- Open Access
Potassium channel KCN11 is required for maintaining cellular osmolarity during nitrogen starvation to control proper cell physiology and TAG accumulation in Chlamydomonas reinhardtii
Biotechnology for Biofuels volume 13, Article number: 129 (2020)
Nitrogen (N) starvation in algae induces a variety of structural and metabolic changes including accumulation of triacylglycerol (TAG). Given the promising prospect of using algae as feedstock for biofuel production, accumulation of TAG upon N starvation becomes an ideal system to study TAG biosynthesis. Under nitrogen-depleted conditions, algae also accumulate compatible solutes such as sugar and certain amino acids, which is expected to elevate osmolarity in the cytoplasm. However, how osmoregulation is maintained and how it impacts on carbon metabolism, especially TAG accumulation under N starvation, are not well understood.
We show here that potassium channel KCN11 localized in the contractile vacuole (CV) mediates osmoregulation during N starvation and loss of KCN11 profoundly affects cell physiology and TAG biosynthesis. KCN11 level is increased and the CV pulsation is accelerated. Loss of KCN11 induces aberrant CV cycle, inhibition of cell growth, increase of cell size, inhibition of chlorophyll loss and TAG accumulation. These effects are rescued by addition of sucrose to raise osmolarity in the culture medium, indicating that osmoregulation is required for cell adaptation to N starvation. Metabolomic analysis shows reduction of acetyl-CoA and accumulation of glyceraldehyde-3-phosphate in kcn11 mutant relative to the control under N starvation, indicating that defects in acetyl-CoA biosynthesis and some metabolic steps from glyceraldehyde-3-phosphate to TAG contribute to the decreased TAG accumulation due to loss of osmoregulation.
This work provides novel insight of osmoregulation during N starvation in the control of cell physiology and metabolism especially TAG accumulation. According to these findings, we propose that osmolarity should be carefully monitored during the industrial production of biodiesel.
Nitrogen (N) is a key element for the growth and development of plant cells and algae. The impact of N deficiency on gene expression and metabolism in Chlamydomonas reinhardtii, a widely used model for studying various fundamental processes, has been studied for decades. This includes studies of photosynthesis and of the activation of the gametogenesis program [1,2,3,4]. These studies documented the changes in significant physiological reprogramming, such as ribosome abundance, starch accumulation, and organization of the thylakoid membrane [5,6,7,8,9]. Interest in these pathways has renewed recently because of the use of C. reinhardtii as a reference organism for understanding triacylglycerol (TAG) accumulation pathways induced by N starvation [10,11,12,13,14,15,16].
Recently, a transcriptomic analysis in Neochloris oleoabundans has reported that N starvation leads to a significant change in the metabolism of both sugar and proline; in particular, the conversion from UDP-glucose to sucrose is strongly enhanced under nitrogen-depleted condition . Sugars and proline are main groups of compatible solutes found in algae . In seed plants, N starvation also induces accumulation of amino acids that function as compatible solutes . Synthesis and degradation of compatible solutes (also known as “low molecular weight metabolites”) are important mechanisms for achieving osmotic balance. Osmotic adjustment is pivotal for cell survival and metabolism in unicellular algae. The regulatory responses of algae include changes of cell volume, intracellular ion concentration, intracellular glycerol concentration, and the expression of some genes [20, 21]. Inhibited growth and photosynthetic rates by osmotic stress are also observed in Chlamydomonas reinhardtii . Under N starvation conditions in Chlamydomonas, it is unknown whether osmoregulation is changed relative to normal growth conditions, and how osmoregulation is maintained. Furthermore, how osmoregulation affects TAG accumulation is not clear.
The osmoregulation of Chlamydomonas reinhardii is mediated by contractile vacuoles (CVs). Two CVs, localized in the cell anterior near the flagellar base, pulsate alternatively to remove excessive water from the cytoplasm to maintain cellular osmolarity [23, 24]. Our previous study showed that a potassium channel KCN11 is located in the membrane of the contractive vacuole. Loss of KCN11 in a kcn11 mutant generated by DNA insertional mutagenesis disrupts proper pulsation of the contractile vacuole and osmoregulation , suggesting that KCN11 is important for osmoregulation. It has been reported that the expression of KCN11 was up-regulated during N starvation . Thus, we aim to investigate the role of KCN11 in osmoregulation as well as metabolic changes under N starvation.
Elevation of KCN11 level and contractile vacuole cycling rate during N starvation
Transcriptional analysis showed that the expression of KCN11 mRNA is strongly induced upon N starvation . To determine whether the protein level of KCN11 is also increased, kcn11 rescued cells expressing HA-tagged KCN11 were transferred from N-replete to N-depleted media followed by immunoblot analysis. As shown in Fig. 1a, the level of KCN11 was increased several folds shortly after cells being transferred to N-delete medium and remained highly expressed for a period of 48 h. Next, we examined CV cycling, a process that the CV absorbs water from the cytoplasm followed by water discharge to the outside of the cell repeatedly, which is an indicator of osmoregulation . Compared to N-replete conditions, the contractile vacuole period under N-depleted conditions was decreased approximately by half, which reflects an increase of CV cycling rate (Fig. 1b). These data suggest that N starvation increases cellular osmolarity, which is accompanied with increased protein level of KCN11 and CV cycling rate.
The kcn11 mutant fails to expel liquid from the cells efficiently
Our previous work showed that under normal growth condition, KCN11 does not affect the CV cycle. However, under hypotonic condition, CV pulsation is accelerated and lack of KCN11 impaired CV pulsation and cell growth . The increase of cellular osmolarity during N starvation would increase water influx. Such a situation is similar to a hypotonic condition. To determine whether KCN11 is required for CV pulsation during N starvation, the CV cycles were measured. In wild-type cells and rescued cells, the CVs pulsate with an oscillating pattern (Fig. 1c). In contrast, the CV cycles of N-starved kcn11 were too aberrant to do the quantitative analysis. Some CVs did not or slowly pulsate with abnormal large CV size (Fig. 1c). These data demonstrate that KCN11 is essential for CV pulsation during N starvation. Nevertheless, the kcn11 mutant is able to survive in the absence of nitrogen (Fig. 1d), indicating that osmoregulation is not essential for cell survival under N deprivation.
Loss of KCN11 alters cell morphology, growth and chlorophyll content
Loss of KCN11 impairs CV pulsation during N starvation, which is expected to affect osmoregulation leading to defects in various cellular processes. Microscopic examination found that kcn11 mutant cells gradually lost their flagella during N starvation (Fig. 2a, b). The cell size decreased during N starvation for wild-type cells. In contrast, the cell size was increased in kcn11 mutant cells (Fig. 2c). Within 1 day of N starvation, wild-type cells were still able to divide. However, cell proliferation in the kcn11 mutant was inhibited (Fig. 2d). We also found that KCN11 affected chlorophyll content of the cell. The cellular level of chlorophyll decreased rapidly in wild-type cells during a 2-day culture in N-deficient conditions (from 1.73 to 0.26 pg per cell). In contrast, the cellular level of chlorophyll in kcn11 cells decreased much slower (from 1.32 to 0.73 pg per cell) (Fig. 2e, f).
KCN11 affects TAG accumulation during N starvation
Accumulation of TAG is induced during N starvation in Chlamydomonas . We then evaluated the influence of KCN11 on the accumulation of lipid. In contrast to wild-type and rescued cells, kcn11 mutant cells barely formed lipid droplets shown by Nile Red staining (Fig. 3a). The cellular number and size of the lipid droplets were greatly reduced in the kcn11 mutant relative to the control cells (Fig. 3b, c). These observations were consistent with analysis by electronic microscopy (Fig. 3d). We analyzed TAG amount by TLC (Fig. 3e, f). The amount of TAG in kcn11 mutant was 4.35 µg per 4 × 106 cells, which is 25.89% of that in wild-type cells (16.8 µg per 4 × 106 cells) after 2 days of N deficiency. These data demonstrate that KCN11 is required for TAG accumulation during N starvation.
Relieving osmotic stress and/or potassium stress rescues defects caused by KCN11 deletion
The defect in CV cycle in kcn11 mutant cells suggests that loss of osmoregulation may be responsible for various defective cellular processes mentioned above during N starvation. It remains to be demonstrated experimentally that this is indeed the case. To this end, we elevated the osmolarity of the N-depleted culture medium by adding different concentrations of sucrose. With increasing concentrations of sucrose, we found that the cell size of the kcn11 mutant gradually decreased and approached normal cell size at 40 mM sucrose (Fig. 4a). We also observed that cell growth of the kcn11 mutant was also rescued at concentrations above 40 mM sucrose (Fig. 4b). Next, we examined the effect of 40 mM sucrose on the cellular chlorophyll level and TAG accumulation. Adding sucrose barely affected the chlorophyll content of the wild-type cells; however, that of the kcn11 mutant decreased (Fig. 4c). Microscopic analysis showed that addition of sucrose also rescued the number and size of the droplets in kcn11 mutant cells (Fig. 4d–f).
Considering KCN11 is an outwardly potassium channel localized in the CV membrane , disruption of KCN11 may lead to an increase of potassium concentration in the cytoplasm. Abnormal accumulation of potassium in the cytoplasm may also contribute to some of the defective phenotypes in the kcn11 mutant. Potassium was replaced with sodium in the N-depleted medium. The cell size, growth and chlorophyll content of kcn11 mutant cells were not rescued (data not shown). Interestingly, the number of lipid droplets was apparently increased in the kcn11 mutant when potassium was omitted (Fig. 5a, b). However, the size of the lipid droplets was not rescued (Fig. 5a, c). These data suggest that osmoregulation impaired by the absence of KCN11 is required for various aspects of cell physiology and metabolism following N deprivation.
Analysis of carbon metabolism affected by loss of KCN11
Glycolysis and TCA cycle provide the raw materials and reducing power for TAG de novo synthesis. In view of this, we investigated the main metabolites in the glycolysis pathway and the TCA cycle in N-replete and N-depleted media of wild-type and kcn11 cells, respectively (Fig. 6). This analysis may reveal the metabolic basis for TAG accumulation during N starvation and the metabolic steps for TAG accumulation that are profoundly affected by failure of osmoregulation due to loss of KCN11.
Compared to nitrogen-replete condition, a lot of metabolites in the glycolytic pathway during N starvation such as glucose-6-phosphate (G6P), fructose-6-phosphate (F6P), glyceraldehyde-3-phosphate (GA3P) and dihydroxyacetone phosphate (DHAP) and pyruvate increased significantly during nitrogen deficiency, both for wild-type and kcn11 cells. Please note that DHAP is an important substrate for lipid synthesis and acetyl-CoA provided by pyruvate is a “building block” for fatty acids’ synthesis. The glycolytic metabolites (especially DHAP and pyruvate) may account for the production of fatty acids and lipids during nitrogen deficiency. Likewise, compared to nitrogen-replete condition, a lot of metabolites in the Krebs cycle such as isocitrate, α-ketoglutarate (AKG), succinate and malate increased significantly during nitrogen deficiency, which is also consistent for TAG accumulation under this condition. We also observed that the levels of some metabolites were decreased under N-depleted conditions. The reasons are unknown. It may reflect that some of the metabolites have higher turnover rates.
Acetyl-CoA and G3P are the end-products derived from the glycolytic pathway and/or the TCA cycle for TAG biosynthesis. The level of acetyl-CoA was decreased in the N-depleted kcn11 mutant relative to N-depleted wild-type cells. This may suggest that the lower level of acetyl-CoA may contribute to the inhibition of TAG synthesis in kcn11 mutant during N starvation. Interestingly, the level of G3P is much higher in the N-depleted kcn11 mutant relative to N-depleted wild-type cells. Given that kcn11 mutant was unable to accumulate TAG, it suggests that some of the downstream metabolic steps toward TAG synthesis may be defective in kcn11 mutant during N starvation. To determine whether these effects were caused by failed osmoregulation due to KCN11 mutation, we measured the levels of acetyl-CoA and G3P in N-delete kcn11 cells in the presence of 40 mM sucrose. As expected, the level of acetyl-CoA was increased while that of G3P was decreased relative to the control without addition of sucrose. Thus, we propose that osmoregulation mediated by KCN11 affects the production of acetyl-CoA and some metabolic steps from G3P to TAG.
We have discovered that osmoregulation mediated by KCN11 plays a critical role in cell physiology and metabolism during N starvation in C. reinhardtii. We showed that the level of KCN11 was elevated and the rate of CV pulsation was increased when cells were cultured in N-depleted medium. Deletion of KCN11 in the kcn11 mutant resulted in impairment of the CV cycle. These data demonstrate that N starvation increases cellular osmolarity, which is counter-balanced by accelerated CV pulsation. What is the trigger for inducing such a change in CV pulsation? One hypothesis is that the increased osmolarity resulting from accumulation of small metabolites in the cytosol would allow more water to flow in from outside the cell due to osmotic pressure. The CV would be filled up quickly with water from the cytoplasm, which is subsequently discharged to the outside, thus increased CV cycling is entailed. The level of KCN11 is elevated under nitrogen deficiency, it is interesting to explore whether there is a correlation between KCN11 level and CV period that reflects cytosolic osmolarity by analyzing cells at different times after onset of N depletion. Under N starvation, except for defects in CV pulsation, kcn11 is also defective in regulation of cell growth and size and metabolic changes such as chlorophyll loss and TAG accumulation. KCN11 is a potassium channel; disruption of KCN11 may also result in elevation of cellular potassium, which may cause potassium toxicity leading to physiological defects . However, omitting potassium can only partially restore TAG accumulation but other defects. In contrast, raising the osmolarity in the culture medium by addition of sucrose rescues all the defects, indicating that osmoregulation is pivotal for proper cell physiology and metabolism.
As an important molecule that is present at the intersection of multiple biochemical pathways, acetyl-CoA can be produced by several metabolic pathways, including glycolysis, TCA cycle, amino acid catabolism and lipids’ oxidation. TAG synthesis requires acetyl-CoA as well as G3P. Our metabolic study shows lots of upstream glycolytic metabolites in kcn11 mutant were more than those in wild type following N deprivation, but there was no significant difference in pyruvate content and even less acetyl-CoA in kcn11 mutant, indicating that enzymes of initial glycolytic pathway which are primarily in the chloroplast were activated, while pyruvate kinase which is primarily cytosolic and pyruvate dehydrogenase which is primarily in the chloroplast and mitochondria were suppressed in the kcn11 mutant [27, 28]. We have also observed there is more glutamine in kcn11, suggesting a block from glutamine to acetyl-CoA, which probably occurs in the mitochondria . G3P is backbone of TAG and starting material for TAG synthesis. The higher level of G3P in kcn11 under N-depleted conditions suggests that G3P may not be efficiently utilized and accumulated. It indicates that some of the metabolic steps downstream of G3P which is primarily in the chloroplast are negatively affected . Studies in diatom showed that carbon limitation by low light reorients carbon metabolism to production of phosphoenolpyruvic acid (PEP) and/or pyruvate, indicating that these metabolites are critical for carbon and downstream metabolisms [29, 30]. The suppression of production of pyruvate and its immediate product acetyl-CoA in the kcn11 mutant are consistent with their critical role in lipid biosynthesis. In addition, our findings are consistent with previous studies that alteration of osmolarity could induce changes in protein conformational equilibria and modulate the activities of enzymes [31, 32].
Microalgae accumulate TAG as energy storage during N starvation. As TAG can be turned into biofuel after transesterification with methanol, algae have been regarded as one of the most promising feedstocks for the production of biofuels. A major limitation is that nitrogen deprivation provokes several side effects such as impairments in photosynthesis , as well as the slow down and cessation of cell growth . For a long time, researchers have tried a variety of methods to realize the mutual improvement of both biomass and TAG [35,36,37,38]; however, the outcome is barely satisfactory . Several studies showed that manipulation of intracellular carbon flow can promote the synthesis of TAG in cells. For example, sta6 mutant is able to accumulate more TAG because of the lack of small subunit of ADPGlc pyrophosphorylase for starch formation . Indeed, a comparative study has shown that several metabolic processes are altered in the sta6 mutant; therefore, detailed analysis toward carbon flux in mutants affecting TAG synthesis may contribute to the understanding of the relationship between carbon metabolism and TAG synthesis . So far, only a few mutants that are defective in TAG accumulation have been found in Chlamydomonas. For example, starch-accumulating mutants (e.g., sta6 [ADP-glucose pyrophosphorylase], sta7-10 [isoamylase], bgal1 [β-galactosidase-like protein]), acyl-editing mutants (e.g., pgd1 [plastid galactoglycerolipid degradation 1], tgd2 [trigalactosyldiacylglycerol 2], pdat1 [phospholipid:diacylglycerol acyltransferase 1]) and TAG mobilization mutants (e.g., lip4 [lipase 4]) [16, 38, 42,43,44,45]. The kcn11 mutant is a new addition to this mutant library. Other mutants of CV function may show similar phenotypes . In addition, considering the important role of osmotic stress in carbon metabolism , the current study provides a new perspective for the investigation of TAG accumulation mechanism.
Loss of KCN11, a protein located in the membrane of the contractile vacuole (CV), profoundly affects cell physiology and TAG biosynthesis under N starvation. These effects are rescued by raising osmolarity in the N-depleted culture medium. Further metabolomic analysis reveals that the metabolic basis for TAG accumulation and the metabolic steps for TAG accumulation are affected by failure of osmoregulation. These results indicate an important role of osmolarity in controlling proper cell physiology and TAG accumulation during N deprivation. According to our findings, we propose that osmolarity should be carefully monitored during the industrial production of biodiesel.
Materials and methods
Stains, culture conditions and morphological analysis
Chlamydomonas reinhardtii strain 21gr (mt+) (CC-1690) is available from the Chlamydomonas Genetics Center, University of Minnesota. Generation of a kcn11 mutant and a rescued strain expressing KCN11-HA was as described previously . Cells were cultured in 250-ml erlenmeyer flasks with aeration with normal air at 23 °C under a 14 h-light–10 h-dark cycle. The light intensity was ~ 2000 Lux. For studies of N deficiency, cells grown in M medium were centrifuged, washed and further cultured in M–N medium at continuous illumination. Cell densities were estimated by counting fixed cells (1% glutaraldehyde) in the blood counting chamber. A Zeiss Axio Observer Z1 microscope (Zeiss) equipped with an electron microscope charge-coupled device camera (QuantEM512SC, Photometrics) was applied for cell imaging. Cell volumes were calculated based on the ellipsoid shape of Chlamydomonas cells using the formula 4/3π[L/2][W/2]2 , where L is cell length and W cell width, both of them were measured using ImageJ software (National Institutes of Health).
Contractile vacuole cycle was measured as described previously using two microscopy imaging systems . The microscopy system described above was used to take images every 50 ms for statistical analysis and a Zeiss LSM780 META Observer Z1 Confocal Laser Microscope with 100× objective (NA1.40) was used to present the CV cycle for each cell.
Cells were stained with FDA (20 µg/ml, final concentration) for 5 min in the dark at room temperature and the samples were captured under Zeiss Axio Observer Z1 microscope equipped with a CCD camera (QuantEM 512SC, Photometrics) using a 40× objective to calculate the cell survival rate.
Measurement of chlorophyll content and lipid analysis
Chlorophyll of cell pellet was extracted using 95% (v/v) ethanol and chlorophyll concentrations were calculated after measuring absorbance at 663 and 645 nm. Total chlorophyll was determined using equation, [Chl] (mg/l) = 20.2 * OD645 + 8.02 * OD663 . For neutral lipids staining, cells starved for different time as indicated were stained with Nile Red (1 μg/ml in DMSO, final concentration, Sigma) for 5 min in the dark. Images were acquired using the Zeiss microscope (see above) equipped with 100 × oil objective lens. The Nile Red and chlorophyll signals were captured using the green (BP, 515–565 nm) and red (BP, 575–640 nm) fluorescence filters (Zeiss, Germany), respectively. Total lipids were extracted in a chloroform:methanol (1:2, v/v) system. After centrifuged at 3000×g for 10 min, the lower organic phase was transferred into a glass tube, dried at 70 °C under N2 gas and dissolved again in dimethylbenzene. The protein phase between water and organic phase was dried and dissolved in 0.2 M KOH at 37 °C overnight, the concentration determined by BSA assay was used as loading control. Neutral lipids (TAG) were separated by thin-layer chromatography (TLC) using silica plates developed with n-hexane:diethyl ether:acetic acid (70:30:1, v/v) and visualized by spraying the plates with CuSO4–H3PO4 (10% CuSO4 w/v, 10% H3PO4 v/v) followed by heating at 120 °C. ImageJ software was used for the quantification (https://imagej.nih.gov/ij/) (NIH, USA).
SDS-PAGE and immunoblotting
SDS-PAGE and immunoblotting analysis were essentially as described previously . Primary antibodies used are rat monoclonal anti-HA (1:2000, clone 3F10, Roche) and rabbit anti-CrCDPK3 antibody .
Metabolites were simply extracted in a water–methanol–chloroform mixture (1:2:1, v:v:v) after metabolic activity quenching by injecting cells into 70% methanol (1:5, v:v). Targeted metabolomic experiment was analyzed by TSQ Quantiva. C18-based reverse-phase chromatography was utilized with 10 mM tributylamine, 15 mM acetate in water and 100% methanol as mobile phase A and B, respectively. This analysis focused on TCA cycle, glycolysis pathway, pentose phosphate pathway, amino acids and purine metabolism. In this experiment, we used a 25-min gradient from 5 to 90% mobile B. Positive–negative ion switching mode was performed for data acquisition. Cycle time was set as 1 s and a total of 300 ion pairs were included. The resolutions for Q1 and Q3 are both 0.7 FWHM. The source parameters are as follows: 3500 v for positive and 2500 v for negative ion mode; capillary temperature: 320 °C; heater temperature: 300 °C; sheath gas flow rate: 35; auxiliary gas flow rate: 10. Data analysis and quantitation were performed by the software Tracefinder (Thermo Fisher, CA).
The Dionex Ultimate 3000 UPLC system was coupled to a Q Exactive orbitrap mass spectrometer (Thermo Fisher, CA), equipped with a heated electrospray ionization (HESI) probe in positive ion mode. Extracts were separated by an ACQUITY UPLC HSS T3 column (2.1 × 100 mm, 1.8 μm, Waters). A binary solvent system was used, in which mobile phase A consisted of 5 mM ammonium acetate and 100% H2O, and mobile phase B of 100% methanol. A 10-min gradient with flow rate of 250 μl/min was used as follows: 0–2 min at 1% B; 2–4 min, 1–30% B; 4–6 min, 30–98% B; 6–7.1 min, 98% B; and 7.1–10 min, 1% B. Column chamber and sample tray were held at 35 °C and 10 °C, respectively. The data with mass range m/z 700–1500 were acquired by data-dependent MSMS acquisition. The full scan and fragment spectra were collected with resolution of 70,000 and 17,500, respectively. The source parameters are as follows: spray voltage: 3000 v; capillary temperature: 320 °C; heater temperature: 300 °C; sheath gas flow rate: 35; auxiliary gas flow rate: 10. Data analysis and quantitation were performed by the software Xcalibur 3.0.63 (Thermo Fisher, CA).
Availability of data and materials
All the data and materials are available by reasonable request.
- C. reinhardtii :
- TCA cycle:
Tricarboxylic acid cycle
Martin NC, Goodenough UW. Gametic differentiation in Chlamydomonas reinhardtii. I. Production of gametes and their fine structure. J Cell Biol. 1975;67:587–605.
Peltier G, Schmidt GW. Chlororespiration: an adaptation to nitrogen deficiency in Chlamydomonas reinhardtii. Proc Natl Acad Sci USA. 1991;88:4791–5.
Bulte L, Wollman FA. Evidence for a selective destabilization of an integral membrane protein, the cytochrome b6/f complex, during gametogenesis in Chlamydomonas reinhardtii. Eur J Biochem. 1992;204:327–36.
Abe J, Kubo T, Takagi Y, Saito T, Miura K, Fukuzawa H, Matsuda Y. The transcriptional program of synchronous gametogenesis in Chlamydomonas reinhardtii. Curr Genet. 2004;46:304–15.
Siaut M, Cuine S, Cagnon C, Fessler B, Nguyen M, Carrier P, Beyly A, Beisson F, Triantaphylides C, Li-Beisson Y, Peltier G. Oil accumulation in the model green alga Chlamydomonas reinhardtii: characterization, variability between common laboratory strains and relationship with starch reserves. BMC Biotechnol. 2011;11:7.
Cakmak T, Angun P, Demiray YE, Ozkan AD, Elibol Z, Tekinay T. Differential effects of nitrogen and sulfur deprivation on growth and biodiesel feedstock production of Chlamydomonas reinhardtii. Biotechnol Bioeng. 2012;109:1947–57.
Juergens MT, Deshpande RR, Lucker BF, Park JJ, Wang H, Gargouri M, Holguin FO, Disbrow B, Schaub T, Skepper JN, et al. The regulation of photosynthetic structure and function during nitrogen deprivation in Chlamydomonas reinhardtii. Plant Physiol. 2015;167:558–73.
Preininger É, Kósa A, Lőrincz ZS, Nyitrai P, Simon J, Böddi B, Keresztes Á, Gyurján I. Structural and functional changes in the photosynthetic apparatus of Chlamydomonas reinhardtii during nitrogen deprivation and replenishment. Photosynthetica. 2015;53:369–77.
Martin NC, Chiang K, Goodenough UW. Turnover of chloroplast and cytoplasmic ribosomes during gametogenesis in Chlamydomonas reinhardi. Dev Biol. 1976;51:190–201.
Hu Q, Sommerfeld M, Jarvis E, Ghirardi M, Posewitz M, Seibert M, Darzins A. Microalgal triacylglycerols as feedstocks for biofuel production: perspectives and advances. Plant J. 2008;54:621–39.
Wang ZT, Ullrich N, Joo S, Waffenschmidt S, Goodenough U. Algal lipid bodies: stress induction, purification, and biochemical characterization in wild-type and starchless Chlamydomonas reinhardtii. Eukaryot Cell. 2009;8:1856–68.
Miller R, Wu G, Deshpande RR, Vieler A, Gartner K, Li X, Moellering ER, Zauner S, Cornish AJ, Liu B, et al. Changes in transcript abundance in Chlamydomonas reinhardtii following nitrogen deprivation predict diversion of metabolism. Plant Physiol. 2010;154:1737–52.
Lenka SK, Carbonaro N, Park R, Miller SM, Thorpe I, Li Y. Current advances in molecular, biochemical, and computational modeling analysis of microalgal triacylglycerol biosynthesis. Biotechnol Adv. 2016;34:1046–63.
Wase N, Tu B, Allen JW, Black PN, DiRusso CC. Identification and metabolite profiling of chemical activators of lipid accumulation in green algae. Plant Physiol. 2017;174:2146–65.
Liang Y, Kong F, Torres RI, Burlacot A, Cuine S, Legeret B, Billon E, Brotman Y, Alseekh S, Fernie AR, et al. Branched-chain amino acid catabolism impacts triacylglycerol homeostasis in Chlamydomonas reinhardtii. Plant Physiol. 2019;179:1502–14.
Warakanont J, Tsai CH, Michel EJ, Murphy GR, Hsueh PY, Roston RL, Sears BB, Benning C. Chloroplast lipid transfer processes in Chlamydomonas reinhardtii involving a TRIGALACTOSYLDIACYLGLYCEROL 2 (TGD2) orthologue. Plant J. 2015;84:1005–20.
de Jaeger L, Carreres BM, Springer J, Schaap PJ, Eggink G, Martins DSV, Wijffels RH, Martens DE. Neochloris oleoabundans is worth its salt: transcriptomic analysis under salt and nitrogen stress. PLoS ONE. 2018;13:e194834.
Wegmann K. Osmoregulation in eukaryotic algae. FEMS Microbiol Lett. 1986;39:37–43.
Huang T, Jander G. Abscisic acid-regulated protein degradation causes osmotic stress-induced accumulation of branched-chain amino acids in Arabidopsis thaliana. Planta. 2017;246:737–47.
Chen H, Jiang JG. Osmotic responses of Dunaliella to the changes of salinity. J Cell Physiol. 2009;219:251–8.
Komsic-Buchmann K, Wostehoff L, Becker B. The contractile vacuole as a key regulator of cellular water flow in Chlamydomonas reinhardtii. Eukaryot Cell. 2014;13:1421–30.
Husic HD, Tolbert NE. Effect of osmotic stress on carbon metabolism in Chlamydomonas reinhardtii: accumulation of glycerol as an osmoregulatory solute. Plant Physiol. 1986;82:594–6.
Komsic-Buchmann K, Stephan LM, Becker B. The SEC6 protein is required for contractile vacuole function in Chlamydomonas reinhardtii. J Cell Sci. 2012;125:2885–95.
Luykx P, Hoppenrath M, Robinson DG. Structure and behavior of contractile vacuoles in Chlamydomonas reinhardtii. Protoplasma. 1997;198:73–84.
Xu F, Wu X, Jiang LH, Zhao H, Pan J. An organelle K+ channel is required for osmoregulation in Chlamydomonas reinhardtii. J Cell Sci. 2016;129:3008–14.
Ahanger MA, Tomar NS, Tittal M, Argal S, Agarwal RM. Plant growth under water/salt stress: ROS production; antioxidants and significance of added potassium under such conditions. Physiol Mol Biol Plants. 2017;23:731–44.
Johnson X, Alric J. Central carbon metabolism and electron transport in Chlamydomonas reinhardtii: metabolic constraints for carbon partitioning between oil and starch. Eukaryot Cell. 2013;12:776–93.
Khozin-Goldberg I, Cohen Z. Unraveling algal lipid metabolism: recent advances in gene identification. Biochimie. 2011;93:91–100.
Heydarizadeh P, Boureba W, Zahedi M, Huang B, Moreau B, Lukomska E, Couzinet-Mossion A, Wielgosz-Collin G, Martin-Jezequel V, Bougaran G, et al. Response of CO2-starved diatom Phaeodactylum tricornutum to light intensity transition. Philos Trans R Soc Lond B Biol Sci. 2017;372:20160396.
Heydarizadeh P, Veidl B, Huang B, Lukomska E, Wielgosz-Collin G, Couzinet-Mossion A, Bougaran G, Marchand J, Schoefs B. Carbon orientation in the diatom Phaeodactylum tricornutum: the effects of carbon limitation and photon flux density. Front Plant Sci. 2019;10:471.
Saunders AJ, Davis-Searles PR, Allen DL, Pielak GJ, Erie DA. Osmolyte-induced changes in protein conformational equilibria. Biopolymers. 2000;53:293–307.
Sharma P, Dubey RS. Modulation of nitrate reductase activity in rice seedlings under aluminium toxicity and water stress: role of osmolytes as enzyme protectant. J Plant Physiol. 2005;162:854–64.
Park JJ, Wang H, Gargouri M, Deshpande RR, Skepper JN, Holguin FO, Juergens MT, Shachar-Hill Y, Hicks LM, Gang DR. The response of Chlamydomonas reinhardtii to nitrogen deprivation: a systems biology analysis. Plant J. 2015;81:611–24.
Beck CF, Acker A. Gametic differentiation of Chlamydomonas reinhardtii: control by nitrogen and light. Plant Physiol. 1992;98:822–6.
Driver T, Trivedi DK, McIntosh OA, Dean AP, Goodacre R, Pittman JK. Two glycerol-3-phosphate dehydrogenases from Chlamydomonas have distinct roles in lipid metabolism. Plant Physiol. 2017;174:2083–97.
Kim Y, Terng EL, Riekhof WR, Cahoon EB, Cerutti H. Endoplasmic reticulum acyltransferase with prokaryotic substrate preference contributes to triacylglycerol assembly in Chlamydomonas. Proc Natl Acad Sci USA. 2018;115:1652–7.
Zhu Z, Yuan G, Fan X, Fan Y, Yang M, Yin Y, Liu J, Liu Y, Cao X, Tian J, Xue S. The synchronous TAG production with the growth by the expression of chloroplast transit peptide-fused ScPDAT in Chlamydomonas reinhardtii. Biotechnol Biofuels. 2018;11:156.
Li X, Moellering ER, Liu B, Johnny C, Fedewa M, Sears BB, Kuo MH, Benning C. A galactoglycerolipid lipase is required for triacylglycerol accumulation and survival following nitrogen deprivation in Chlamydomonas reinhardtii. Plant Cell. 2012;24:4670–86.
La Russa M, Bogen C, Uhmeyer A, Doebbe A, Filippone E, Kruse O, Mussgnug JH. Functional analysis of three type-2 DGAT homologue genes for triacylglycerol production in the green microalga Chlamydomonas reinhardtii. J Biotechnol. 2012;162:13–20.
Li Y, Han D, Hu G, Sommerfeld M, Hu Q. Inhibition of starch synthesis results in overproduction of lipids in Chlamydomonas reinhardtii. Biotechnol Bioeng. 2010;107:258–68.
Blaby IK, Glaesener AG, Mettler T, Fitz-Gibbon ST, Gallaher SD, Liu B, Boyle NR, Kropat J, Stitt M, Johnson S, et al. Systems-level analysis of nitrogen starvation-induced modifications of carbon metabolism in a Chlamydomonas reinhardtii starchless mutant. Plant Cell. 2013;25:4305–23.
Hung CH, Kanehara K, Nakamura Y. Isolation and characterization of a mutant defective in triacylglycerol accumulation in nitrogen-starved Chlamydomonas reinhardtii. Biochim Biophys Acta. 2016;1861:1282–93.
Boyle NR, Page MD, Liu B, Blaby IK, Casero D, Kropat J, Cokus SJ, Hong-Hermesdorf A, Shaw J, Karpowicz SJ, et al. Three acyltransferases and nitrogen-responsive regulator are implicated in nitrogen starvation-induced triacylglycerol accumulation in Chlamydomonas. J Biol Chem. 2012;287:15811–25.
Warakanont J, Li-Beisson Y, Benning C. LIP4 is involved in triacylglycerol degradation in Chlamydomonas reinhardtii. Plant Cell Physiol. 2019;60:1250–9.
Work VH, Radakovits R, Jinkerson RE, Meuser JE, Elliott LG, Vinyard DJ, Laurens LM, Dismukes GC, Posewitz MC. Increased lipid accumulation in the Chlamydomonas reinhardtii sta7-10 starchless isoamylase mutant and increased carbohydrate synthesis in complemented strains. Eukaryot Cell. 2010;9:1251–61.
Umen JG, Goodenough UW. Control of cell division by a retinoblastoma protein homolog in Chlamydomonas. Genes Dev. 2001;15:1652–61.
Fan J, Hu Z, Chan Z, Chen K, Amombo E, Chen L, Fu J. Alleviation of cold damage to photosystem II and metabolisms by melatonin in Bermudagrass. Front Plant Sci. 2015;6:925.
Cao M, Meng D, Wang L, Bei S, Snell WJ, Pan J. Activation loop phosphorylation of a protein kinase is a molecular marker of organelle size that dynamically reports flagellar length. Proc Natl Acad Sci USA. 2013;110:12337–42.
Liang Y, Pan J. Regulation of flagellar biogenesis by a calcium dependent protein kinase in Chlamydomonas reinhardtii. PLoS ONE. 2013;8:e69902.
We thank Dr. Peng Jiang from Tsinghua University for suggestions on metabolic analysis and Center of Biomedical Analysis, Tsinghua University for assistance with imaging and metabolic analysis.
This work was supported by the National Key R&D Program of China (2018YFA0902500) (to J.P.) and the National Natural Science Foundation of China (81901078) (to F.X.) and (31172405) (to J. P.).
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Xu, F., Pan, J. Potassium channel KCN11 is required for maintaining cellular osmolarity during nitrogen starvation to control proper cell physiology and TAG accumulation in Chlamydomonas reinhardtii. Biotechnol Biofuels 13, 129 (2020). https://doi.org/10.1186/s13068-020-01769-x
- N starvation