Transcriptome and key genes expression related to carbon fixation pathways in Chlorella PY-ZU1 cells and their growth under high concentrations of CO 2

Yun Huang; Jun Cheng; Hongxiang Lu; Yong He; Junhu Zhou; Kefa Cen

doi:10.1186/s13068-017-0868-z

Research
Open Access

Transcriptome and key genes expression related to carbon fixation pathways in Chlorella PY-ZU1 cells and their growth under high concentrations of CO₂

Yun Huang^{1, 2},
Jun Cheng¹Email author,
Hongxiang Lu¹,
Yong He¹,
Junhu Zhou¹ and
Kefa Cen¹

Biotechnology for Biofuels201710:181

https://doi.org/10.1186/s13068-017-0868-z

Received: 27 April 2017
Accepted: 5 July 2017
Published: 11 July 2017

Abstract

Background

The biomass yield of Chlorella PY-ZU1 drastically increased when cultivated under high CO₂ condition compared with that cultivated under air condition. However, less attention has been given to the microalgae photosynthetic mechanisms response to different CO₂ concentrations. The genetic reasons for the higher growth rate, CO₂ fixation rate, and photosynthetic efficiency of microalgal cells under higher CO₂ concentration have not been clearly defined yet.

Results

In this study, the Illumina sequencing and de novo transcriptome assembly of Chlorella PY-ZU1 cells cultivated under 15% CO₂ were performed and compared with those of cells grown under air. It was found that carbonic anhydrase (CAs, enzyme for interconversion of bicarbonate to CO₂) dramatically decreased to near 0 in 15% CO₂-grown cells, which indicated that CO₂ molecules directly permeated into cells under high CO₂ stress without CO₂-concentrating mechanism. Extrapolating from the growth conditions and quantitative Real-Time PCR of CCM-related genes, the K _m (CO₂) (the minimum intracellular CO₂ concentration that rubisco required) of Chlorella PY-ZU1 might be in the range of 80–192 μM. More adenosine triphosphates was saved for carbon fixation-related pathways. The transcript abundance of rubisco (the most important enzyme of CO₂ fixation reaction) was 16.3 times higher in 15% CO₂-grown cells than that under air. Besides, the transcript abundances of most key genes involved in carbon fixation pathways were also enhanced in 15% CO₂-grown cells.

Conclusions

Carbon fixation and nitrogen metabolism are the two most important metabolisms in the photosynthetic cells. These genes related to the two most metabolisms with significantly differential expressions were beneficial for microalgal growth (2.85 g L⁻¹) under 15% CO₂ concentration. Considering the micro and macro growth phenomena of Chlorella PY-ZU1 under different concentrations of CO₂ (0.04–60%), CO₂ transport pathways responses to different CO₂ (0.04–60%) concentrations was reconstructed.

Keywords

CO₂ fixation pathway
Genes transcript sequences
15% CO₂ concentration
Carbonic anhydrase
Rubisco

Background

Global warming necessitates the reduction of accumulated CO₂ in the atmosphere. Utilizing biological conversions by microalgae is a promising approach to reduce CO₂ emissions [1, 2]. However, the current atmospheric CO₂ concentration of ~0.04% is not enough for microalgae photosynthesis [3]. Moreover, the photosynthetic mechanism ribulose-1,5-bisphosphate carboxylase/oxygenase (rubisco), the first and stromal enzyme that catalyzes the entry of CO₂ into the Calvin–Benson cycle, is adapted to the considerably higher CO₂ concentrations encountered by C₃ plants [4]. The K _m for CO₂ of microalgal rubisco, often exceed 25 μM [5]. However, the dissolved CO₂ in freshwater is only ~15 μM when in equilibrium with air. However, rubisco has a poor apparent affinity with CO₂ when the dissolved CO₂ concentration is less than the K _m (CO₂) of rubisco, led to decrease in photosynthetic efficiency [6, 7]. To overcome this challenge, a number of prokaryotic and eukaryotic microalgae have developed a CO₂-concentrating mechanism (CCM) to maximize photosynthesis under limited CO₂ conditions [8]. Given that CO₂ is the only form of dissolved inorganic carbon that rubisco can fix, the most likely evolutionary goal of the CCM process is to increase dissolved CO₂ concentrations at rubisco locations for fixation [9].

A number of studies have been conducted on the mechanisms underlying the acclimation of microalgal cells to limited CO₂ concentrations [7, 8, 10]. Carbonic anhydrase (CAs) and CCM play an important role in the efficient utilization of dissolved inorganic carbon under CO₂-limited conditions. However, CCM requires more energy flow in PSI and leaves less energy available for the Calvin–Benson cycle, thus reducing microalgal growth and CO₂ fixation efficiency [11]. Therefore, several studies have focused on CO₂ fixation by microalgae from high concentrations of CO₂ gas, such as flue gas, to increase CO₂ fixation efficiency [12]. In our previous study, the biomass yield (2.78 g L⁻¹) of Chlorella PY-ZU1 cultivated under 15% CO₂ increased by 1.19-fold compared with that of microalgae cultivated under air (1.30 g L⁻¹) [13]. However, less attention has been given to the photosynthetic mechanisms of microalgal response to different CO₂ concentrations. And, the genetic reasons for the higher growth rate, CO₂ fixation rate, and photosynthetic efficiency of domesticated microalgae cells under higher CO₂ concentration remain unclear.

Nevertheless, CCM models have clearly shown that CCM will work when microalgae cells are exposed to limited CO₂ conditions [14]. There is still a lack of research on the exact conditions, including CO₂ conditions and K _m (CO₂), and under which condition CCM would switch on. Moreover, the relationship between the diversity and evolutionary pathways of key carbon fixation-related genes and photosynthetic performance is still unknown because of their dependency on microalgae species [15]. Therefore, in the present study, we analyzed the transcriptome and gene expression of Chlorella PY-ZU1 cells cultivated under different CO₂ concentrations and reconstructed the CO₂ transport pathways into Chlorella PY-ZU1 responses to different CO₂ concentrations. The growth conditions of Chlorella PY-ZU1 and DIC in the medium were also measured to extrapolate the value of K _m (CO₂).

Methods

Strains and media

This strain used in the present study was Chlorella PY-ZU1, a highly CO₂-tolerant and fast-growing microalgal species that obtained from Chlorella pyrenoidosa after γ irradiation and high CO₂ domestication [6]. The cells were maintained and cultivated in Brostol’s solution (also known as soil extract, SE) [1, 6].

Analysis of differentially expressed Chlorella PY-ZU1 genes under continuous aeration with 15% CO₂ and air

Chlorella PY-ZU1 strains were cultivated in SE medium under 15% CO₂ or air. Cells in the logarithmic phase (after cultivated 36 h) were collected by centrifugation for DNA extraction. The gene for full-length 18s rDNA was amplified to obtain the algal genome according to the protocol performed in Cheng’s study [16]. The following primers were utilized to amplify 18s rDNA: 18s-F, AACCTGGTTGATCCTGCCAGT and 18s-R, TGATCCTTCTGCAGGTTCACCT. The gene was inserted into the cloning vector, pMD19-T. Positive results were selected for sequencing. Total RNA was extracted by TRIzol reagent (Invitrogen) for cDNA library construction and Illumina sequencing. mRNA was separated by magnetic sand method, cleaved to synthesize double-stranded cDNA, and filled to plane. Poly (A) was added at the 3ʹ terminal end, and index connection was linked using TruSeq™ RNA Sample Preparation Kit. The target strip was enriched using polymerase chain reaction (PCR; 15 cycles) and recycled by 2% agarose gel. Quantitative determination was performed by TBS380 (Picogreen). Bridge amplification was conducted to generate cBot clusters. The 2*100 bp sequencing test was performed by HiSeq 2000 sequencing platform. Sequence assembly and annotation were similar to those performed in Cheng’s study [16].

Gene expression statistics and differential expression analysis

Total RNA extracted from algae grown in normal medium (under Air) and high-CO₂ medium [15% (v/v) CO₂] was used to prepare gene expression libraries using the Illumina Gene Expression Sample Prep Kit and then subjected to Illumina sequencing. The RNA-Seq reads were mapped to our transcriptome reference database, and transcript abundances were quantified by RSEM (http://deweylab.biostat.wisc.edu/rsem/). Genes with differential expression between these two samples were identified using the numbers of mapped reads as EdgeR inputs (http://www.bioconductor.org/packages/release/bioc/html/edgeR.html). Genes were defined as differentially expressed if they exhibited a 2-fold or greater change between the air and high-CO₂ samples and a false discovery rate (FDR) of 5% or less. Differentially expressed genes were regarded as up-regulated if their expression levels in high-CO₂ samples were significantly higher than those in air samples. Conversely, genes that showed lower expression levels in the high-CO₂ samples were regarded as down-regulated. Gene set enrichment analyses were performed using goatools (https://github.com/tanghaibao/goatools) and KOBAS (http://kobas.cbi.pku.edu.cn/home.do).

Quantitative real-time PCR (qRT-PCR) validation

To investigate the developmental expression patterns of rubisco, CAs, and nitrate reductase, samples of microalgae cells cultivated for different durations under 15% CO₂ or air were collected. Real-time reverse transcript polymerase chain reaction (real-time PCR, RT-PCR) was conducted with gene-specific primers pairs designed by PRIMER PREMIER5 software. The sequences of the specific primer sets are listed in Table 1. Total RNAwas extracted. qRT-PCR was performed with 20-μL reaction volumes containing 2 μL of 10-fold diluted cDNAs, 1 μM of each primer, and 10 μL SYBR Green Premix Ex Taq by the Bio-Rad Real-time PCR system (Bio-Rad, Hercules, CA, USA). The housekeeping gene for 18S ribosome DNA was used as a control. The 18 rDNA gene primers were as follows: algae sense 5′-ACGGCTACCACATCCAAG-3′ and antisense 5′-CCACCCGAAATCCAACTA-3′. The optimized qPCR program consisted of an initial denaturation step at 95 °C for 30 s, followed by 40 cycles at 95 °C for 5 s, and 60 °C for 30 s. qPCR was repeated thrice per gene. Each replication was performed with an independently prepared RNA sample and consisted of three technical replicates . A relative quantitative method (ΔΔCt) was used to evaluate the quantitative variation [17].

Table 1

Sequences of specific primers used for real-time PCR

Gene	EC no.	Sense	Antisense
Rubisco	4.1.1.39	CTCCACCCGCTCCGTCTAAG	GACAAACTCGTGCGACATTCTT
Nitrate reductase	1.7.1.1	GGGATGGGCGACCTTGAT	GCCTCCCGAACCTTGAGAA
CA	4.2.1.1	TGTGAGCGGACAGCAACCA	GGGACGAAGAGGAGAAGAGGG

Cultivation of microalgae under continuous aeration with different concentrations of CO₂

All Chlorella PY-ZU1 cultivation experiments were performed in an artificial greenhouse at 27 °C. Initial biomass concentration was maintained at 0.2 g L⁻¹. Microalgae were cultivated in the cylindrical photoreactors (BR) (160 × Ф56 mm; 300-mL working volume) with the optimized SE medium (SE* medium). SE* medium contained 1 g of NaNO₃, 0.15 g of K₂HPO₄·3H₂O, 0.15 g of MgSO₄·7H₂O, 0.025 g of CaCl₂·2H₂O, 0.025 g of NaCl, 40 mL of soil extract, 0.005 g of FeCl₃·6H₂O, 1 mL of Fe-EDTA, and 1 mL of A5 solution in 958 mL of deionized water [1]. Enriched CO₂ gas [from 384 ppm to 60% (v/v)] was bubbled into the BR via a pipe at a rate of 30 mL min⁻¹. Initial pH was adjusted to 6.5 by using 0.1 M HCl and 0.1 M NaOH. During incubation, light intensity of 6000 Lux was applied on the surface of the BR with four cool white lights and two plant lights (TLD 36 W; Philips) fixed above the BR.

To obtain the dry biomass during cultivation, 10-mL samples were dewatered by centrifugation (Beckman Avanti J26-XP, USA) at 8500 rpm for 10 min and dried at 70 °C for 24 h. Biomass yield (g L⁻¹) was calculated from the microalgae dry weight produced per liter. Chlorophyll was extracted by macerating microalgae in DMSO/80% acetone (1/2, V/V) and then measured [18]. NO₃ ⁻ concentrations were analyzed by ion chromatography (MagIC, Metrohm, Switzerland). All experiments were performed in duplicate, and all data showed were reported as mean values and standard deviations (in figures) or standard errors (in tables) in this study.

Calculation of dissolved CO₂ concentration

Dissolved inorganic carbon (DIC) and CO₂ in the culture were calculated according to the CO₂ dissolved process [17] as follows:

$${\text{CO}}_{2} \,({\text{g}}) + {\text{H}}_{2} {\text{O}} \leftrightarrow {\text{H}}_{2} {\text{CO}}_{3} \,({\text{g}})\quad K_{\text{H}} = \frac{{\left[ {{\text{H}}_{2} {\text{CO}}_{3} } \right]}}{{{\text{P}}_{{{\text{CO}}_{2} }} }}$$

$${\text{H}}_{2} {\text{CO}}_{3} ({\text{g}}) \leftrightarrow {\text{H}}^{ + } + {\text{HCO}}_{3}^{ - } ({\text{g}})\quad K_{\text{a1}} = \frac{{[{\text{H}}^{ + } ][{\text{HCO}}_{3}^{ - } ]}}{{\left[ {{\text{H}}_{2} {\text{CO}}_{3} } \right]}}.$$

During cultivation, the culture pH was 5.5–7.0, thus,

$$[{\text{DIC}}] = [{\text{H}}_{2} {\text{CO}}_{3} ] + [{\text{HCO}}_{3}^{ - } ] = K_{\text{H}} \times P_{{{\text{CO}}_{2} }} \times \left( {1 + \frac{{K_{\text{a1}} }}{{{\text{H}}^{ + } }}} \right)$$

$$[{\text{CO}}_{2} ] = K_{\text{H}} \times P_{{{\text{CO}}_{2} }} .$$

(1)

The influent and effluent CO₂ concentrations were monitored online by a CO₂ analyzer (Servomex4100, UK). At a constant temperature of 27 °C, K _H = 3.2 × 10⁻² M atm⁻¹ and K _a1 = 4.3 × 10⁻⁷ M [19]. [H⁺] = 10^−pH, $P_{{{\text{CO}}_{ 2} }} = {\text{mean }}\left( {P_{{{\text{CO}}_{ 2} {\text{input}}}} , \, P_{{{\text{CO}}_{ 2} {\text{output}}}} } \right).$

Reconstruction of inorganic carbon transport pathways

The microstructure of Chlorella PY-ZU1 was also measured by TEM in our previous study [20]. An apparent protein body (pyrenoid) was found inside the chloroplast in Chlorella PY-ZU1 from the image. The microstructure of Chlorella PY-ZU1 used in this work were compared with that of the green microalgae Chlorophyta, one species with the same genus of Chlorella PY-ZU1. In the Chlorophyta a pyrenoid is localized inside the chloroplast, starch often is accumulated around the pyrenoid and the presence of concentric thylakoid systems is visible around this starch sheath [21]. CCM goes on the pyrenoid model, and CA is in the pyrenoid that localized in chloroplast [22]. CCM goes on passive diffusion of CO₂ through the plasmalemma and active bicarbonate transport into the chloroplast [8, 21]. Inorganic carbon transport pathways reconstructed based on de novo assembly and annotation of Chlorella PY-ZU1. The genes involved in these pathways in Chlorella PY-ZU1 were condensed and simplified according to their transcript abundances.

Results

Gene expression of carbonic anhydrase and rubisco under high CO₂ stress

Chlorella PY-ZU1 had a higher biomass yield (2.85 g L⁻¹) and shorter growth cycle (7 days) when cultivated in SE medium under continuous aeration with 15% (v/v) CO₂ gas. This CO₂ concentration is equivalent to that of flue gas from most coal-fired power plants. By contrast, the biomass concentration of Chlorella PY-ZU1 was only 1.30 g L⁻¹ after 10 days of cultivation under air. It was previously reported that high CO₂ induced algae growth [23]. Carbon fixation and nitrogen metabolism are the two most important aspects of primary cell metabolism. Therefore, we expected to observe significant differences in the expression of genes encoding enzymes of carbon fixation and nitrogen metabolism.

When aerated into the microalgal suspension, CO₂ first dissolves in the medium, and then transfers from the extracellular culture medium through the cell membrane to the intracellular chloroplast. Then, CO₂ is converted by ribulose-1,5-bisphosphate (RuBP) upon the catalysis of RuBP carboxylase (rubisco) to 3-phosphoglycerate (PGA), the precursor of structural materials in microalgal cells [24]. Rubisco (rbcS, EC4.1.1.39), the first enzyme of the Calvin cycle, fixes CO₂ into the three carbon atoms of RuBP (${\rm CO}_{2} + {\rm C}5\mathop{\longrightarrow}\limits^{{\rm Rubisco}}2{\rm C}3$). The transcript abundance of RuBP increased slightly from 11,043.90 to 11,478.37 under high CO₂ (15% CO₂), whereas it was highly expressed under both high (15% CO₂) and low (air) CO₂ (Fig. 2). A 2-fold increase in transcript abundance was observed for PGK (EC2.7.2.3), which catalyzes the phosphorylation of 3-PGA to 1,3-bisphosphoglycerate. Moreover, triose phosphate isomerase (tpiA, EC5.3.1.1), which reversibly converts GAP into dihydroxyacetone phosphate (DHAP), increased by approximately 10.4-fold. The transcript abundance of a series of enzymes that converts GAP to sedoheptulose-7-phosphate (S7P), such as fructose-1,6-bisphosphatase aldolase (fbaB, EC4.1.2.13), increased more than 2-fold, whereas those of transketolase (tkt, EC2.2.1.1) and sedoheptulose-1,7-bisphosphatase (SBPase, EC3.1.3.37) improved slightly. Ribose-5-phosphate isomerase (rpiA, EC5.3.1.6), which converts R5P into ribulose-5-phosphate (Ru5P), increased by 7.8-fold. Phosphoribulokinase (prkB, EC2.7.1.19), which phosphorylates Ru5P into RuBP, increased by 4.0-fold. Therefore, almost all of the enzymes involved in the Calvin cycle had increased transcript abundances (Additional file 1) under high CO₂. The results indicated that the whole carbon fixation process was driven by 15% CO₂ gas. Therefore, the growth rate of Chlorella PY-ZU1 increased under 15% CO₂ compared with under air (Fig. 1).

Fig. 1
Growth curves of *Chlorella PY*-*ZU1* cultivated under continuous aeration with 15% CO₂ gas versus air (CO₂ = 384 ppm)

Moreover, rubisco was still highly expressed even Chlorella PY-ZU1 was cultivated under limited CO₂, such as air. The high expression of rubisco was caused by CCM in microalgae cells. Rubisco is only activated when CO₂ concentration is greater than its K _m (CO₂), because that CO₂ is the only carbon source that rubisco can utilize. However, when aerated with air, 99% of carbon in the culture is in the form of HCO₃ ⁻ [1]. CO₂ concentration in the medium hardly meets the requirements of rubisco because of the low solubility of CO₂. Gene transcript abundance of CAs in Chlorella PY-ZU1 pyrenoids increased to 5190 from 39 under cultivation with 15% CO₂. CAs expression increased to maintain high CO₂ concentration in pyrenoids. Furthermore, CCM was simultaneously activated as most of the dissolved inorganic carbon, HCO₃ ⁻, was transferred by pump through the chloroplast membrane into the internal pyrenoid; HCO₃ was then converted by CAs to CO₂ as function (2) in the chloroplast to meet the needs of rubisco (Fig. 2) [25]. However, CCM occurred at the cost of ATP. Increased CCM expression consumed more energy for CO₂ transfer, thus decreasing the energy available for carbon fixation and other pathways of photosynthetic growth. Conversely, when cultivated under continuous aeration with 15% CO₂, CAs was barely expressed in Chlorella PY-ZU1 pyrenoids. CCM was inactive. The CO₂ that diffused directly into pyrenoids by high CO₂ osmotic pressure was sufficient for rubisco. Therefore CO₂ transfer pathway was simplified. Hence, more ATP was available for photosynthesis to promote growth.

Fig. 2
Genes transcript abundance of reconstructed carbon fixation pathway in *Chlorella PY-ZU1* cells cultivated with 15% CO₂ gas versus air. *Black dotted box* indicated CO₂ transfer process (CO₂ concentrating mechanism), and *red dotted box* indicated Calvin cycle. Key enzymes of Calvin cycle are shown in *boxes* as enzyme commission (EC) numbers. *Red box* indicated an up-regulation, and *black box* indicated no significant changes

$${\rm HCO}_{3}^{ - } + {\rm H}^{ + } \mathop{\longrightarrow}\limits^{{{\text{Carbonic anhydrase}}}}{\rm CO}_{2} +{\rm H}_{2} {\rm O}$$

(2)

CAs and rubisco are the most important genes of carbon fixation pathways. To confirm the transcriptome results, the expression levels of genes encoding CA and rubisco were measured by qRT-PCR under different cultivation times (Fig. 3a). Under high CO₂, the CAs transcript level was significantly reduced to 0 (The original data showed in Additional file 2), which is consistent with the transcriptome results (Fig. 2). Moreover, the study conducted by Fan et al. reported a similar, remarkably decreased CAs expression when oleaginous Chlorella cells were exposed to 5% CO₂ [26]. This result is also consistent with previous reports that CO₂ concentration significantly affects CAs activity in Chlorella pyrenoidosa cells, and that elevating CO₂ concentration decreases CAs activity [27].

Rubisco expression levels increased under high CO₂ (Fig. 3b). This result is consistent with the transcriptome results. Under 15% CO₂, the enhanced rubisco expression of Chlorella PY-ZU1 cells might induce more CO₂ to directly permeate intracellular pyrenoids for conversion into cellular energy storage molecules and to promote ATP conversion to glucose, thereby improving the photosynthetic efficiency of microalgae. Therefore, high CO₂ concentrations reduced the ATP consumption of CO₂ transfer. On the other hand, high CO₂ concentrations improved CO₂ conversion and photosynthetic efficiency, thus eventually reducing the growth cycle and increasing the biomass yield (2.85 g L⁻¹) of Chlorella PY-ZU1.

In addition, the time when rubisco had highest transcriptional level (24 h of high CO₂ and 48 h of air) and the time CAs had lowest transcriptional level under air (48 h) were also the time when maximum microalgae growth rate was achieved (24 h of high CO₂ and 48 h of air) (Fig. 1). That fully illustrated that CAs and rubisco had the ability to regulate microalgae growth.

Response of nitrogen metabolism and chlorophyll synthesis to high CO₂ stress

Similar to carbon fixation, the transcript abundance of important enzymes in nitrogen metabolism, including those of nitrate reductase, nitrite reductase and glutamate dehydrogenase (ghdA), also increased under high CO₂ (Fig. 4a). Nitrogen is an essential element for chlorophyll and protein synthesis. After nitrate reductase and nitrite reductase increased, nitrate ions absorbed by microalgae were immediately catalyzed to nitrite ions and then to ammonia through a series of reduction reactions to synthesize nitrogenous compounds, such as amino acids, which in turn increased the efficiency of nitrate ion uptake from the medium by microalgae cells. On the aspect of nitrogen source consumption (in this study, the nitrogen source was sodium nitrate), Chlorella PY-ZU1 consumed almost all of the 3 mM nitrate during the first 2 days, especially on the first day (Fig. 4b) when cultivated under continuous aeration with 15% CO₂. By contrast, Chlorella PY-ZU1 only consumed 1.26 mM nitrate during the first 2 days, and nitrate was not completely consumed until the sixth day when cultivated under air. On the genetic level, the transcript abundance of nitrate reductase, the first enzyme in nitrogen metabolism, increased by approximately 10-fold by the 24th h and 8-fold by the 48th h under high CO₂ compared with that under air (Fig. 4c). The higher transcript expression of nitrate reductase accelerated the transformation of nitrate to nitrite and O₂ catalyzed by nitrate reductase (Function 3). This higher gene expression might manifest by the rapid consumption of nitrate. Furthermore, by the catalysis of the up-regulated nitrite reductase, more nitrite was converted to amino acid synthesis precursors, such as ammonia (Function 4), thereby accelerating the synthesis of proteinaceous materials, such as chlorophyll (Fig. 4d).

Fig. 4
Genes transcript abundance of nitrogen metabolism pathway in cells (a), nitrate consumption (b), qRT-PCR of nitrate reductase (c) and chlorophyll synthesis (d) of *Chlorella* PY-ZU1 cultivated under 15% CO₂ versus air. Key enzymes of Calvin cycle were shown in *boxes* as enzyme commission (EC) numbers. *Red box* indicated an up-regulation, *blue box* indicated a down-regulation, and *black box* indicated no significant changes

$$2{\rm NO}_{3}^{ - } \mathop{\longrightarrow}\limits^{{\rm Nitrate}\,\, {\rm reductase}}2{\rm NO}_{2}^{ - } + {\rm O}_{2}$$

(3)

$${\rm NO}_{2}^{ - } + 6{\rm NADPH}\mathop{\longrightarrow}\limits^{{\rm Nitrite}\,\,{\rm reductase}}{\rm NH}_{4}^{ + } + 2{\rm OH}^{ - } + 6{\rm NADP}$$

(4)

Under 15% (v/v) CO₂, 23.65 mg L⁻¹ of chlorophyll was produced during the first day of cultivation. Chlorophyll concentration remained stable in the range of 23–26 mg L⁻¹. All of the 3 mM nitrate in the medium was consumed during the following 3 days (Fig. 4d). Chlorophyll was vital in photosynthesis and allowed Chlorella PY-ZU1 cells to absorb energy from light. Moreover, light conversion efficiency is linearly correlated with chlorophyll content [1, 28]. Increased chlorophyll provided more energy for photosynthetic reactions, thereby improving the photosynthetic growth rate of Chlorella PY-ZU1. However, the high nitrogen consumption during the first 3 days resulted in nitrogen deficiency in the following days under 15% CO₂. Microalgae consumed its chlorophyll to maintain cell growth under nitrogen deficiency from the 4th day, and the chlorophyll content of Chlorella PY-ZU1 decreased. By contrast, chlorophyll content of Chlorella PY-ZU1 still increased when cultivated under air. Given that chlorophyll synthesis is almost directly proportional to nitrate concentration in the culture medium, the chlorophyll contents of Chlorella PY-ZU1 were almost the same under different CO₂ conditions by the end of the cultivation period [1, 29]. However, during cultivation, the chlorophyll content of Chlorella PY-ZU1 cultivated under 15% CO₂ was always higher than that of under air, which resulted in higher microalgae growth rate (Fig. 1).

Analysis of different concentrations of CO₂ transport and fixation mechanisms

Figure 5 shows the biomass productivity of Chlorella PY-ZU1 cultivated in optimized SE medium under different CO₂ concentrations. Excessively low (<1%) and high (>30%) CO₂ concentration could restrain microalgae growth and resulted in lower biomass yield (<2 g L⁻¹). However, when cultivated under 1% CO₂, the biomass yield drastically increased by 130.2% to 3.73 g L⁻¹ compared with the 1.62 g L⁻¹ obtained by cultivation under 0.5% CO₂. The drastically increased biomass yield in response to higher CO₂ concentrations indicated some changes in the pathway of CO₂ transfer and utilization by microalgae. CCM will work when microalgae is cultivated under limited CO₂ conditions, such as air. However, it will not work if the CO₂ that directly diffused to pyrenoids by extra- and intracellular CO₂ osmotic pressure is sufficient for rubisco, more energy was concentrated for cell growth. Thus, biomass productivity was dramatically enhanced [11]. An external concentration of 0.5% CO₂ was too low for Chlorella PY-ZU1 because it could not supply enough CO₂ through osmosis to rubisco. However, 1% external CO₂ could overcome diffusion resistance to enable CO₂ flux from the external medium to the cytoplasm. Moreover, enough CO₂ diffusion by high CO₂ stress to the cytoplasm resulted in non-operational CCM. Therefore, >1% external CO₂ concentration maintained enough CO₂ in pyrenoids for rubisco only through direct diffusion, which is dependent on extra- and intra-cellular CO₂ osmotic pressure. When cultivated under 3–30% CO₂, Chlorella PY-ZU1 had stable, higher biomass yields of 4.60–4.78 g L⁻¹. Therefore, 3–15% was ideal CO₂ concentration for Chlorella PY-ZU1 growth. However, when CO₂ concentration exceeded 30%, excess CO₂ inhibited microalgal growth and sharply decreased biomass yield (1.89 g L⁻¹). Therefore, >30% external CO₂ is too high for Chlorella PY-ZU1 given the overly acidic culture after aeration with higher CO₂ concentrations [26, 27].

Fig. 5
Biomass yield of *Chlorella* PY-ZU1 cultivated with optimized SE medium under various concentrations of CO₂

Discussion

The CCM process has a specific CAs to catalyze the conversion of HCO₃ to CO₂ at the expense of ATP [26]. For optimal efficiency, the carboxysomal CAs activity needs to match, as closely as possible, the maximal rate of CO₂ fixation [4, 30] under limited CO₂ conditions. The dissolved CO₂ concentration increased from 6.14 μM to 4.60 mM as the aerated CO₂ concentration increased from 384 ppm (air) to 15% (Table 2). K _m (CO₂) of rubisco is the critical point in the activation of rubisco [15] and allows cells to initiate the CCM process [31]. Therefore, microalgal growth rate and biomass yield will increase significantly when the dissolved CO₂ concentration in the culture is higher than K _m (CO₂) of rubisco. The biomass yield of Chlorella PY-ZU1 cultivated under 1% CO₂ increased sharply by 130.2% to 3.73 g L⁻¹ compared with 1.62 g L⁻¹ obtained from cultivation with 0.5% CO₂. It is known that CCM is energy consumption process and K _m is the critical point in the activation of rubisco. On one hand, if the intracellular CO₂ concentration around rubisco is higher than K _m, CCM would not work. More energy would be saved for microalgae growth. This is to say we can estimate whether CCM works from the microalgae growth condition. On the other hand, the mixed CO₂ gas aerated into microalgae suspension as carbon source. The intracellular CO₂ should be balanced with the dissolved CO₂ in suspension without CCM after equilibrium of CO₂ gas dissolving. The microalgae growth rate has a significant increase when the dissolved CO₂ concentration in culture increased from 80 to 192 μM. It could be deduced CCM did not work under 192 μM of dissolved CO₂ concentration but might still work under 80 μM. Therefore, the K _m (CO₂) value of rubisco in Chlorella PY-ZU1 might be in the range of 80–192 μM, which corresponds to 1% aerated CO₂ concentration. These values are consistent with those of previous reports.

Table 2

pH and dissolved CO₂ concentration of Chlorella PY-ZU1 culture aerated with various concentrations of CO₂ gas

Aerated CO₂ conc. %	0.0384	0.5	1	3	6	15	30	60
pH	10.73 ± 0.15	9.86 ± 0.41	8.75 ± 0.10	7.88 ± 0.07	7.35 ± 0.05	6.96 ± 0.17	6.04 ± 0.58	5.63 ± 0.38
Dissolved CO₂ conc. (μM)	6.14 ± 0.04	80 ± 2.0	192 ± 1.8	800 ± 20	1600 ± 32	4600 ± 20	9400 ± 37	19,100 ± 56

Furthermore, we utilized de novo assembly and annotation to reconstruct the possible pathways in Chlorella PY-ZU1 cells for inorganic carbon transport to pyrenoids from the external medium in response to different aerated CO₂ concentrations based on the pyrenoid model [22]. When cultivated under limited CO₂, such as under air, the dissolved CO₂ concentration of 6.14 μM in the culture could not meet the CO₂ demands of rubisco. Therefore, Chlorella PY-ZU1 initiated CCM to localize CO₂ in pyrenoids. However, >1% CO₂ concentration supplied enough dissolved CO₂ (>192 μM). Thus, the cell did not initiate CCM. The free CO₂ molecules permeating to the pyrenoids were sufficient for direct use by rubisco. Increased CO₂ accumulation increased the cell’s photosynthetic efficiency, resulting in a higher biomass yield of 3.73 g L⁻¹. In addition, with the further increasing of CO₂ concentration to 30%, the dissolved CO₂ concentration increased to 9.4 mM. Although, the dissolved CO₂ also could meet the demands of rubisco. Excessive CO₂ could acidify the microalgae culture, resulting in cell “anesthesia” [32] and decreasing enzymatic activity [33, 34], which eventually drastically decreases Chlorella PY-ZU1 biomass yield. Therefore, <1% CO₂ was too limited for Chlorella PY-ZU1. As a result, CCM was initiated to concentrate CO₂. Therefore, 1–30% CO₂ concentration is very suitable for Chlorella PY-ZU1 growth, whereas >30% CO₂ is excessive for microalgae growth (Fig. 6).

Fig. 6
Reconstructed CO₂ transport schematic pathway of *Chlorella* PY-ZU1 under various concentrations of CO₂

Conclusions

The biomass yield of Chlorella PY-ZU1 cultivated under 0.5% CO₂ was only 1.62 g L⁻¹. However, when cultivated under 1% CO₂, the biomass yield drastically increased by 130.2% to 3.73 g L⁻¹. The drastically increased biomass yield in response to higher CO₂ concentration indicated some changes happened in CO₂ transfer and utilization by microalgae. CAs in Chlorella PY-ZU1 cells cultivated under 15% CO₂ barely expressed. That indicated CO₂ could directly permeate into intra-cell for rubisco to fix without CCM working at the expense of ATP. While CCM in cells that cultivated under <1% CO₂ conditions would work for CO₂ transport. Carbon fixation and nitrogen metabolisms are the two most important aspects of primary cell metabolisms. Besides the improved expression of enzymes in carbon fixation pathways, the enzymes in nitrogen metabolism pathways, including nitrate reductase, nitrite reductase and glutamate dehydrogenase, also had an increased expression level under 15% CO₂ condition. Further studies should be taken to determine CO₂ distribution and verify the exact K _m (CO₂) of rubisco in microalgae cells.

Abbreviations

CAs:: carbonic anhydrase

CCM:: CO₂ concentrating mechanism

K _m (CO₂):: concentration of CO₂ required for 50% of the maximum photosynthesis rate

Rubisco:: ribulose-1,5-bisphosphate carboxylase/oxygenase

RuBP:: ribulose-1,5-bisphosphate

3-PGA:: 3-phosphoglyceride

DHAP:: dihydroxyacetone phosphate

S7P:: sedoheptulose-7-phosphate

fbaB:: fructose-1,6-bisphosphatase aldolase

Ru5P:: ribulose-5-phosphate

SBPase:: sedoheptulose-1,7-bisphosphatase

Declarations

Authors’ contributions

YH and JC proposed the idea and hypothesis. YH carried out the experiment design and performed the Illumina sequencing and de novo transcriptome assembly and drafted the manuscript. HL and YH carried out the microalgae cultivation experiments. JC performed the statistical analysis. JZ and KC helped to draft and revise the manuscript. All authors read and approved the final manuscript.

Acknowledgements

This study is supported by National key research and development program-China (2016YFB0601001), National Natural Science Foundation—China (51476141).

Competing interests

The authors declare that they have no competing interests.

Availability of data and materials

The datasets supporting the conclusions of this article are included within the article.

Consent for publication

All authors have approved the manuscript for submission and confirm that the content of the manuscript has not been published, or submitted for publication elsewhere.

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Authors’ Affiliations

(1)

State Key Laboratory of Clean Energy Utilization, Zhejiang University, Hangzhou, 310027, China

(2)

Key Laboratory of Low-grade Energy Utilization Technologies and Systems of Ministry of Education, Chongqing University, Chongqing, 400044, China

References

Huang J, Yang Z, Guan F, Cui D, Guan G, Jiang W, Li Y. Improved production of a recombinant Rhizomucor miehei lipase expressed in Pichia pastoris and its application for conversion of microalgae oil to biodiesel. Biotechnol Biofuels. 2014;7:111–21.View ArticleGoogle Scholar
Chang H, Huang Y, Fu Q, Liao Q, Zhu X. Kinetic characteristics and modeling of microalgae Chlorella vulgaris growth and CO₂ biofixation considering the coupled effects of light intensity and dissolved inorganic carbon. Bioresour Technol. 2016;206:231–8.View ArticleGoogle Scholar
Larkum A. Limitations and prospects of natural photosynthesis for bioenergy production. Curr Opin Biotech. 2010;21:271–6.View ArticleGoogle Scholar
Kupriyanova E, Pronina N. Carbonic anhydrase: enzyme that has transformed the biosphere. Russ J Plant Physiol. 2011;58:197–209.View ArticleGoogle Scholar
Bhatti S, Colman B. Evidence for the occurrence of photorespiration in synurophyte algae. Photosynth Res. 2011;109:251–6.View ArticleGoogle Scholar
Cheng J, Huang Y, Feng J, Sun J, Zhou J, Cen KF. Mutate Chlorella sp. by nuclear irradiation to fix high concentrations of CO₂. Bioresour Technol. 2013;136:496–501.View ArticleGoogle Scholar
Satoh A, Kurano N, Miyachi S. Inhibition of photosynthesis by intracellular carbonic anhydrase in microalgae under excess concentrations of CO₂. Photosynth Res. 2001;68:215–24.View ArticleGoogle Scholar
Raven J, Giordano M, Beardall J, Maberly S. Algal evolution in relation to atmospheric CO₂: carboxylases, carbon-concentrating mechanisms and carbon oxidation cycles. Phil T R Soc B. 2012;367:493–507.View ArticleGoogle Scholar
Aizawa K, Miyachi S. Carbonic anhydrase and CO₂ concentrating mechanisms in microalgae and cyanobacteria. FEMS Microbiol Lett. 1986;39:215–33.View ArticleGoogle Scholar
Kupriyanova E, Samylina O. CO₂-concentrating mechanism and its traits in haloalkaliphilic cyanobacteria. Microbiology. 2015;84:112–24.View ArticleGoogle Scholar
Satoh A, Kurano N, Senger H, Miyachi S. Regulation of energy balance in photosystems in response to changes in CO₂ concentrations and light intensities during growth in extremely-high-CO₂-tolerant green microalgae. Plant Cell Physiol. 2002;43:440–51.View ArticleGoogle Scholar
Zhao B, Su Y, Zhang Y, Cui G. Carbon dioxide fixation and biomass production from combustion flue gas using energy microalgae. Energy. 2015;89:347–57.View ArticleGoogle Scholar
Huang Y, Cheng J, Lu H, Huang R, Zhou J, Cen K. Simultaneous enhancement of microalgae biomass growth and lipid accumulation under continuous aeration with 15% CO₂. RSC Adv. 2015;5:50851–8.View ArticleGoogle Scholar
Thoms S, Pahlow M, Wolf-Gladrow D. Model of the carbon concentrating mechanism in chloroplasts of eukaryotic algae. J Theor Biol. 2001;208:295–313.View ArticleGoogle Scholar
Schwedock J, Harmer T, Scott K, Hektor H, Seitz A, Fontana M, Distel D, Cavanaugh C. Characterization and expression of genes from the RubisCO gene cluster of the chemoautotrophic symbiont of Solemya velum: cbbLSQO. Arch Microbiol. 2004;182:18–29.View ArticleGoogle Scholar
Cheng R, Feng J, Zhang B, Huang Y, Cheng J, Zhang C. Transcriptome and gene expression analysis of an oleaginous diatom under different salinity conditions. BioEnergy Res. 2014;7:192–205.View ArticleGoogle Scholar
Matsuda Y, Hara T, Colman B. Regulation of the induction of bicarbonate uptake by dissolved CO₂ in the marine diatom, Phaeodactylum tricornutum. Plant Cell Environ. 2001;24:611–20.View ArticleGoogle Scholar
Lorenzen C. Determination of chlorophyll and pheo-pigments: spectrophotometric equations. Limnol Oceanogr. 1967;12:343–6.View ArticleGoogle Scholar
Millero F, Graham T, Huang F, Bustos-Serrano H, Pierrot D. Dissociation constants of carbonic acid in seawater as a function of salinity and temperature. Mar Chem. 2006;100:80–94.View ArticleGoogle Scholar
Cheng J, Sun J, Huang Y, Feng J, Zhou J, Cen K. Dynamic microstructures and fractal characterization of cell wall disruption for microwave irradiation-assisted lipid extraction from wet microalgae. Bioresour Technol. 2013;150:67–72.View ArticleGoogle Scholar
Fridlyand L. Models of CO₂ concentrating mechanisms in microalgae taking into account cell and chloroplast structure. Biosystems. 1997;44:41–57.View ArticleGoogle Scholar
Kuchitsu K, Tsuzuki M, Miyachi S. Polypeptide composition and enzyme activities of the pyrenoid and its regulation by CO₂ concentration in unicellular green algae. Can J Bot. 1991;69:1062–9.View ArticleGoogle Scholar
Ho S, Chen C, Lee D, Chang J. Perspectives on microalgal CO₂ emission mitigation systems—a review. Biotech Adv. 2011;29:189–98.View ArticleGoogle Scholar
Badger M, Andrews T, Whitney S, Ludwig M, Yellowlees D, Leggat W, Price G. The diversity and coevolution of rubisco, plastids, pyrenoids, and chloroplast-based CO₂-concentrating mechanisms in algae. Can J Bot. 1998;76:1052–71.Google Scholar
Price G. Inorganic carbon transporters of the cyanobacterial CO₂ concentrating mechanism. Photosynth Res. 2011;109:47–57.View ArticleGoogle Scholar
Fan J, Xu H, Luo Y, Wan M, Huang J, Wang W, Li Y. Impacts of CO₂ concentration on growth, lipid accumulation, and carbon-concentrating-mechanism-related gene expression in oleaginous Chlorella. Appl Microbiol Biotechnol. 2015;99:2451–62.View ArticleGoogle Scholar
Xia J, Gao K. Impacts of elevated CO₂ concentration on biochemical composition, carbonic anhydrase, and nitrate reductase activity of freshwater green algae. J Integr Plant Biol. 2005;47:668–75.View ArticleGoogle Scholar
Kim W, Park J, Gim G, Jeong S, Kang C, Kim D, Kim S. Optimization of culture conditions and comparison of biomass productivity of three green algae. Bioproc Biosyst Eng. 2012;35:19–27.View ArticleGoogle Scholar
Edwards V, Tett P, Jones K. Changes in the yield of chlorophyll a from dissolved available inorganic nitrogen after an enrichment event—applications for predicting eutrophication in coastal waters. Cont Shelf Res. 2003;23:1771–85.View ArticleGoogle Scholar
Moroney J, Somanchi A. How do algae concentrate CO₂ to increase the efficiency of photosynthetic carbon fixation. Plant Physiol. 1999;119:9–16.View ArticleGoogle Scholar
Lan Y, Keith A. Determination of apparent Km values for ribulose-1,5-bisphosphate carboxylase/oxygenase (rubisco) activase using the spectrophotometric assay of rubisco activity. Plant Physiol. 1991;95:604–9.View ArticleGoogle Scholar
Rabinowitch Eugenne I. Photosynthesis and related processes. Soil Sci. 1951;72:482.View ArticleGoogle Scholar
Drake B, Gonzàlez-Meler M, Long S. More efficient plants: a consequence of rising atmospheric CO₂. Physiol Mol Biol Plant. 1997;48:609–39.View ArticleGoogle Scholar
Sage R. Acclimation of photosynthesis to increasing atmospheric CO₂: the gas exchange perspective. Photosynth Res. 1994;39:351–68.View ArticleGoogle Scholar

Transcriptome and key genes expression related to carbon fixation pathways in Chlorella PY-ZU1 cells and their growth under high concentrations of CO₂