Iron is an essential micronutrient involved in many biological processes and is often limiting for primary production in large regions of the World Ocean. Metagenomic and physiological studies have identified clades or ecotypes of marine phytoplankton that are specialized in iron depleted ecological niches. Although less studied, eukaryotic picophytoplankton does contribute significantly to primary production and carbon transfer to higher trophic levels. In particular, metagenomic studies of the green picoalga Ostreococcus have revealed the occurrence of two main clades distributed along coast-offshore gradients, suggesting niche partitioning in different nutrient regimes. Here, we present a study of the response to iron limitation of four Ostreococcus strains isolated from contrasted environments. Whereas the strains isolated in nutrient-rich waters showed high iron requirements, the oceanic strains could cope with lower iron concentrations. The RCC802 strain, in particular, was able to maintain high growth rate at low iron levels. Together physiological and transcriptomic data indicate that the competitiveness of RCC802 under iron limitation is related to a lowering of iron needs though a reduction of the photosynthetic machinery and of protein content, rather than to cell size reduction. Our results overall suggest that iron is one of the factors driving the differentiation of physiologically specialized Ostreococcus strains in the ocean.
Iron is an essential element for all living organisms and in particular for photosynthetic phytoplanktonic cells in which numerous iron-sulphur centre and heme containing proteins are involved in the photosynthetic electron transfer and the nitrate reduction reactions. The extensive use of iron in the cellular machinery of modern microorganisms is inherited from the growth of their ancestors in the iron rich Archean ocean. However the geochemical evolution of the chemical composition of the ocean, largely driven by the evolution of life, has led to vanishing iron concentrations in the present ocean1. Thus, iron is a limiting resource in very large regions of the ocean.
Phytoplanktonic species are diverse in size, shape, phylogenetic origin and have evolved specific strategies to colonize ecological niches where iron is limiting (for a review see ref. 2). Physiological and molecular responses to iron limitation have been well studied in nano and microphytoplankton. Cultures of different species have revealed the critical role surface/volume ratio to deal with iron limitation3, 4 but several other adaptations to low iron conditions have also been reported. In oceanic diatoms, for example, the lowering of iron needs can be achieved by optimizing the architecture of the photosynthetic machinery through a decrease of the iron-rich complexes such as photosystem I and cytochrome b 6 /f 5,6,7. Iron storage into the ferritin protein pool also constitutes an efficient physiological strategy to cope with sporadic iron supply in pennate diatoms8.
The acclimation and adaptation strategies are less understood in picophytoplankton, despite the fact that small phytoplanktonic cells, such as the tiny picocyanobacterium Prochlorococcus, numerically dominate oligotrophic water phytoplanktonic communities9, 10. Metagenomic and physiological studies in iron depleted regions point to the presence of Prochlorococcus clades adapted to iron scarcity11,12,13. These adaptations could notably rely on the selection of specific gene repertoires during the evolution, such as the replacement of iron Super Oxide Dismutase (SOD) by Nickel SOD14, 15. Together, genomic and phylogeographic studies strongly suggest the existence of iron adapted lineages in prokaryotic picophytoplankton. A recent study in Synechococcus revealed that a coastal strain acclimates to changes in Fe concentration by modulating iron uptake, storage, and photosynthetic proteins16.
We recently unveiled a central role for ferritin in the day-night regulation of iron homeostasis in the picoeukaryotic alga Ostreococcus tauri and showed that the transcriptional response to iron limitation in this microorganism is tighly dependent on the diurnal cycle17, 18. Still, the adaptive responses of eukaryotic picophytoplankton to low iron conditions remain largely unexplored. Within the photosynthetic picoeukaryotes, the order of Mamelliales (Mamiellophyceae, Chlorophyta), encompassing the genera Ostreococcus, Bathycoccus and Micromonas, has a worldwide geographic distribution and it has been shown to contribute significantly to primary production in coastal ecosystems19,20,21,22. Ribosomal DNA sequence phylogenies segregate Ostreococcus sp into 4 phylogenetic clades (A-D) and physiological studies have demonstrated the existence of high- and low-light adapted strains in the genus Ostreococcus 23,24,25,26. Specific primers were successfully developed to amplify Ostreococcus clades A, B and C 18S ribosomal DNA, enabling the study of niche-partitioning in natural populations27. Coastal, meso- to eutrophic areas were dominated by clades A and C (renamed clade Ol), whereas open-ocean, oligotrophic regions were dominated by clade B (renamed clade OlI)27. This study also indicated that the distribution of Ostreococcus lineages is not explained primarily by light irradiance, and that the specialization in different nutrient regimes along coast-offshore gradients might be a key driver of picoeukaryotes evolution/diversification27.
In this paper, we compare the physiological responses to iron limitation of several Ostreococcus strains inhabiting different environments. Using a combination of physiological and transcriptomic approaches, we unveil several aspects of the specialization of Ostreococcus to environments with different levels of iron bioavailability. In particular, we have characterized a Mediterranean strain, RCC802, which shows very low iron requirement, and whose main adaptation trait to iron limitation is a marked cell biomass reduction.
Material and Methods
Algal Strains and culture conditions
Ostreococcus strains were obtained from the Roscoff Culture Collection (http://www.roscoff-culture-collection.org/): Ostreococcus tauri strain OTTH595 (RCC745; isolated from Thau Lagoon, France), Ostreococcus sp. RCC802 (isolated at 65 m in the Sicily channel, Italy), Ostreococcus sp. RCC809 (isolated from 105 m in the tropical Atlantic Ocean), and Ostreococcus sp. RCC789 (strain BL_82-7_clonal, isolated from surface water of Barcelona harbour, Spain).
Cells were grown at 20 °C under 25 µmol quanta m−2 s−1 of constant blue light (blue led, λMAX = 465 nm) in AQUIL medium17, 28 containing concentrations of Fe(III)-EDTA ranging between 5.4 and 270 nM, corresponding to the theoretical solubility limit of iron in sea water. All culture manipulations were conducted in clean room (class 10,000) equipped with a laminar flow hood (class 100). Synthetic ocean water (SOW) and solutions of inorganic nutrients (NO3 − and PO4 3−) were separately purified by removing trace metals using a Chelex 100 ion exchange resin (Bio-Rad). Final nutrients concentrations were 300 µM NO3 − and 10 µM PO4 3−. Trace metal solutions were buffered with 0.1 M of EDTA. For iron content determinations, cells were grown in modified F (Mf) medium29, 30 and iron was provided as radioactive 55Fe(III)-EDTA (1:20).
Growth rates and cell diameter measurement
To remove contaminating iron and deplete intracellular iron storage, Ostreococcus strains were first acclimated during 5 days in 1.5 mL of AQUIL medium containing 5.4 nM Fe(III)-EDTA (1:1). To study the growth response function of iron supply, triplicate flasks containing various concentrations of Fe(III)-EDTA ranging from 5.4 nM to 270 nM Fe(III)-EDTA in Aquil medium, were inoculated with 106 cells mL−1 of iron-depleted cells. These cultures were grown at 20 °C, under 25 µmol quanta m−2 s−1 of continuous blue light, as described above. Cell density and chlorophyll (Chl) red fluorescence were measured using a flow cytometer (BD Accury C6). Growth rates were computed as the slope of a Ln (Nt) vs. time plot, where Nt is the cell abundance (cell/mL) number at time t. Average cell diameter was estimated using a CASY multi-channel cell counting system. (Schärfe System GmbH, Germany).
Determination of photosynthetic parameters and chlorophyll quantitation
Light-response curves were recorded using a pulse amplitude modulated fluorometer (Phyto-PAM, Walz) connected to a chart recorder (Labpro, Vernier). Chlorophyll contents were determined using HPLC (Hewlett-Packard HPLC 1100 Series). Details are given in Supplementary information online.
Intracellular iron content measurements
Cells were grown in Mf medium devoid of iron for a week, and were then transferred to Mf medium containing 1 to 100 nM of 55Fe (III) EDTA (1:20, 29,600 MBq/mg). The iron cell content was determined by scintillation counting after bleaching photosynthetic pigments with sodium hypochlorite, as previously described17, 29.
Protein extraction and quantitation
The different Ostreococcus strains were grown in AQUIL medium containing various concentrations of Fe(III)-EDTA, in 24-wells microplates, under 20 µmol quanta m−2 s−1 of blue light irradiance at 20 °C. After 6 days, cells were harvested in 2 mL micro-tubes by centrifugation at 8 000 × g for 10 min. Dry pellets were frozen in liquid nitrogen ant stored at at −80 °C until extraction. All manipulations were carried out on ice. Cell pellets were ground in 50 µL extraction buffer (50 mM Tris-HCl pH 7.4, 100 mM NaCl, 5 mM EDTA, 0.5% (v/v) Nonidet NP40 (Sigma), 10% (v/v) glycerol, using a Tissue Lyser system (Quiagen). The samples were then centrifuged at 10 000 × g for 10 min to remove filter debris. The supernatant was collected, and the total protein concentration was determined using BCA (Bicinchoninic Acid) assay as described elsewhere31.
Oxygen levels were measured using a 24-channel sensor dish oxygen reader (Presens, Regenburg Germany). Cells were grown for one week in sealed OxoDishes® 4 mL vials, in AQUIL medium containing various concentrations of Fe(III)-EDTA. The sensor was placed at 20 °C under blue light. Before recording, light was switched off for 12 hours and the oxygen levels were then measured for 1 h under 20 µmol quanta m−2 s−1 blue light. Oxygen consumption, i.e. respiration, was subsequently monitored during 1 hour in darkness. Positive control consisted of cell-free medium oxygenated for 1 h. The negative control (0% O2) was obtained by dissolving 0.2 g of sodium L-ascorbate in 0.1 M NaOH.
RNA extraction and sequencing
Cell cultures were grown for 5 days in 100 mL AQUIL medium containing 5.4 nM (−Fe condition) or 270 nM (+Fe condition) Fe(III)-EDTA. Cultures were placed under 12:12 light/dark cycles of blue light at 40 µmol quanta m−2 s−1. Three cultures were harvested at 3 h, 9 h, 15 h, 22 h (time 0 h corresponded to dawn and time 12 h to dusk), by centrifugation for 10 min at 8 000 × g. Pellets were frozen in liquid nitrogen and stored at −80 °C. RNA extraction was carried out as described by Moulager et al.32. All manipulations were carried out on ice. The 24 RNA samples (12 +Fe, 12 –Fe) were submitted to high-throughput RNA sequencing using Illumina HiSeq™ 2000 custom pair-end stranded sequencing (Fasteris, Switzerland). After quality controls and filtering of low quality reads (bases quality lower than 15 on sliding window size of 4 bases), clean reads from all samples were gathered, resulting in a dataset of around 300 millions reads. Since there is no reference genome in RCC802, webuild by de novo assembly a reference transcriptome with the TRINITY program in version 2.1.133 using the default parameters and paired-end method. The transcript expression levels in each sample was determined by mapping each read from the sample to the reference transcriptome using BOWTIE34 and counting the number of aligned reads using BEDTOOLS35. We next applied the DEseq program36 to identify differentially expressed genes and calculate an associated risk of error (p-value). Different filtering procedures were finally performed in order to remove potential chimera. Systematic sequence comparisons with O. tauri (http://bioinformatics.psb.ugent.be/orcae/overview/OsttaV2) coding sequences were performed using tblastx program in version 2.2.29+37 with an evalue of 10 e−30. The whole procedure is detailed in Supplementary information online.
Growth rates of Ostreococcus strains under iron limitation
We selected a panel of Ostreococcus strains isolated in contrasted trophic regimes and representative of each of the different clades (Table 1). All strains were isolated in the Mediterranean Sea, but the clade B low light ecotype RCC809, which was isolated in the tropical Atlantic Ocean at 105 m depth. Two coastal strains were included in the study, RCC789 (clade D), from Barcelona harbour, and the lagoon strain OTTH595 (clade C) known as Ostreococcus tauri, the first Ostreococcus species discovered in the Thau lagoon in 199538. Both Ostreococcus tauri and RCC789 come from eutrophic areas where nutrient bioavailability is high, including iron. RCC802 (clade A) has been isolated at a 65 m depth between Sicily and Tunisia during the PROSOPE cruise39. Both RCC802 and RCC809 come from nutrient poor environments that display low Chl a concentrations in surface waters (Supplementary Figure 1)40. These geographic zones, however, are exposed to sporadic iron fertilization by aeolian mineral dust from the Sahara desert41, 42.
Ostreococcus strains were acclimated in AQUIL medium containing 5.4 nM Fe(III)-EDTA), to set the cells at the minimum iron level. The growth rates were then measured in response to a supply of various concentrations of total Fe, ranging from 5.4 to 270 nM. Upon transfer to iron replete conditions (270 nM total Fe), RCC802 displayed higher growth rates than the three other strains (Fig. 1). This strain outcompeted all other strains, maintaining high growth rates (∼1 d−1) for all Fe concentrations, except for 5.4 nM total Fe concentration, at which a 20% decrease in growth rate (0.8 ± 0.09 d−1) was observed. The coastal strains OTTH595 and RCC789 were the most sensitive to iron limitation. Their growth rates dropped dramatically for total Fe concentrations lower than 270 nM (0.42 d−1 ± 0.02 at 270 nM to 0.16 d−1 ± 0.04 at 54 nM total Fe for OTTH595; no growth of RCC789 from 54 nM). RCC809 displayed an intermediate response with a growth rate of 0.5 d−1 and of 0.15 d−1 at 54 nM and 5.4 nM total Fe, respectively.
Photosynthetic parameters of iron limited cells
The efficiency of light energy conversion by photosynthesis was studied using PAM fluorimetry (Fig. 2). Since the coastal strains OTTH595 and RCC789 exhibited very similar responses to iron limitation in terms of growth rates (Fig. 1), only OTTH595 together with RCC802 and RCC809 were further studied. In our standard culture conditions, all strains displayed optimal FV/FM values of about 0.65, as reported in previous studies26. We compared the photosystem II quantum yield of the three strains in iron replete and limiting conditions, corresponding to the lowest iron concentrations at which cell growth was observed, i.e. 54, 27 and 5.4 nM of total Fe for OTTH595, RCC809 and RCC802, respectively (Fig. 1).Under iron limitation, the photosystem II quantum yield of OTTH595 and RCC809 strains decreased by about 50% compared to iron replete conditions (from 0.64 to 0.34 for OTTH595 and from 0.59 to 0.31 for RCC809). For RCC802, only a moderate decrease of about 10% (from 0.61 to 0.54) was observed (Fig. 2A).
Light response curves were recorded to evaluate photosynthetic capacities. The maximal relative Electron Transfer Rate (rETRMAX) in photosystem II, a key photosynthetic complex located in the thylakoidal membranes of the plastid, dramatically dropped by more than 50% for both OTTH595 and RCC809 respectively. By contrast, no significant change in rETRmax values was observed for RCC802 (Fig. 2B). The α parameter, which corresponds to the initial slope of the light response curve, is related to the light harvesting efficiency of PSII at limiting light irradiance and thus provides indications on the functional size of the photosystem II antenna. Under iron limitation the α parameter of OTTH595 and RCC809 was 35% lower than under replete conditions, indicating reduced light harvesting capacities. As for rETRMAX, RCC802 show less than 10% decrease in the α parameter between iron depleted and replete conditions (Fig. 2C).
Cellular iron content was determined after 3 days of incubation of exponentially growing cells in the presence of various concentrations of 55Fe(III)-EDTA (Fig. 3). Under iron replete condition of 270 nM total Fe, similar iron contents were detected in OTTH595 (1.1 ± 0.1 10−15 mol 55Fe cells−1), RCC809 (1.10 ± 0.09 10−15 mol 55Fe cells−1) and RCC802 (1.28 ± 0.09 10−15 mol 55Fe cells−1). In OTTH595 and RCC809 Fe contents remained fairly constant for Fe concentrations of 27 and 54 nM (between 0.85 ± 0.04 and 1.20 ± 0.05 10−15 mol 55Fe cells−1). In RCC802, in contrast, the iron content dropped progressively from 1.51 ± 0.04 down to 0.040 ± 0.003 10−15 mol 55Fe cells−1, corresponding to a 19 fold reduction. At 5.4 nM total Fe, RCC809 and OTTH595 also had low Fe contents (0.39 ± 0.02 and 0.22 ± 0.02 10−15 mol 55Fe cells−1), however no cell growth was observed at this Fe concentration for these two strains (see Fig. 1).
Cell size and cell biomass reductions in response to iron limitation
We assessed the variations of the cellular volume in response to extracellular iron concentrations (Fig. 4A). The cell surface was inferred from the average cell diameter determined using a CASY cell counter, assuming a spherical shape of these coccoid cells. When cells were transferred from iron replete conditions (270 nM total Fe) to limiting conditions, both OTTH595 and RCC809 reduced their cellular volume, from 2.72 µm3 to 2.09 µm3 under limitation (108 nM of total Fe) for OTTH595 and from 2.45 µm3 down to 2.12 µm3 at 54 nM of total Fe for RCC809. For lower iron concentrations, however, the cellular volume of RCC809 was similar to the initial value, i.e. in iron replete conditions (2.5 µm3). In sharp contrast, the cellular volume of the RCC802 strain was about 4 fold smaller (∼0.6 µm3) than the two other strains, and remained constant independently of the external iron concentrations.
The Chl red fluorescence parameter (FL3), as determined by flow cytometry, provides a reliable proxy of the Chl content in Ostreococcus cells (Supplementary Figure 2). Figure 4B shows that for all strains, the cell Chl fluorescence decreased in response to iron limitation from 36.4 ± 0.4 down to 11.7 ± 0.1 in RCC802), from 59.7 ± 0.3 down to 41.5 ± 0.3 in RCC809 and from 76.4 ± 0.8 down to 55.3 ± 1.3 in OTTH595. The cellular protein content was determined under the same conditions (Fig. 4C). Under iron replete conditions, the protein cell content was about 2 to 3 fold lower in RCC802 (0.170 ± 0.02 pg cell−1) than in OTTH595 (0.464 ± 0.005 pg cell−1) and RCC809 (0.3 ± 0.04 pg cell−1). As for the cell Chl fluorescence, the protein content of RCC802 decreased dramatically in response to iron limitation (0.11 ± 0.01 pg cell−1 at 5.4 nM Fe(III)-EDTA corresponding to a 35% decrease). In OTTH595 and RCC802, smaller reductions in protein contents were observed, i.e. from 0.31 down to 0.29 pg cell−1 in RCC809 (5% decrease) and from 0.46 to 0.36 pg cell−1 in OTTH595 (20% decrease).
Normalized oxygen production of RCC802
The respiration and the oxygen net evolving cellular rates were measured in the RCC802 strain, under iron depleted (5.4 nM) and replete conditions (108 nM). The oxygen production, resulting from the activity of photosystems II, decreased by 50% under iron limitation, while the consumption due to respiration was four-times lower (Supplementary Figure 3). The net oxygen production (production - consumption) was reduced from 7.97 to 3.59 fM min−1 cell−1, corresponding to a 55% lowering (Fig. 5A). Interestingly, when normalized to the Chl red fluorescence, the net production of oxygen remained fairly stable in iron replete and depleted conditions (Fig. 5B).
Transcriptomic response of RCC802 to iron limitation
A transcriptomic study was conducted to get further insights into the regulation of mechanisms underlying acclimation and adaptation of RCC802 to iron depleted environments. RCC802 cultures were exposed to 12 h day:12 h night cycles under iron limited (5.4 nM Fe(III)-EDTA) and under iron replete conditions, for 7 days. RNA extracted from cells were harvested at 3, 9, 12, 15 and 22 h (i.e. 3 h before and after dawn and dusk) and subjected to RNAseq analysis, as described in Supplementary Figure 4. As there is no reference genome for RCC802, we undertook a de novo assembly approach to generate a full-length “reference transcriptome assembly” composed of all predicted transcripts produced by RCC802 in at least one experimental condition (Supplementary Figure 4). The number of reads, mapped on each reference transcript was used to calculate Log2(Fold Change) (LogFC) values (comparing −Fe and +Fe growth conditions) for each time point. Out of 2233 differentially expressed transcripts 980 were found to be upregulated (LogFC > 1, p-value < 0.01) and 1253 downregulated (LogFC < −1, pvalue < 0.01). After isoform filtering and removal of fusion transcripts based on systematic sequences comparisons with OTTH595, 1251 differentially expressed transcripts were kept (see Supplementary Data File 1). Based on the observation that a vast majority the genes of O. tauri are strongly regulated by the day/night cycle43, we focussed on genes that are induced or repressed in response to iron limitation at all day times. In iron depleted conditions 64 transcripts were downregulated (Fig. 6B, Supplementary Table 1). About one third of the sequences (23) were related to photosynthesis including (i) photosystem proteins such as chlorophyll a/b binding light-harvesting protein of PSI (Lhca proteins), and chlorophyll synthesis such as the Coproporphyrinogen III oxidase, (ii) components of the Calvin-Benson cycle such as the 1,5 ribulose bisphosphate carboxylase oxygenase (RubisCO) and the fructose-1,6-bisphosphatase. The second largest class of repressed transcripts (14) encodes enzymes involved in amino acid metabolism and components of the translation machinery such as translation elongation/initiation factors. Among the 15 remaining downregulated genes with putative homologues or functional domains in other organisms, we identified several iron binding proteins including cytochrome P450, cytochrome b 561 and a putative mitochondrial ferric reductase (Supplementary Table 2).
Only 13 transcripts were induced across all daytimes. A RCC802 flavodoxin with no homologue in O. tauri was overexpressed in all iron-depleted conditions, whereas the iron-containing ferredoxin was repressed under the same conditions (Fig. 6C). A putative Basic Helix loop Helix transcription factor was the only transcription factor induced at all day times under iron limitation.
Iron adapted strains in the genus Ostreococcus
Using iron limitation experiments, we were able to point out, among several Ostreococcus strains, differential abilities to grow in iron limiting conditions. Three different types of response are observed (Fig. 1). The coastal strains OTTH595 and RCC789 were capable of growing only under iron concentrations higher than 54 and 108 nM total Fe respectively, while the oceanic RCC809 strain showed growth down to 27 nM total Fe. RCC802, in contrast, grew well at all Fe concentrations tested with only a 20% reduction in growth rate at 5.4 nM total Fe. Comparison of growth rate inhibition between iron replete and limiting conditions clearly supports that RCC802 has the ability to grow under severe iron limitation like oceanic species such as the diatom Thalassiosira oceanica or the coccolithophorid Emiliana huxlyeyi (Table 2). In contrast, strains isolated in meso- to eutrophic environments showed much higher iron requirements. These differences in growth rate response were associated to differential physiological responses, such as the modulation of the chlorophyll and protein cell content, the photosynthetic activity, the iron cell content in response to iron limitation (Figs 1, 2, 3 and 4). RCC802 and to some extent RCC809 strains come from geographic areas where iron bioavailability is on average low, with only sporadic iron supplies from Sahara.
Our study overall strongly supports the existence of Ostreococcus strains or ecotypes physiologically adapted to environments where iron concentration may be low41. Interestingly, RCC802 showed higher growth rates than the other strains not only under iron depleted conditions, but also following iron addition to iron-limited cells (270 nM Fe(III)-EDTA condition in Fig. 1). This suggests that this strain may not be specialized to low iron environments but rather acclimates efficiently to fluctuating environmental iron bioavailability. It is also possible that OTTH595 and RCC809 did not perform as well as RCC802 under iron replete conditions because they had been more severely limited during the acclimation phase. The cellular iron quotas of RCC802 varied by about 20 fold between iron replete and iron depleted conditions (while maintaining cellular growth rate), thereby exemplifying the plastic response of RCC802 to fluctuating iron bioavailability. OTTH595 and RCC809, in contrast, showed little variation in iron content between iron replete (270 nM) and the lowest iron concentration at which cell growth occurred (54 and 27 nM, respectively).
Field studies have revealed that Ostreococcus OI (clade A and C) and OII (clade B) are rarely abundant at the same location and that OI populations are dominant in coastal, cool and/mesotrophic areas wheras OII populations are more abundant in warm, deep oligotrophic regions27. In agreement with these data OTTH595 (clade C) exhibits higher iron requirements than the deep strain RCC809 (clade B). Surprisingly, however, RCC802 (clade A) which belongs to OI clade and was isolated at 65 m deep, has very low iron requirements compared to other strains. Together these data indicate that like light irradiance, iron is a factor which influences the ecological niche partitioning of Ostreococcus strains.
Cell biomass reduction: a strategy to cope with iron limitation
Our observations showing that under iron limiting conditions, RCC802 exhibits the highest growth rate and the smallest cell diameter (compared to RCC809 and OTTH595) are consistent with the hypothesis that cell iron supply is limited by diffusion3, 44, 45. The smallest cells are more efficient to use iron because the supply of iron per unit of cellular volume is inversely related to the square of the cellular radius. We observed, however, that the size of RCC802 did not change when iron concentration decreased. RCC802 cells may have reach a minimal cell size, may be due to physical constraints such as mitotic spindle organization, which precludes further cell size reduction under iron limitation46. The main strategy of this strain to deal with iron limitation would, thus, rely on the optimisation of iron use rather than on cell size reduction. In agreement with this hypothesis we observed a nearly 20 fold decrease in intracellular iron content while maintaining cell size and growth rates under iron limitation.
Cell biomass, as estimated from the total amount of protein per cell, was much lower in RCC802 than in other strains. Compared to RCC809 and OTTH595, RCC802, showed a marked decrease of the Chl cell content, which was associated with a decrease of the oxygen net production rate per cell under iron limitation. When the oxygen net production was normalized by the Chl cell fluorescence (reflecting the Chl cell content), there was, however, no variation between iron depleted and iron replete conditions, demonstrating that the photosynthetic efficiency per Chl molecule was not affected. This is supported by the fact that the RCC802 photosystem II parameters did not significantly decrease upon iron limitation unlike in OTTH595 and RCC809, for which the growth rate decrease was associated to a pronounced drop of the photosystem II quantum yield and relative electron transport rate, strongly suggesting a global photosynthesis impairment (Fig. 2). This decrease likely originates from photosystem II photoinactivation (see e.g. ref. 47) and/or the induction of excess light energy dissipation mechanisms23, 26. Moreover, iron depletion induced a decrease in the light harvesting capacities in these strains and a global decrease of the Chl cell content (Figs 2C and 4B). These observations indicate that OTTH595 and RCC809 responded to iron limitation by drastically decreasing the amount of light energy utilized, which resulted in a strong decrease of the growth rate compared to RCC802 (Fig. 1). The downregulation of photosynthesis is probably the consequence of the high requirement for Fe of the photosynthetic apparatus, as characterized in other photosynthetic organisms such as diatoms44.
Altogether, our results suggest that, in response to iron limitation, RCC802 decreases the quantity of photosynthetic complexes per cell, i.e. the ‘volume’ of the photosynthetic machinery while maintaining its efficiency. In agreement with this hypothesis, RNAseq analysis, showed that in response to iron limitation, about one third of down regulated transcripts during all day time encode proteins involved in various aspects of photosynthesis including Chl synthesis, photosystem composition and Calvin-Benson cycle. The overall reduction in protein content is also reflected at the transcriptional level by the repression of genes involved in protein synthesis. In the low iron ecotype Thalassiosira oceanica, a similar reduction of the cellular protein content was probably due to a smaller number of chloroplasts per cell44. Ostreococcus species, unlike diatoms, contain a single chloroplast per cell, which occupies about 50% of the cell volume. The reduction of protein and chlorophyll content per cell in RCC802 is therefore likely to reflect a global reduction of the photosynthetic machinery and of the chloroplast. When comparing the expression patterns of the 64 RCC802 downregulated transcripts with putative homologues in OTTH595, we found that most genes were not downregulated in this latter species (Supplementary Table 3). This observation is consistent with the fact that OTTH595 does not reduce as much its cellular biomass under iron limitation.
Adaptations relying on the regulation of iron binding proteins are also suggested by the transcriptomic analyses. For example, an RCC802 flavodoxin, which had no homologue in OTTH595 or RCC809, is upregulated under iron limitation, while ferredoxin is downregulated (Fig. 6) suggesting that in RCC802 like in oceanic diatoms, the substitution of ferredoxin by flavodoxin may contribute to the ecological success under chronically low iron environments5,6,7. The single BHLH gene is the only transcription factor of RCC802 to be constitutively induced under iron limitation. BHLH, in contrast, was down regulated in OTTH595 under iron limitation. BHLH may, therefore, be a transcriptional regulator involved in the efficient acclimation of RCC802 to low iron environments, like theBHLH Fer gene of higher plants48.
Our results establish the existence of an Ostreococcus “low iron requiring strain”, which acclimates efficiently to low iron conditions. They support the field studies suggesting that picoeukaryotes should not be seen only as components of mesotrophic areas27 and suggest that iron may drive the differentiation of physiologically specialized strains along coast-ocean gradients. The main acclimation to low iron environment by Ostreococcus sp. RCC802 appears to involve primarily a reduction of cell biomass, rather than the reduction of cell surface/volume ratio reported in nano and microphytoplankton.
Saito, M. A., Sigman, D. M. & Morel, F. M. M. The bioinorganic chemistry of the ancient ocean: The co-evolution of cyanobacterial metal requirements and biogeochemical cycles at the Archean-Proterozoic boundary? Inorganica Chim. Acta 356, 308–318 (2003).
Morrissey, J. & Bowler, C. Iron Utilization in Marine Cyanobacteria and Eukaryotic Algae. Front. Microbiol. 3, 43 (2012).
Sunda, W. G. & Huntsman, S. A. Interrelated influence of iron, light and cell size on marine phytoplankton growth. Nature 2051, 1193–1197 (1997).
Lis, H., Shaked, Y., Kranzler, C., Keren, N. & Morel, F. M. M. Iron bioavailability to phytoplankton: an empirical approach. Isme J. 9, 1003–1013 (2015).
Strzepek, R. F. & Harrison, P. J. Photosynthetic architecture differs in coastal and oceanic diatoms. Nature 431, 689–692 (2004).
Peers, G. & Price, N. M. Copper-containing plastocyanin used for electron transport by an oceanic diatom. Nature 441, 341–4 (2006).
Lommer, M. et al. Recent transfer of an iron-regulated gene from the plastid to the nuclear genome in an oceanic diatom adapted to chronic iron limitation. BMC Genomics 11, 718 (2010).
Marchetti, A. et al. Ferritin is used for iron storage in bloom-forming marine pennate diatoms. Nature 457, 467–470 (2009).
Scanlan, D. J. Physiological diversity and niche adaptation in marine Synechococcus. Adv. Microb. Physiol. 47, 1–64 (2003).
Martiny, A. C., Huang, Y. & Li, W. Occurrence of phosphate acquisition genes in Prochlorococcus cells from different ocean regions. Environ. Microbiol. 11, 1340–1347 (2009).
Venter, J. C., Rusch, D. B., Martiny, A. C., Dupont, C. L. & Halpern, A. L. Characterization of Prochlorococcus clades from iron-depleted oceanic regions. Proc. Natl. Acad. Sci. 107, 16184–16189 (2010).
Huang, S. et al. Novel lineages of Prochlorococcus and Synechococcus in the global oceans. ISME J. 6, 285–97 (2012).
Biller, S. J., Berube, P. M., Lindell, D. & Chisholm, S. W. Prochlorococcus: the structure and function of collective diversity. Nat Rev Micro 13, 13–27 (2015).
Dufresne, A. et al. Genome sequence of the cyanobacterium Prochlorococcus marinus SS120, a nearly minimal oxyphototrophic genome. Proc. Natl. Acad. Sci. USA 100, 10020–10025 (2003).
Palenik, B. et al. The genome of a motile marine Synechococcus. Nature 424, 1037–1042 (2003).
Mackey, K. R. M. et al. Divergent responses of Atlantic coastal and oceanic Synechococcus to iron limitation. Proc. Natl. Acad. Sci. 112, 9944–9949 (2015).
Botebol, H. et al. Central role for ferritin in the day/night regulation of iron homeostasis in marine phytoplankton. Proc. Natl. Acad. Sci. 112, 14652–14657 (2015).
Lelandais, G. et al. Ostreococcus tauri is a new model green alga for studying iron metabolism in eukaryotic phytoplankton. BMC Genomics 17, 1–23 (2016).
Vaquer, A., Troussellier, M., Courties, C. & Bibent, B. Standing stock and dynamics of picophytoplankton in the Thau Lagoon (northwest Mediterranean coast). Limnol. Oceanogr. 41, 1821–1828 (1996).
Bec, B., Husseini-Ratrema, Collos, Y., Souchu, P. & Vaquer, A. Phytoplankton seasonal dynamics in a Mediterranean coastal lagoon: emphasis on the picoeukaryote community. J. Plankton Res. 27, 881–894 (2005).
O’Kelly, C. J., Sieracki, M. E., Thier, E. C. & Hobson, I. C. A transient bloom of Ostreococcus (Chlorophyta, Prasinophyceae) in West Neck Bay, Long Island, New York. J. Phycol. 39, 850–854 (2003).
Collado-Fabbri, S., Vaulot, D. & Ulloa, O. Structure and seasonal dynamics of the eukaryotic picophytoplankton community in a wind-driven coastal upwelling ecosystem. Limnol. Oceanogr. 56, 2334–2346 (2011).
Six, C., Finkel, Z., Rodríguez, F. & Marie, D. Contrasting photoacclimation costs in ecotypes of the marine eukaryotic picoplankter Ostreococcus. Limnol. Oceanogr. 53, 255–265 (2008).
Rodríguez, F. et al. Ecotype diversity in the marine picoeukaryote Ostreococcus (Chlorophyta, Prasinophyceae). Environ. Microbiol. 7, 853–9 (2005).
Subirana, L. et al. Morphology, genome plasticity, and phylogeny in the genus ostreococcus reveal a cryptic species, O. mediterraneus sp. nov. (Mamiellales, Mamiellophyceae). Protist 164, 643–59 (2013).
Six, C., Sherrard, R., Lionard, M., Roy, S. & Campbell, D. A. Photosystem II and pigment dynamics among ecotypes of the green alga Ostreococcus. Plant Physiol. 151, 379–390 (2009).
Demir-Hilton, E. et al. Global distribution patterns of distinct clades of the photosynthetic picoeukaryote Ostreococcus. ISME J. 5, 1095–107 (2011).
Price, N. M. et al. Preparation and Chemistry of the Artificial Algal Culture Medium Aquil. Biol. Oceanogr. 6, 443–461 (1989).
Sutak, R. et al. A comparative study of iron uptake mechanisms in marine microalgae: iron binding at the cell surface is a critical step. Plant Physiol. 160, 2271–2284 (2012).
Botebol, H. et al. Different iron sources to study the physiology and biochemistry of iron metabolism in marine micro-algae. Biometals 27, 75–88 (2014).
Smith, P., Krohn, R. & Hermanson, G. Measurement of protein using bicinchoninic acid. Anal. Biochem. 150, 76–85 (1985).
Moulager, M. et al. Light-dependent regulation of cell division in Ostreococcus: evidence for a major transcriptional input. Plant Physiol. 144, 1360–1369 (2007).
Grabherr, M. G. et al. Full-length transcriptome assembly from RNA-Seq data without a reference genome. Nat. Biotechnol. 29, 644–52 (2011).
Langmead, B., Trapnell, C., Pop, M. & Salzberg, S. L. Ultrafast and memory-efficient alignment of short DNA sequences to the human genome. Genome Biol. 10, R25 (2009).
Quinlan, A. R. & Hall, I. M. BEDTools: A flexible suite of utilities for comparing genomic features. Bioinformatics 26, 841–842 (2010).
Anders, S. & Huber, W. Differential expression analysis for sequence count data. Genome Biol. 11, R106 (2010).
Camacho, C. et al. BLAST command line applications user manual. BLAST® Help. Bethesda, MD Natl. Cent. Biotechnol. Inf. (2008).
Courties, C., Vaquer, A. & Troussellier, M. Smallest eukaryotic organism. Nature 370, 255 (1994).
Claustre, H. et al. Is desert dust making oligotrophic waters greener? Geophys. Res. Lett. 29(107), 1–4 (2002).
Partensky, F., Blanchot, J., Lantoine, F., Neveux, J. & Marie, D. Vertical structure of picophytoplankton at different trophic sites of the tropical northeastern Atlantic Ocean. Deep Sea Res. Part I Oceanogr. Res. Pap. 43, 1191–1213 (1996).
Guieu, C. et al. Impact of high Saharan dust inputs on dissolved iron concentrations in the Mediterranean Sea. Geophys. Res. Lett. 29, 2–5 (2002).
Mills, M. M., Ridame, C., Davey, M., La Roche, J. & Geider, R. J. Iron and phosphorus co-limit nitrogen fixation in the eastern tropical North Atlantic. Nature 429, 292–294 (2004).
Monnier, A. et al. Orchestrated transcription of biological processes in the marine picoeukaryote Ostreococcus exposed to light/dark cycles. BMC Genomics 11, 192 (2010).
Lommer, M. et al. Genome and low-iron response of an oceanic diatom adapted to chronic iron limitation. Genome Biol. 13, R66 (2012).
Nunn, B. L. et al. Diatom proteomics reveals unique acclimation strategies to mitigate fe limitation. PLoS One 8, e75653 (2013).
Gan, L., Ladinsky, M. S. & Jensen, G. J. Organization of the smallest eukaryotic spindle. Curr. Biol. 21, 1578–1583 (2011).
Murata, N., Takahashi, S., Nishiyama, Y. & Allakhverdiev, S. I. Photoinhibition of photosystem II under environmental stress. Biochim. Biophys. Acta (BBA)-Bioenergetics 1767, 414–421 (2007).
Ling, H.-Q., Bauer, P., Bereczky, Z., Keller, B. & Ganal, M. The tomato fer gene encoding a bHLH protein controls iron-uptake responses in roots. Proc. Natl. Acad. Sci. USA 99, 13938–13943 (2002).
Guillou, L. et al. Diversity of picoplanktonic prasinophytes assessed by direct nuclear SSU rDNA sequencing of environmental samples and novel isolates retrieved from oceanic and coastal marine ecosystems. Protist 155, 193–214 (2004).
Sunda, W. G. & Huntsman, S. A. Iron uptake and growth limitation in oceanic and coastal phytoplankton. Mar. Chem. 50, 189–206 (1995).
Funding is acknowledged from ANR “PhytoIron” (ANR 11BSV7 018 02) to F.Y.B. and E.L. H.B. was supported by a fellowship from the Institut National des Sciences de l’Univers (INSU CNRS). We thank Audrey Gueuneugues for help with preparing Aquil Medium.
The authors declare that they have no competing interests.
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Botebol, H., Lelandais, G., Six, C. et al. Acclimation of a low iron adapted Ostreococcus strain to iron limitation through cell biomass lowering. Sci Rep 7, 327 (2017). https://doi.org/10.1038/s41598-017-00216-6
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