Skip to main content
PMC home page
Frontiers in Plant Science logoLink to Frontiers in Plant Science
. 2018 May 7;9:590. doi: 10.3389/fpls.2018.00590

Elevated Inorganic Carbon Concentrating Mechanism Confers Tolerance to High Light in an Arctic Chlorella sp. ArM0029B

Kwon Hwangbo 1,2, Jong-Min Lim 1, Seok-Won Jeong 2, Jayaraman Vikramathithan 1, Youn-Il Park 2, Won-Joong Jeong 1,*
PMCID: PMC5949578  PMID: 29868055

Abstract

Microalgae and higher plants employ an inorganic carbon (Ci) concentrating mechanism (CCM) to increase CO2 availability to Rubisco. Operation of the CCM should enhance the activity of the Calvin cycle, which could act as an electron sink for electrons generated by photosynthesis, and lower the redox status of photosynthetic electron transport chains. In this study, a hypothesis that microalgal cells with fully operating CCM are less likely to be photodamaged was tested by comparing a Chlorella mutant with its wild type (WT). The mutant acquired by screening gamma-ray-induced mutant libraries of Chlorella sp. ArM0029B exhibited constitutively active CCM (CAC) even in the presence of additional Ci sources under mixotrophic growth conditions. In comparison to the WT alga, the mutant named to constitutively active CCM1 (CAC1) showed more transcript levels for genes coding proteins related to CCM such as Ci transporters and carbonic anhydrases (CA), and greater levels of intracellular Ci content and CA activity regardless of whether growth is limited by light or not. Under photoinhibitory conditions, CAC1 mutant showed faster growth than WT cells with more PSII reaction center core component D1 protein (encoded by psbA), higher photochemical efficiency as estimated by the chlorophyll fluorescence parameter (Fv/Fm), and fewer reactive oxygen species (ROS). Interestingly, high light (HL)-induced increase in ROS contents in WT cells was significantly inhibited by bicarbonate supplementation. It is concluded that constitutive operation of CCM endows Chlorella cells with resistance to HL partly by reducing the endogenous generation of ROS. These results will provide useful information on the interaction between CCM expression, ROS production, and photodamage in Chlorella and related microalgae.

Keywords: CCM, high light tolerance, ROS, photodamage, Chlorella

Introduction

Light is essential for photosynthesis, but excess light can be damaging as it can increase the formation of reactive oxygen species (ROS) (Aro et al., 1993). These include singlet oxygen (1O2), which is produced at the reaction center of photosystem II (PSII; Vass, 2011); superoxide (O2–); and hydrogen peroxide (H2O2). The latter is generated during the Mehler-ascorbate peroxidase (MAP) cycle (Nishiyama et al., 2004; Roberty et al., 2014). ROS can directly damage PSII or inhibit its repair (Murata et al., 2007; Vass and Cser, 2009). The compounds can also result in lipid peroxidation, site-specific amino acid modifications, and mutations (Lesser, 2006). In addition to these destructive effects, ROS also plays a role as signaling molecules in various biochemical and physiological responses leading to improving stress tolerance or causing programmed cell death (Bechtold et al., 2008; Lemoine and Schoefs, 2010; Foyer and Shigeoka, 2011).

Photosynthetic organisms have several protective mechanisms against ROS-induced damage. All photosynthetic organisms perform non-photochemical quenching, which dissipates absorbed excess light energy as heat, reducing the energy reaching the PSII reaction center (Muller et al., 2001). The size of the chlorophyll-containing light-harvesting complex is regulated by the intensity of light in the environment: when light it excessive, the number of light-harvesting antenna molecules decreases, reducing the amount of light absorbed (Smith et al., 1990; Melis, 1991). The D1 protein in the reaction center of PSII is particularly susceptible to light-induced oxidative damage. PSII has efficient and dynamically regulated machinery that selectively degrades photodamaged D1 and replaces it with new D1 protein (Ohad et al., 1984; Aro et al., 1993). Photorespiration plays an important role in PSII protection against ROS (Kozaki and Takeba, 1996; Baroli and Melis, 1998; Wang et al., 2015). Recently, it was demonstrated that the addition of bicarbonate to the culture medium of a microalga alleviated oxygen stress via increase in the ratio of dissolved CO2 to dissolved O2, that would lead to lowering ROS generation (Peng et al., 2017).

Aquatic organisms must acquire the CO2 that they need from the surrounding water, in which it diffuses 10,000 times more slowly than it does in air. These organisms have overcome this limitation by evolving an inorganic carbon (Ci) concentrating mechanism (CCM) to increase Ci in the cell. The CCM improves the photosynthetic performance of the organism by increasing the CO2 concentration in the vicinity of Rubisco. This simultaneously enhances carbon fixation and suppresses photorespiration (Wang et al., 2015). The CCM contains an Ci transporter for CO2 and HCO3–, a pyrenoid that serves as a barrier to CO2 leakage, and a carbonic anhydrase (CA) that carries out interconversion of CO2 and HCO3– (Wang et al., 2011). The CCM is induced when CO2 is limiting and is mainly regulated by Ci concentration (Giordano et al., 2005).

The CCM of microalgae is induced not only by limiting CO2 but by high light (HL) (Wang et al., 2011). Expression of several CCM genes in cyanobacteria, Chlamydomonas, and diatoms was induced by the combination of low CO2 and HL conditions (Hihara et al., 2001; Huang et al., 2002; Im and Grossman, 2002; Heydarizadeh et al., 2017), but not by the combination of HL and high-CO2 conditions. It may be, then, that the HL signal is insufficient for the induction of CCM genes in microalgae (McGinn et al., 2003; Woodger et al., 2003).

The CO2 fixed by Rubisco in the Calvin cycle is the final electron acceptor of photosynthetic electron flow, and the availability of CO2 affects the amount of photodamage. This was demonstrated in Chlamydomonas reinhardtii (Baroli and Melis, 1998) and Dunaliella salina (Fischer et al., 2006) grown under HL conditions. As CO2 was depleted in these algae, the rate of photodamage increased.

It has been suggested that activation of CCMs could reduce photodamage by increasing the CO2 levels in cells. If this is the case, then, the operation of the CCM that enhances Calvin cycle activity could act as a sink for the electrons generated by photosynthesis, and hence lower the redox status of photosynthetic electron transport chains. Under these conditions, cells with fully operating CCMs would be less likely to be damaged by light. This hypothesis was tested using a mutant of Chlorella sp. ArM0029B, a species from the arctic (Ahn et al., 2012). The mutant named to constitutively active CCM1 (CAC1) has constitutive expression of CCM and HL tolerance under mixotrophic growth conditions. The physiological and biochemical differences between the wild-type (WT) alga and CAC1 grown at low and HL conditions were characterized and compared.

Materials and Methods

Mutant Isolation and Culture Conditions

Cells of Chlorella sp. ArM0029B were cultured at 25°C in Tris–acetate–phosphate (TAP) medium (Harris, 1989). Mutants of this species were generated by irradiating cells with 300 Gy (100 Gy per hour) in a 60Co gamma irradiator (150 TBq Capacity; ACEL, Nordion, Ottawa, ON, Canada) at the Korean Atomic Energy Research Institute. A mutant tolerant to HL intensity was isolated from the mutant library by growing cultures under intermediate light intensity (300–350 μmol m-2 s-1). The mutant was named to “CAC1”. Cultures were grown under low [referred to as low light (LL); 50–80 μmol m-2 s-1] or HL (650–800 μmol m-2 s-1) intensities. Growth rate was assessed by counting cells under a microscope after 0.5 × 106 cells ml-1 was inoculated in 50 ml culture.

Identification of CCM Genes in Chlorella sp. ArM0029B

Carbon concentrating mechanism-related genes were identified from the genome information of Chlorella sp. ArM0029B as part of genome project (funded by Advanced Biomass R&D Center). A Basic Local Alignment Search Tool (BLAST) search was performed, using CCM proteins of C. reinhardtii as bait, to identify homologs of CCM proteins in Chlorella.

Western Blot

Total proteins were extracted from WT and mutant cells according to the method of Minko et al. (1999). Total protein (1 × 107 cells) was separated in a 15% (w/v) polyacrylamide gel (Laemmli, 1970) and transferred onto an Immobilon-P membrane (Millipore, Billerica, MA, United States). Rabbit anti-AtpB, LhcB2, PsaC, and PsbA polyclonal antibodies (Agrisera, Vännä, Sweden) were used to detect specific proteins. Immunodetection was performed using chemiluminescence (ECL; Amersham, Arlington Heights, IL, United States) according to the manufacturer’s instructions. Band densities were measured using ImageJ software (NIH, Bethesda, MD, United States); western blots band densities were normalized to total proteins stained with Ponceau S.

RNA Analysis

Total RNA was extracted from WT and mutant cells (approximately 1 × 108 cells) using TRIzol reagent (Invitrogen, Carlsbad, CA, United States) according to the manufacturer’s instructions. For northern blot analysis, 15 μg of total RNA was separated by agarose gel electrophoresis and blotted onto a Hybond-N nylon membrane (Amersham Biosciences, Marlborough, MA, United States). DNA fragments that had been amplified with gene-specific primers were used as probes (Supplementary Table S1). After hybridization with a 32P-labeled probe, the membrane was washed and exposed to a phospho-imaging plate (Fujifilm, Tokyo, Japan) for 1–3 days. The hybridization signals were detected with Bio-Imaging Analyzer BAS-1800II (Fujifilm, Tokyo, Japan). For semi-quantitative PCR analysis, reverse transcription (RT) was carried out using 2 μg of total RNA with oligo-dT, 200 U of murine moloney leukemia virus (M-MLV) reverse transcriptase (Promega, Madison, WI, United States), 500 μM of each dNTP, and 20 U of ribonuclease inhibitor. Semi-quantitative RT-PCR analysis was performed with 25–35 cycles using each gene-specific primer (Supplementary Table S1). The expression of the small subunit 3 of the Rubisco gene (rbcS3; MG669272) was used as a loading control. Band densities were measured using ImageJ software (NIH, Bethesda, MD, United States); for northern blots and semi-quantitative RT-PCR, band densities were normalized to loading control.

Measurements of Intracellular Ci, Fluorescence Parameter (Fv/Fm), and Photosynthetic O2 Evolution

Intracellular Ci levels were measured according to Park et al. (1999), in which oxygen evolution is correlated with intracellular Ci, with some modifications. The cells (3 × 108 cells) were washed three times with CO2-free 20 mM MES. The amount of oxygen generated by the cell was measured with an Oxylab oxygen electrode (OXYL1; Hansatech, King’s Lynn, United Kingdom). The maximal photochemical efficiency as estimated with the chlorophyll fluorescence parameter Fv/Fm determined according to Kitajima and Butler (1975) with a Handy Plant Efficiency Analyzer (Hansatech, King’s Lynn, United Kingdom). Light response curves for photosynthetic O2 evolution rate were measured with an Oxylab oxygen electrode (OXYL1; Hansatech, King’s Lynn, United Kingdom) at 0, 250, 500, 750, and 1,000 μmol photons m-2 s-1. Each light intensity was applied for 5 min. Chlorophyll contents were determined as previously described (Porra et al., 1989).

Determination of Carbonic Anhydrase Activity

Carbonic anhydrase activity was determined by the potentiometric method of Wilbur and Anderson (1948) with some modifications. Cultures with 108 cells were centrifuged at 3,000 rpm for 5 min and washed twice with 10 mM Tris buffer (pH 8.3) containing 1 mM dithiothreitol (DTT) and 1 mM EDTA. For detection of extracellular CA activity, the integrity of the cells in the pellet was confirmed by viewing them under the microscope. They were resuspended in the same Tris buffer and enzymatic activity was measured immediately. For detection of total CA activity, the pelleted cells were ground with a tissue lyser (QIAGEN, Hilden, Germany) in liquid nitrogen to a fine powder. Ground tissue was resuspended in the same Tris buffer and the enzymatic activity of the total extract was measured.

In Vivo Detection of ROS

Production of ROS was detected by the method of Halliwell and Gutteridge (1999) with some modifications. Cell suspensions containing 1 × 107 cells in 2 ml of medium supplemented with 5 μM 2′,7′-dichlorofluorescein-diacetate (DCF-DA) at 25°C were incubated in the dark for 1 h with shaking. The fluorescence of the samples was measured with a spectrofluorometer (Model LS55; PerkinElmer, Norwalk, CT, United States) at room temperature, with an excitation wavelength of 485 nm and an emission band between 500 and 600 nm. The fluorescence intensity at 520 nm (F520) was used to determine the relative ROS production.

Statistical Analysis

For statistical analysis, SPSS software (version 25; IBM, Armonk, NY, United States) was used. The treatment effects were evaluated by a Tukey’s test (p < 0.01).

Results

High-Light-Tolerant Mutant Exhibited Constitutively Active CCM Under Mixotrophy

Photosynthetic O2 evolution rates of Chlorella WT cells grown under LL or HL intensities revealed saturation behavior above 500 μmol m-2 s-1 (Supplementary Figure S1). In the present study, intermediate light condition (300–350 μmol m-2 s-1) was chosen for screening mutants from the mutant libraries by incubating them on agar plates. Limiting light intensity would be too low to induce photoinhibition of photosynthesis, while excess light would be too high, lowering the chance of algal cells survived. Out of about 3,000 random mutants screened, a fast-growing, HL-tolerant mutant was isolated from the intermediate light condition. This HL resistance was also observed in liquid growth conditions. Growth of this mutant and the WT grown in liquid media were similar at LL, but the mutant grew rapidly in HL where WT growth were severely inhibited (Figure 1).

FIGURE 1.

FIGURE 1

Open in a new tab

Growth of wild-type (WT) and CAC1-mutant cells under photosynthesis limiting low light (LL, 50–80 μmol m-2 s-1) and saturating, high light (HL, 650–800 μmol m-2 s-1) intensities for 7 days. Data are the means ± SE (n = 3).

To correlate CCM machinery with HL tolerance of the mutant, transcript levels of CCM genes, CA activity, and intracellular Ci content were assessed. Genome of Chlorella sp. ArM0029B contains CCM genes such as : two bicarbonate transporter genes [HLA3 and LCIA1020; homologs for HL-induced gene 3 (HLA3) and low CO2-induced gene A (LCIA) of C. reinhardtii], one CO2 channel gene [RHP1; homolog for rhesus-like proteins 1 and 2 (RHP1/2) of C. reinhardtii], one Ci transporter gene [CCP430; homolog for low-CO2-inducible chloroplast envelope proteins 1 and 2 (CCP1/2) of C. reinhardtii], four low-CO2-inducible genes [LCI420, LCI450, LCI70, and LCI520; homologs for low CO2-induced gene B, C, D, and E (LCIB, LCIC, LCID, and LCIE) of C. reinhardtii], and five CA genes [CAH230, CAH200, CAH920, CAH1510, and CAH0010; homologs of CA 1, 2, 3, 5, 7, and 9 (CAH1, CAH2, CAH3, CAH5, CAH7, and CAH9) of C. reinhardtii]. More information is included in Figure 2. Transcript levels of these genes assessed by Northern and RT-PCR analyses demonstrated that most of CCM genes were constitutively and highly expressed in mutant, relative to the WT (Figure 3 and Supplementary Figure S2). In the WT alga, expression of genes encoding Ci transporters and CAs in the HL was lower (0.61–0.96-fold) than in LL (Figure 3), while in HL, there were 1.24–2.99-fold more transcripts of LCI70, LCIA1020, and CAH1510 than were present in LL. Most of CCM genes, specifically HLA3, CCP430, LCI420, LCI520, LCI450, LCI70, CAH920, CAH1510, CAH230, CAH0010, and RHP1 were 1.42–7.87-fold highly expressed when cultures were supplemented with bicarbonate, compared to bicarbonate-free cultures, although expression of LCIA1020 and CAH200 was decreased (0.67–0.71-fold) and 1.51–0.67-fold increased, respectively, in bicarbonate. Expression of CCM genes was either unchanged or slightly lower (0.46–0.91-fold) when cultures were supplemented with high CO2 (Supplementary Figure S3).

FIGURE 2.

FIGURE 2

Open in a new tab

Proposed composition of CCM and relative transcript changes of CCM genes in WT and CAC1 of Chlorella sp. ArM0029B. Color codes indicate relative transcripts level of CCM genes in CAC1 mutants compared to WT grown under LL (50–80 μmol m-2 s-1) or HL (650–800 μmol m-2 s-1) conditions. Localization of each proteins was predicted by subcellular localization prediction tools including TargetP v1.1 (Emanuelsson et al., 2007), ChloroP v1.1 (Emanuelsson et al., 1999), SignalP v4.1 (Emanuelsson et al., 2007), SMART v8 (Letunic et al., 2014), and TMHMM v2.0 (Krogh et al., 2001). Ci transporter, CCP430 (MG669265); bicarbonate transporters, HLA3 (MG669266) and LCIA1020 (MG669271); CO2 channel, RHP1 (MG669273); low CO2 inducible proteins, LCI70 (MG669267), LCI420 (MG669268), LCI450 (MG669269), and LCI520 (MG669270); carbonic anhydrases, CAH200 (MG669261), CAH230 (MG669262), CAH0010 (MG669260), CAH920 (MG669263), and CAH1510 (MG669264). GenBank accession numbers of each genes are in parentheses.

FIGURE 3.

FIGURE 3

Open in a new tab

Transcript levels of CCM genes in WT and CAC1-mutant grown under photosynthesis limiting LL (50–80 μmol m-2 s-1) and saturating, HL (650–800 μmol m-2 s-1) intensities for 3 days. The Northern blot and RT-PCR bands were quantified from Supplementary Figure S2 and shown as relative abundance normalized to the WT expression level, which is considered as 1.0.

There was more expression of the CCM genes in the mutant than in the WT under both light regimes. Especially, the expression of genes encoding the HLA3 homolog and the LCIB/C homologs was 1.15–5.39-fold more increased in the mutant compared to the WT. In contrast, expression of LCI520, LCI450, LCI70, and LCIA1020 in the mutant was slightly lower (0.29–0.7-fold) in HL than in LL, but the expression was still higher (1.1–1.75-fold) except for LCIA1020 in the mutant than in the WT. Similarly, while the expression of HLA3, LCI420, and LCI520 was less (0.42–0.91-fold) when the mutant was supplemented with bicarbonate, these were also still 1.17–1.69-fold greater in the mutant than in the WT. Expression of RHP1 in algae was detected only in when bicarbonate was supplied. Expression of this gene was similar in both algae under LL, but was 1.55-fold higher in the mutant than in the WT under HL (Figure 3).

Carbon concentrating mechanism machinery is massively under the transcriptional control (Brueggeman et al., 2012). Thus, differential expression of CAHs between the WT and the mutant as described above should be manifested as changes in CA activities. As expected, CA activity in both algae was less in HL than in LL, but the CA activity in the mutant was much greater than in the WT (Figure 4A). Compared to the WT alga, under LL, the total CA activity of the mutant was 4.5 times greater; extracellular activity was seven times greater, and intracellular CA activity was 2.5 times greater. Compared to the WT, under HL, the total CA activity of mutant was 1.7 times greater, extracellular CA activity was 2.4 times greater, while intracellular CA activity was similar in the two algae.

FIGURE 4.

FIGURE 4

Open in a new tab

Carbonic anhydrase (CA) activity (A), intracellular inorganic C (Ci) content (B), and intracellular Ci consumption time (C) in WT and CAC1 mutant grown under photosynthesis limiting LL (50–80 μmol m-2 s-1) and saturating, HL (650–800 μmol m-2 s-1) intensities for 3 days. eCA, extracellular CA activity; iCA, intracellular CA activity; total, eCA activity + iCA activity; data are means ± SE (n = 3). Means denoted by different letters indicated significant difference at p < 0.01 according to Tukey’s test.

Cells with a CAC would contain high content of intracellular Ci. Indeed, in LL, the intracellular Ci content in the mutant was 1.4 times greater than that of the WT (Figure 4B). However, intracellular Ci in the WT and the mutant was comparable under HL (Figure 4B). Interestingly, the mutant consumed the intracellular Ci 4.2-fold faster than that in WT (Figure 4C). Overall, the mutant isolated under the intermediate light showed a phenotype with CAC and hence was named as CAC1.

Photosynthetic Apparatus, ROS, and Growth Performance

If CCM have a role for lowering the extent of PSII photodamage, the primary target of photoinhibition, then CAC1 with robust CCM grow faster than WT cells under HL condition. First, the extent of photodamage in the WT and mutant algae grown under HL was compared by assessing the amount of D1 protein, PSII photochemical efficiency, photosynthetic O2 evolution rate, and cell growth curves. These analyses were done in cells cultured for 3 days. Fast growing phase of the WT and CAC1 supplemented with additional bicarbonate observed between 2 and 3 days after inoculation, followed by stationary phase (Figure 1). Three-day old cells rather than stationary phase cells were chosen to avoid the involvement of other factors such as high-density-related nutrient deficiency and self-shading in the process of PSII photodamage and repair processes. In the WT, there was less (0.49-fold) D1 protein (PsbA) in HL than in LL, although the psbA expression was not changed, indicating that the WT cells were under the photoinhibitory condition. In the mutant, however, levels of the D1 protein as well as expression of psbA were similar in both light regimes (Figure 5A). Consistent with D1 protein levels, maximal photochemical efficiency of PSII estimated as a fluorescence parameter, Fv/Fm, and maximal photosynthetic O2 evolution rate of HL adapted WT cells was 73 and 36% of the CAC1, respectively (Figure 5B and Supplementary Figure S1). Taken together, these data strongly indicate that CAC1 are more resistant than the WT to HL stress.

FIGURE 5.

FIGURE 5

Open in a new tab

Western and northern analyses of PSII core protein PsbA (A) and maximal photochemical efficiency of PSII (Fv/Fm) (B) of WT and CAC1 mutant grown under photosynthesis limiting LL (50–80 μmol m-2 s-1) and saturating, HL (650–800 μmol m-2 s-1) intensities for 3 days. The Western blot bands were quantified and shown as relative abundance normalized to D1 (PsbA) accumulation level in the WT, which is considered as 1.0. Data are means ± SE (n = 4). MB, methylene blue staining; PS, Ponceau S-staining. Means denoted by different letters indicated significant difference at p < 0.01 according to Tukey’s test.

If HL resistance observed in CAC1 mutant is related to enhanced Ci content, then bicarbonate or gaseous CO2 supplies would restore growth of the WT cells comparable to CAC1 under HL. This view was tested by assessing cell growth supplied with either bicarbonate (10 mM) or high CO2 (2%) under intermediate light. A spot growth test (visualization of growth on agar medium) demonstrated that growth of both the WT and CAC1 was slightly increased in high CO2 compared to the non-supplemented controls, but CAC1 still grew faster than the WT (Supplementary Figure S4). However, bicarbonate supplementation markedly increased growth of the WT cells, being similar to that of CAC1 (Supplementary Figure S4). This apparent restoration was also apparent in liquid culture under HL condition (Figure 6), supporting the view that CCM has a photoprotective role against HL stress.

FIGURE 6.

FIGURE 6

Open in a new tab

Growth of WT and CAC1 mutant supplemented with Ci source (10 mM NaHCO3) under HL (650–800 μmol m-2 s-1) intensities for 7 days. Data are means ± SE (n = 3).

Finally, a positive role of CCM against photodamage was predicted to be that, first, CAC1 cells would have lowered ROS contents and, second, enhanced Ci levels alleviate ROS contents. As predicted, in HL CAC1 contained less (0.56-fold) ROS contents compared to the WT cells (Figure 7). In HL compared to LL, ROS content increased 2.74-fold in the WT but 1.45-fold in the mutant (Figure 7). Further, bicarbonate supplementation to the WT cells significantly inhibited increases in ROS contents. In HL WT cells without additional bicarbonate contained 1.68-fold higher ROS than those supplemented with bicarbonate (Figure 7).

FIGURE 7.

FIGURE 7

Open in a new tab

ROS contents in WT and CAC1 mutant grown under photosynthesis limiting LL (50–80 μmol m-2 s-1) and saturating, HL (650–800 μmol m-2 s-1) intensities for 3 days. Data are means ± SE (n = 4). Means denoted by different letters indicated significant difference at p < 0.01 according to Tukey’s test.

Discussion

In photosynthetic organisms, including algae, HL leads to the generation of ROS, which damages the photosynthetic apparatus and impairs growth (Murata et al., 2007; Vass and Cser, 2009). Enhanced Ci contents would lower ROS generation via enhanced utilization of reducing power and ATP generated during light-dependent reaction of photosynthesis. In the present study, this view was supported by characterization of the CAC1 mutant of an arctic species of Chlorella sp. ArM29B.

Constitutively active CCM1 is tolerant to light intensity above 150 μmol m-2 s-1 where the growth of the WT begins to be compromised (data not shown). In HL-grown WT, cell growth was severely reduced due to PSII photodamage as revealed by lowered D1 protein content, maximal photochemical efficiency of PSII (estimated by Fv/Fm parameter), and maximal photosynthesis rate. In contrast, these parameters in the CAC1 mutant were less affected in the same light treatment, indicating that CAC1 mutant is more resistant to photodamage than WT.

Reactive oxygen species can induce photodamage, which reduces photosynthesis and growth. ROS content increased drastically in HL in the WT, but there was less effect in the mutant (Figure 7). The addition of bicarbonate to the WT cells in HL reduced the content of ROS to levels comparable to those in CAC1. As expected, bicarbonate addition to the WT culture in HL increased the accumulation of the D1 protein (Supplementary Figure S5). It appears that the bicarbonate enabled the WT alga to “mimic” the performance of the mutant phenotypically. The WT cells appear to possess protective mechanisms against HL, but ROS may accumulate above the cells’ capacity for protection, and directly damage the cells’ photosystems. It may be, then, that the cellular damage inflicted by ROS could be alleviated by the addition of effective electron acceptors. Of note here is that the CO2 fixed by Rubisco in the Calvin cycle is the final electron acceptor in photosynthetic electron flow (Baroli and Melis, 1998). More Ci was available in CAC1 due to its constitutive CCM expression (Figure 4B); harmful excess electrons may have been consumed by the Calvin cycle in CAC1 and could not generate excess ROS and cause photodamage. Furthermore, the bicarbonate effect observed may assist electron transfer to PSII by a light-induced primary charge separation and subsequent water oxidation (Wydrzynski and Satoh, 2005; Shevela et al., 2012); this would be achieved by increased consumption of bicarbonate in the thylakoid lumen of either the CCM-activated-CAC1 cell or the bicarbonate-supplied WT cell in HL.

Carbon concentrating mechanism in most algae and cyanobacteria is down regulated in a high inorganic or organic carbon environment (Moroney et al., 1987; Fett and Coleman, 1994; Iglesias-Rodriguez and Merrett, 1997; Wang et al., 2011). In the present study, cells were cultured with acetate containing TAP medium as an organic carbon source. Thus, CCM in the WT cells may be largely down regulated due to high carbon environment created by acetate. Contrary to this expectation, the expression of many CCM genes, particularly HLA3, CCP430, LCI420, LCI520, LCI450, LCI70, CAH920, CAH1510, CAH230, CAH0010, and CAH200, was increased in the WT when bicarbonate was included in the medium even in the presence of acetate (Figure 3). These results suggest that a different bicarbonate-sensing machinery is present with Ci signaling pathway in this alga Chlorella sp. ArM0029B and/or the bicarbonate-driven-Ci signal inside or outside of cell may bypass the Ci concentration recognition system (sensor) under high organic carbon environment (Figure 8). Insensitivity of CCM gene expression in the WT in response to high CO2 (Supplementary Figure S3) favors the presence of two independent carbon sensors (Figure 8). Similarly, the cyanobacterium Synechococcus PCC7942 cells grown in a high Ci environment readily took up CO2 but not HCO3– (Price and Badger, 1989). Contrary to WT cells, CAC1 cells exhibited constitutive expression of CCM genes even in the presence of organic carbon source. Insensitivity of ROS production in CAC1 against exogenous bicarbonate supply under HL conditions implicates the involvement of ROS signaling cascade in CCM expression. Thus, further molecular genetic studies will reveal possible different machineries sensing bicarbonate or CO2 and signaling to and role of relation to ROS signaling to CCM expression.

FIGURE 8.

FIGURE 8

Open in a new tab

A proposed model for dual Ci signaling pathways in Chlorella sp. ArM0029B. In Chlorella sp. ArM0029B, expression of CCM genes is suppressed by high concentration of intracellular Ci mostly derived from the acetate assimilatory pathway. Under this photoheterotrophic growth conditions, bicarbonate sensing and signaling pathway (blue line) are not operating. When high concentration of HCO3– is exogenously provided, this bicarbonate pathway becomes active. Constitutive operation of CCM machinery observed in CAC1 mutant implicates that CAC1 suppresses Ci signaling pathway to the CCM genes (red line). Failure of high exogenous CO2 in CCM activation implicates the presence of membranous CO2 transporter that allows CO2 entry fast enough not to be hydrated by external CAHs. Thus, dual signaling pathways for external bicarbonate and internal Ci to the CCM apparatus are probably present in Chlorella sp. ArM0029B. CAH, carbonic anhydrase; Ci, inorganic carbon; LCI, low CO2 inducible protein.

It is concluded that CAC1 constitutively operates its CCM, which causes high levels of Ci to accumulate in its cells. Based on these results, it is proposed that operation of the CCM acts as an electron sink for the electrons generated by photosynthesis: activation of the CCM provides more CO2 for fixation by Rubisco, which enhances Calvin cycle activity. It would follow, then, that constitutive operation of CCM endows Chlorella cells with resistance to HL partly by lowering endogenous generation of ROS. Present study will provide useful information on the interaction between CCM expression, ROS production, and photodamage in Chlorella and related microalgae.

Author Contributions

W-JJ designed the experiments and wrote the manuscript. KH, J-ML, S-WJ, and JV performed the experiments. Y-IP analyzed the data and commented on the manuscript. All authors contributed to writing the manuscript.

Conflict of Interest Statement

The authors declare that the research was conducted in the absence of any commercial or financial relationships that could be construed as a potential conflict of interest.

Footnotes

Funding. This work was supported by a grant from the Advanced Biomass R&D Center (ABC) of Global Frontier Project funded by the Ministry of Science and ICT (ABC-2011-0031343) and a grant from the Golden Seed Project, Ministry of Agriculture, Food, and Rural Affairs (MAFRA) and Rural Development Administration (RDA) (213008-05-2-SB820).

Supplementary Material

The Supplementary Material for this article can be found online at: https://www.frontiersin.org/articles/10.3389/fpls.2018.00590/full#supplementary-material

FIGURE S1

Light response curve of photosynthetic O2 evolution of wild-type (WT) and CAC1 mutant grown under photosynthesis limiting low light (LL, 50–80 μmol m-2 s-1) and saturating, high light (HL, 650–800 μmol m-2 s-1) intensities for 3 days. Data are means ± SE (n = 3).

Click here for additional data file. (53.3KB, JPEG)
FIGURE S2

Transcript levels of CCM genes in WT and CAC1 mutant grown under photosynthesis limiting LL (50–80 μmol m-2 s-1) and saturating, HL (650–800 μmol m-2 s-1) intensities for 3 days. MB, methylene blue staining.

Click here for additional data file. (97.3KB, JPEG)
FIGURE S3

Transcripts analyses of CCM genes WT and CAC1 mutant grown in air (low CO2) and high CO2 (2%) limiting LL (50–80 μmol m-2 s-1) for 3 days. The RT-PCR bands were quantified and shown as relative abundance normalized to the WT expression level, which is considered as 1.0.

Click here for additional data file. (64KB, JPEG)
FIGURE S4

Growth of WT and CAC1 mutant supplemented with Ci sources under limiting LL (50–80 μmol m-2 s-1) and intermediate light (IL, 350–400 μmol m-2 s-1) conditions for 4 days. Ci was supplied as 2% CO2 or 10 mM NaHCO3.

Click here for additional data file. (59.6KB, JPEG)
FIGURE S5

PsbA content as assessed by Western blotting in WT and CAC1 mutant grown under saturating, HL intensity (650–800 μmol m-2 s-1) with (+) or without (-) 10 mM bicarbonate supplementation for 3 days. PS, Ponceau S-staining. The Western blot bands were quantified and shown as relative abundance normalized to D1 (PsbA) accumulation level in the WT, which is considered as 1.0.

Click here for additional data file. (45.5KB, JPEG)
TABLE S1

Sequence of the primers used in this study.

Click here for additional data file. (14.6KB, DOCX)

References

  1. Ahn J. W., Hwangbo K., Lee S. Y., Choi H. G., Park Y. I., Liu J. R., et al. (2012). A new Arctic Chlorella species for biodiesel production. 125 340–343. 10.1016/j.biortech.2012.09.026 [DOI] [PubMed] [Google Scholar]
  2. Aro E. M., Virgin I., Andersson B. (1993). Photoinhibition of Photosystem II. Inactivation, protein damage and turnover. 1143 113–134. 10.1016/0005-2728(93)90134-2 [DOI] [PubMed] [Google Scholar]
  3. Baroli I., Melis A. (1998). Photoinhibitory damage is modulated by the rate of photosynthesis and by the photosystem II light-harvesting chlorophyll antenna size. 205 288–296. 10.1007/s004250050323 [DOI] [PubMed] [Google Scholar]
  4. Bechtold U., Richard O., Zamboni A., Gapper C., Geisler M., Pogson B. J., et al. (2008). Impact of chloroplastic- and extracellular-sourced ROS on high light-responsive gene expression in Arabidopsis. 59 121–133. 10.1093/jxb/erm289 [DOI] [PubMed] [Google Scholar]
  5. Brueggeman A. J., Gangadharaiah D. S., Cserhati M. F., Casero D., Weeks D. P., Ladunga I. (2012). Activation of the carbon concentrating mechanism by CO2 deprivation coincides with massive transcriptional restructuring in Chlamydomonas reinhardtii. 24 1860–1875. 10.1105/tpc.111.093435 [DOI] [PMC free article] [PubMed] [Google Scholar]
  6. Emanuelsson O., Brunak S., Von Heijne G., Nielsen H. (2007). Locating proteins in the cell using TargetP, SignalP and related tools. 2 953–971. 10.1038/nprot.2007.131 [DOI] [PubMed] [Google Scholar]
  7. Emanuelsson O., Nielsen H., von Heijne G. (1999). ChloroP, a neural network-based method for predicting chloroplast transit peptides and their cleavage sites. 8 978–984. 10.1110/ps.8.5.978 [DOI] [PMC free article] [PubMed] [Google Scholar]
  8. Fett J. P., Coleman J. R. (1994). Regulation of periplasmic carbonic anhydrase expression in Chlamydomonas reinhardtii by acetate and pH. 106 103–108. 10.1104/pp.106.1.103 [DOI] [PMC free article] [PubMed] [Google Scholar]
  9. Fischer B., Wiesendanger M., Eggen R. (2006). Growth condition-dependent sensitivity, photodamage and stress response of Chlamydomonas reinhardtii exposed to high light conditions. 47 1135–1145. 10.1093/pcp/pcj085 [DOI] [PubMed] [Google Scholar]
  10. Foyer C. H., Shigeoka S. (2011). Understanding oxidative stress and antioxidant functions to enhance photosynthesis. 155 93–100. 10.1104/pp.110.166181 [DOI] [PMC free article] [PubMed] [Google Scholar]
  11. Giordano M., Beardall J., Raven J. A. (2005). CO2 concentrating mechanisms in algae: mechanisms, environmental modulation, and evolution. 56 99–131. 10.1146/annurev.arplant.56.032604.144052 [DOI] [PubMed] [Google Scholar]
  12. Halliwell B., Gutteridge J. M. C. (1999). Oxford: New York. [Google Scholar]
  13. Harris E. (1989). Amsterdam: Elsevier. [Google Scholar]
  14. Heydarizadeh P., Boureba W., Zahedi M., Huang B., Moreau B., Lukomska E., et al. (2017). Response of CO2-starved diatom Phaeodactylum tricornutum to light intensity transition. 372:20160396. 10.1098/rstb.2016.0396 [DOI] [PMC free article] [PubMed] [Google Scholar]
  15. Hihara Y., Kamei A., Kanehisa M., Kaplan A., Ikeuchi M. (2001). DNA microarray analysis of cyanobacterial gene expression during acclimation to high light. 13 793–806. 10.1105/tpc.13.4.793 [DOI] [PMC free article] [PubMed] [Google Scholar]
  16. Huang L., Mccluskey M. P., Ni H., Larossa R. A. (2002). Global gene expression profiles of the cyanobacterium Synechocystis sp. strain PCC 6803 in response to irradiation with UV-B and white light. 184 6845–6858. 10.1128/JB.184.24.6845-6858.2002 [DOI] [PMC free article] [PubMed] [Google Scholar]
  17. Iglesias-Rodriguez M. D., Merrett M. J. (1997). Dissolved inorganic carbon utilization and the development of extracellular carbonic anhydrase by the marine diatom Phaeodactylum tricornutum. 135 163–168. 10.1046/j.1469-8137.1997.00625.x [DOI] [PubMed] [Google Scholar]
  18. Im C. S., Grossman A. R. (2002). Identification and regulation of high light-induced genes in Chlamydomonas reinhardtii. 30 301–313. 10.1046/j.1365-313X.2001.01287.x [DOI] [PubMed] [Google Scholar]
  19. Kitajima M., Butler W. L. (1975). Quenching of chlorophyll fluorescence and primary photochemistry in chloroplasts by dibromothymoquinone. 376 105–115. 10.1016/0005-2728(75)90209-1 [DOI] [PubMed] [Google Scholar]
  20. Kozaki A., Takeba G. (1996). Photorespiration protects C3 plants from photooxidation. 384 557–560. 10.1038/384557a0 [DOI] [Google Scholar]
  21. Krogh A., Larsson B., von Heijne G., Sonnhammer E. L. (2001). Predicting transmembrane protein topology with a hidden Markov model: application to complete genomes. 305 567–580. 10.1006/jmbi.2000.4315 [DOI] [PubMed] [Google Scholar]
  22. Laemmli U. K. (1970). Cleavage of structural proteins during the assembly of the head of bacteriophage T4. 227 680–685. 10.1038/227680a0 [DOI] [PubMed] [Google Scholar]
  23. Lemoine Y., Schoefs B. (2010). Secondary ketocarotenoid astaxanthin biosynthesis in algae: a multifunctional response to stress. 106 155–177. 10.1007/s11120-010-9583-3 [DOI] [PubMed] [Google Scholar]
  24. Lesser M. P. (2006). Oxidative stress in marine environments: biochemistry and physiological ecology. 68 253–278. 10.1146/annurev.physiol.68.040104.110001 [DOI] [PubMed] [Google Scholar]
  25. Letunic I., Doerks T., Bork P. (2014). SMART: recent updates, new developments and status in 2015. 43 D257–D260. 10.1093/nar/gku949 [DOI] [PMC free article] [PubMed] [Google Scholar]
  26. McGinn P. J., Price G. D., Maleszka R., Badger M. R. (2003). Inorganic carbon limitation and light control the expression of transcripts related to the CO2-concentrating mechanism in the cyanobacterium Synechocystis sp. strain PCC6803. 132 218–229. 10.1104/pp.019349 [DOI] [PMC free article] [PubMed] [Google Scholar]
  27. Melis A. (1991). Dynamics of photosynthetic membrane composition and function. 1058 87–106. 10.1016/S0005-2728(05)80225-7 [DOI] [Google Scholar]
  28. Minko I., Holloway S. P., Nikaido S., Carter M., Odom O. W., Johnson C. H., et al. (1999). Renilla luciferase as a vital reporter for chloroplast gene expression in Chlamydomonas. 262 421–425. 10.1007/s004380051101 [DOI] [PubMed] [Google Scholar]
  29. Moroney J. V., Kitayama M., Togasaki R. K., Tolbert N. E. (1987). Evidence for inorganic carbon transport by intact chloroplasts of Chlamydomonas reinhardtii. 83 460–463. 10.1104/pp.83.3.460 [DOI] [PMC free article] [PubMed] [Google Scholar]
  30. Muller P., Li X. P., Niyogi K. K. (2001). Non-photochemical quenching. A response to excess light energy. 125 1558–1566. 10.1104/pp.125.4.1558 [DOI] [PMC free article] [PubMed] [Google Scholar]
  31. Murata N., Takahashi S., Nishiyama Y., Allakhverdiev S. I. (2007). Photoinhibition of photosystem II under environmental stress. 1767 414–421. 10.1016/j.bbabio.2006.11.019 [DOI] [PubMed] [Google Scholar]
  32. Nishiyama Y., Allakhverdiev S. I., Yamamoto H., Hayashi H., Murata N. (2004). Singlet oxygen inhibits the repair of photosystem II by suppressing the translation elongation of the D1 protein in Synechocystis sp. PCC 6803. 43 11321–11330. 10.1021/bi036178q [DOI] [PubMed] [Google Scholar]
  33. Ohad I., Kyle D. J., Arntzen C. J. (1984). Membrane protein damage and repair: removal and replacement of inactivated 32-kilodalton polypeptides in chloroplast membranes. 99 481–485. 10.1083/jcb.99.2.481 [DOI] [PMC free article] [PubMed] [Google Scholar]
  34. Park Y. I., Karlsson J., Rojdestvenski I., Pronina N., Klimov V., Oquist G., et al. (1999). Role of a novel photosystem II-associated carbonic anhydrase in photosynthetic carbon assimilation in Chlamydomonas reinhardtii. 444 102–105. 10.1016/S0014-5793(99)00037-X [DOI] [PubMed] [Google Scholar]
  35. Peng L., Zhang Z., Lan C. Q., Basak A., Bond N., Ding X., et al. (2017). Alleviation of oxygen stress on Neochloris oleoabundans: effects of bicarbonate and pH. 29 143–152. 10.1007/s10811-016-0931-3 [DOI] [Google Scholar]
  36. Porra R. J., Thompson W. A., Kriedemann P. E. (1989). Determination of accurate extinction coefficients and simultaneous equations for assaying chlorophylls a and b extracted with four different solvents: verification of the concentration of chlorophyll standards by atomic absorption spectroscopy. 975 384–394. 10.1016/S0005-2728(89)80347-0 [DOI] [Google Scholar]
  37. Price G. D., Badger M. R. (1989). Ethoxyzolamide inhibition of CO(2) uptake in the cyanobacterium Synechococcus PCC7942 without apparent inhibition of internal carbonic anhydrase activity. 89 37–43. 10.1104/pp.89.1.37 [DOI] [PMC free article] [PubMed] [Google Scholar]
  38. Roberty S., Bailleul B., Berne N., Franck F., Cardol P. (2014). PSI Mehler reaction is the main alternative photosynthetic electron pathway in Symbiodinium sp., symbiotic dinoflagellates of cnidarians. 204 81–91. 10.1111/nph.12903 [DOI] [PubMed] [Google Scholar]
  39. Shevela D., Eaton-Rye J. J., Shen J. R., Govindjee (2012). Photosystem II and the unique role of bicarbonate: a historical perspective. 1817 1134–1151. 10.1016/j.bbabio.2012.04.003 [DOI] [PubMed] [Google Scholar]
  40. Smith B. M., Morrissey P. J., Guenther J. E., Nemson J. A., Harrison M. A., Allen J. F., et al. (1990). Response of the photosynthetic apparatus in Dunaliella salina (green algae) to irradiance stress. 93 1433–1440. 10.1104/pp.93.4.1433 [DOI] [PMC free article] [PubMed] [Google Scholar]
  41. Vass I. (2011). Role of charge recombination processes in photodamage and photoprotection of the photosystem II complex. 142 6–16. 10.1111/j.1399-3054.2011.01454.x [DOI] [PubMed] [Google Scholar]
  42. Vass I., Cser K. (2009). Janus-faced charge recombinations in photosystem II photoinhibition. 14 200–205. 10.1016/j.tplants.2009.01.009 [DOI] [PubMed] [Google Scholar]
  43. Wang Y., Duanmu D., Spalding M. H. (2011). Carbon dioxide concentrating mechanism in Chlamydomonas reinhardtii: inorganic carbon transport and CO2 recapture. 109 115–122. 10.1007/s11120-011-9643-3 [DOI] [PubMed] [Google Scholar]
  44. Wang Y., Stessman D. J., Spalding M. H. (2015). The CO2 concentrating mechanism and photosynthetic carbon assimilation in limiting CO2: how Chlamydomonas works against the gradient. 82 429–448. 10.1111/tpj.12829 [DOI] [PubMed] [Google Scholar]
  45. Wilbur K. M., Anderson N. G. (1948). Electrometric and colorimetric determination of carbonic anhydrase. 176 147–154. [PubMed] [Google Scholar]
  46. Woodger F. J., Badger M. R., Price G. D. (2003). Inorganic carbon limitation induces transcripts encoding components of the CO(2)-concentrating mechanism in Synechococcus sp. PCC7942 through a redox-independent pathway. 133 2069–2080. 10.1104/pp.103.029728 [DOI] [PMC free article] [PubMed] [Google Scholar]
  47. Wydrzynski T. J., Satoh K. (2005). Photosystem II: the light-driven water:plastoquinone oxidoreductase. 22 1–796. 10.1007/1-4020-4254-X [DOI] [Google Scholar]

Associated Data

This section collects any data citations, data availability statements, or supplementary materials included in this article.

Supplementary Materials

FIGURE S1

Light response curve of photosynthetic O2 evolution of wild-type (WT) and CAC1 mutant grown under photosynthesis limiting low light (LL, 50–80 μmol m-2 s-1) and saturating, high light (HL, 650–800 μmol m-2 s-1) intensities for 3 days. Data are means ± SE (n = 3).

Click here for additional data file. (53.3KB, JPEG)
FIGURE S2

Transcript levels of CCM genes in WT and CAC1 mutant grown under photosynthesis limiting LL (50–80 μmol m-2 s-1) and saturating, HL (650–800 μmol m-2 s-1) intensities for 3 days. MB, methylene blue staining.

Click here for additional data file. (97.3KB, JPEG)
FIGURE S3

Transcripts analyses of CCM genes WT and CAC1 mutant grown in air (low CO2) and high CO2 (2%) limiting LL (50–80 μmol m-2 s-1) for 3 days. The RT-PCR bands were quantified and shown as relative abundance normalized to the WT expression level, which is considered as 1.0.

Click here for additional data file. (64KB, JPEG)
FIGURE S4

Growth of WT and CAC1 mutant supplemented with Ci sources under limiting LL (50–80 μmol m-2 s-1) and intermediate light (IL, 350–400 μmol m-2 s-1) conditions for 4 days. Ci was supplied as 2% CO2 or 10 mM NaHCO3.

Click here for additional data file. (59.6KB, JPEG)
FIGURE S5

PsbA content as assessed by Western blotting in WT and CAC1 mutant grown under saturating, HL intensity (650–800 μmol m-2 s-1) with (+) or without (-) 10 mM bicarbonate supplementation for 3 days. PS, Ponceau S-staining. The Western blot bands were quantified and shown as relative abundance normalized to D1 (PsbA) accumulation level in the WT, which is considered as 1.0.

Click here for additional data file. (45.5KB, JPEG)
TABLE S1

Sequence of the primers used in this study.

Click here for additional data file. (14.6KB, DOCX)

Articles from Frontiers in Plant Science are provided here courtesy of Frontiers Media SA

RESOURCES