell survival dramatically decreased at high H2O2 concentrations. In addition, by using flow cytometric analysis, we observed that lipid increase in response to oxidative stress was accompanied with increased granulation and biovolume in Chlamydomonas cells (Figure 10). Neither Dunaliella tertiolecta nor Dunaliella salina strain Tuz_KS_01 cells showed biovolume increase upon treatment of H2O2 at any experimented concentration.

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Figure 9. Effect of H2O2 induced oxidative stress on cellular lipid accumulation of different algae species.

A) Fluorometric DCFH-DA and FDA analyses showing percantage change of ROS production and percentage change of cell survivability of Chlamydomonas reinhardtii cells cultivated under different H2O2 concentrations. B) Fluorometric Nile red analysis showing the effect of different H2O2 concentrations on cellular lipid accumulation of Chlamydomonas reinhardtii cells C) Fluorometric DCFH-DA and FDA analyses showing percantage change of ROS production and percentage change of cell survivability of Dunaliella tertiolecta cells cultivated under different H2O2 concentrations. D) Fluorometric Nile Red analysis showing the effect of different H2O2 concentrations on cellular lipid accumulation of Dunaliella tertiolecta cells. Data represent the mean values of triplicates ±1 SE.

https://doi.org/10.1371/journal.pone.0091957.g009

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Figure 10. Flow cytometric Nile red, cellular granulation and biovolume analysis of Chlamydomonas reinhardtii cells cultivated under different H2O2 concentrations.

A) A representative histogram of flow-cytometric analysis of lipid contents under different H2O2 concentrations. B) Zebra-plot of SSC (Side Scatter) and FSC (Forward Scatter) expressing cellular granulation and cellular size, respectively, under different H2O2 concentrations. Data represent the mean values of triplicates ±1 SE.

https://doi.org/10.1371/journal.pone.0091957.g010

Conclusions

Nitrogen depletion has been shown to be an effective inducer of lipid production of various unicellular green algae by previous studies. But few studies have examined the physiological and biochemical mechanisms underlying this response. In this study, we isolated a new halophilic green alga species. We presented evidence supporting previous observations that nitrogen depletion causes oxidative stress and lipid accumulation. In addition, we showed that oxidative stress by itself can cause lipid accumulation, suggesting that lipid accumulation under nitrogen depletion is mediated by oxidative stress. These observations are helpful for utilization of green alga for biodiesel production.

Acknowledgments

Authors would like to thank UTEX, The Culture Collection of Algae, for providing kindly of algae species, Chlamydomonas reinhardtii and Dunaliella tertiolecta. MC was supported by Turkish Academy of Sciences Gebip Programme.

Author Contributions

Conceived and designed the experiments: KY MC SC. Performed the experiments: KY IP. Analyzed the data: KY MC. Contributed reagents/materials/analysis tools: SC MC BE. Wrote the paper: KY MC IP SC.

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