Comparative quantitative proteomics of prochlorococcus ecotypes to a decrease in environmental phosphate concentrations

Matthew A Fuszard; Phillip C Wright; Catherine A Biggs

doi:10.1186/2046-9063-8-7

Research

Open Access

Comparative quantitative proteomics of prochlorococcus ecotypes to a decrease in environmental phosphate concentrations

Matthew A Fuszard¹,
Phillip C Wright¹ and
Catherine A Biggs¹Email author

Aquatic Biosystems20128:7

https://doi.org/10.1186/2046-9063-8-7

Received: 8 November 2011

Accepted: 19 March 2012

Published: 19 March 2012

Abstract

Background

The well-lit surface waters of oligotrophic gyres significantly contribute to global primary production. Marine cyanobacteria of the genus Prochlorococcus are a major fraction of photosynthetic organisms within these areas. Labile phosphate is considered a limiting nutrient in some oligotrophic regions such as the Caribbean Sea, and as such it is crucial to understand the physiological response of primary producers such as Prochlorococcus to fluctuations in the availability of this critical nutrient.

Results

Prochlorococcus strains representing both high light (HL) (MIT9312) and low light (LL) (NATL2A and SS120) ecotypes were grown identically in phosphate depleted media (10 μM P_i). The three strains displayed marked differences in cellular protein expression, as determined by high throughput large scale quantitative proteomic analysis. The only strain to demonstrate a significantly different growth rate under reduced phosphate conditions was MIT9312. Additionally, there was a significant increase in phosphate-related proteins such as PhoE (> 15 fold increase) and a depression of the Rubisco protein RbcL abundance in this strain, whereas there appeared to be no significant change within the LL strain SS120.

Conclusions

This differential response between ecotypes highlights the relative importance of phosphate availability to each strain and from these results we draw the conclusion that the expression of phosphate acquisition mechanisms are activated at strain specific phosphate concentrations.

Keywords

Prochlorococcus PstSPhoAPhoEGrowthPhosphate

Background

Within marine oligotrophic systems, such as central subtropical gyres, orthophosphate (P_i) is a crucial macronutrient governing microbial population densities, particularly within the well-lit surface waters of the euphotic zone [1–3]. The principal photosynthetic organism numerically dominating these areas is Prochlorococcus, which is estimated to represent about 50% of all photosynthetic activity within them [4, 5]. Prochlorococcus has been broadly delineated into two clades, or ecotypes, high light (HL) and low light (LL) based upon the ratios of divinylchlorophylla and b within their light harvesting apparatuses and as such their assumed depth within the water column [6, 7]. Further clade subdivisions have been implemented through phylogenetic analyses of 16S rRNA sequences [8]. As a taxon, Prochlorococcus is characterised by its small size (~ 1 μm³), and significantly reduced genomes which ranges from 1.64 Mbps (the HL strain MIT9301) to 2.68 Mbps (the LL strain MIT9303) [9]. This diminished volume and genome is hypothesised to be the result of an accelerated evolutionary process adapting to reduced phosphorus in its environment [10, 11]. Indeed, Prochlorococcus is known to replace phospholipids in its membranes with sulpholipids, which dramatically reduce its P_i requirements [12].

Given the importance of P_i to Prochlorococcus, perhaps it is surprising to find no significant correlation between ecotype distribution and P_i concentration [13]. However, fluxes in P_i transport within these regions are important considerations, which could help to explain the discrepancy. Nevertheless the observation of a large number of known P_i acquisition genes in some LL ecotypes (i.e. MIT9313 and NATL2A), and not others (i.e. SS120) [14, 15] is confusing. Indeed, P_i acquisition genes are present in some HL strains (i.e. MED4) and not others (i.e. MIT9515) [14]. However it was recently observed that the prevalence of Prochlorococcus genes involved in acquisition of phosphate substrates were correlated with areas of low P_i such as the Caribbean Sea and NW Mediterranean [16]. This conflict is likely resolved due to the presence of hypervariable genomic islands within Prochlorococcus, allowing for evolutionarily rapid niche adaptation [17]. Given this, it was hypothesised that the presence or absence of these genes could directly affect the protein content of cells when P_i stressed, and as such directly affect the ability of a strain to acclimate to environmental P_i fluctuations [16]. So the question arises, how effective are cells with and without these genes at acclimating to a shift in environmental P_i? Indeed, the levels of mRNA transcripts of two strains, MED4 and MIT9313, which both contain the two component response regulation system phoBR, behaved quite differently to P_i starvation [14].

To address this we selected three strains, MIT9312, NATL2A and SS120, each representative of an ecotype and a position within the water column (Table 1). MIT9312 is a HLII strain isolated at depth from the Gulf Stream. NATL2A is a LLI strain isolated from the North Atlantic which contains most of the P_i acquisition genes found in MED4 and MIT9312, and yet is thought to experience both high and low light environments due to storm mixing events. SS120, originally isolated in the Sargasso Sea, does not possess phoBR, yet has two copies of the periplasmic phosphate binding protein, PstS. We took these three strains and allowed cells to acclimate to a significant reduction in environmental P_i and investigated their respective protein contents.

Table 1

Details of the strains used in this study, as obtained from NCBI and CCMP.

Strain and genome details
			Genome	Protein	%GC	Chl b/a	Ecotypic
Strain	Refseq	Reference	size (Mbp)	coding		ratio	clade
MIT9312	NC_007577	[18]^a	1.71	1810	31	0.34	HLII
NATL2A	NC_007335	[19]	1.84	2162	35	0.97	LLI
SS120	NC_005042	[20]	1.75	1883	36	1.41	LLII
P acquisition mechanisms
	PhoBR cluster	PtrA cluster	PhoA	PhoE	PstS cluster	ArsA cluster	ArsB cluster	ArsC cluster
MIT9312	√	x	√	√	√	√	x	√
NATL2A	√	√	√	√	√	√	x	√
SS120	x	√	x	x	(2)	x	x	√
Isolation details and culture conditions
	Location	Depth	Isolated by	Date	Culture temp (°C)	Deposited in	Media
MIT9312	Gulf stream	135 m	L. Moore	17/07/1993	22-26	CCMP	Pro99
NATL2A	N. Atlantic	10 m	D. Scanlan	01/04/1990	18-22	CCMP	Pro99
SS120	Sargasso Sea	120 m	S. Frankel & L West-Johnsrud	01/01/1991	18-22	CCMP	Pro99

^a indicates that the genome sequence has been submitted, yet not cleared. Ticks in 'P acquisition mechanisms' indicates presence of gene/cluster, and copies are in parentheses

Results and discussion

Overview

The experimental growth data for each strain under P_i replete and P_i deplete cultures is shown in Figure 1. Logistic curve fitting and statistical analysis of the experimental growth data reveals no significant differences between the growth rates between P_i replete and P_i deplete cultures, with the exception of MIT9312 growth rates whereby P_i replete growth was significantly greater than P_i deplete growth (p < 0.05), as can be seen in Figure 1. It is important to consider the physiological status of the cells at the harvest point when considering protein relative abundances. Importantly, growth analysis shows that both MIT9312 and SS120 were in late exponential/early stationary phase at harvest, whilst NATL2A was in mid exponential phase. As the point of harvest differs for NATL2A, it would be difficult to directly compare the protein complement of NATL2A cells to either MIT9312 or SS120. Given this, the results for NATL2A will be discussed separately.

Figure 1
**Experimental growth curves of MIT9312, NATL2A and SS120 within P**_ireplete (circles) and P_ideplete (triangles) media. Error bars represent one standard error. Growth rates (μ) are given with ± standard error.

Thirty eight, 63 and 34 proteins were identified with 2 or more peptides for strains MIT9312, NATL2A and SS120 respectively (Additional file 1: Table S1) with no false positives. An overview of the respective proteomes, through plotting theoretical values of isoelectric points (pI) against molecular weights (MW) reveal significant bias towards low pI values (Additional file 2: Figure S1), with no further correlation to MW, relative protein abundance, nor total peptide hits per protein (data not shown). This bias may be an artefact of the mass spectrometric analysis, where peptides are protonated directly before entry into the MS in order to assist flight and detection. As a consequence, naturally occurring proton-donor peptides may be preferentially selected. However, as there are no observable correlations between pI and peptide hits per protein, we can be confident that the intracellular protein abundances reported are directly reflective of the physiological status of the cells. Indeed, when interrogating the proportion of proteins with ≥ 50% of peptide hits, we see similarities between strains, such as the presence of RplL, RbcL and CsoS1 (Additional file 1: Table S1), however all three proteins have pI values < 7. Nevertheless, a high pI protein, PetH, is present in both MIT 9312 and SS120 samples. Also, identified proteins from all three strains are located evenly across the genomes, and are representative of most major functional groups such as central metabolism, photosynthesis, transcription and translation, biosynthesis and nutrient acquisition (Figure 2A). Of the 105 unique proteins identified, 6 were found in all three strains (Figure 2B). They are the ATP synthase subunits AtpA and AtpD, the PSII protein PsbO, the nitrogen regulatory protein GlnK, rubisco subunit RbcL, and the carboxysome shell protein CsoS1.

Figure 2
**(A) Distribution of proteins identified in all three strains within functional categories ('Trans' stands for 'Transcription, translation and stress')**. Light hatching represents proteins significantly more abundant than the control, and dark hatching represents proteins significantly less abundant than the control. (B) Venn diagram of all unique proteins specific to, or shared between, the strains.

Using relative abundance cut-offs of 1.6 and 0.6 fold differences to represent increased or decreased relative abundances [21, 22], 4 proteins were more abundant in MIT9312 and 4 were less abundant than the replete cultures. Within NATL2A, 6 proteins were more abundant and 1 was less abundant than the replete cultures. In SS120, 4 were more abundant and none were lower than the replete cultures (Figure 2A).

Nutrient acquisition

What is immediately apparent from our results is the differential abundance of P_i acquisition proteins exhibited by all three strains to being grown in 10 μM P_i. MIT 9312 demonstrates the greatest sensitivity to P_i-deplete media, whereby the P_i stress related porinPhoE is > 15-fold more abundant (Figure 3), the putative alkaline phosphatase PhoA appears to be > 9-fold greater, and the periplasmic P_i binding protein PstS > 3 times more than the replete cultures. This result is directly in line with an earlier proteomic assay of P stress in a HL ecotype, MED4 [21], and closely reflective of microarray analyses of both MED4 and MIT9313 [14], Synechococcucs WH8102 [23], measured alkaline phosphatase activity of MIT9312 [15] and in line with observed responses within earlier P_i depletion studies of other cyanobacteria [15, 24–26].

Within NATL2A, PstS abundance is significantly greater within P_i-deplete conditions, though with greater uncertainty (Additional file 1: Table S1). However neither PhoA nor PhoE was observed with mass spectrometry here, which is surprising as we showed previously that both PhoA and PhoE are greater in abundance alongside PstS in the high light ecotype MED4 [21], as is true with MIT9312 in this study. However, considering that NATL2A cells are in mid-exponential phase as opposed to early stationary phase this may indicate a progressive strategy of protein expression within the cells, however more work is needed to clarify this.

What was also unexpected, was the absence of any P_i acquisition mechanisms (as reflected in observed peptide identifications) within SS120 cells (Additional file 1: Table S1), allied with no significant difference in growth rates between P_i-replete and P_i-deplete cultures (p > 0.05). SS120 is deficient in most P_i acquisition genes [14, 15], however it does have two copies of PstS, neither of which were present in our assay. At first glance, this result appears counter-intuitive, as a 'very' LL strain typically present in vivo within P_i-replete environments would be expected to be adversely affected by a substantial decrease in P_i. However, the absence of a phoBRregulon suggests that the strain is incapable of regulating a response to shifts in environmental concentrations of P_i that are not immediately starvation inducing [27]. Curiously, this also infers that activation of the phoBR response mechanisms within MIT9312 and NATL2A were directly due to the mechanism's innate sensitivity to changing external P_i concentrations. This suggests that the intensity of response is directly proportional to external P_i concentration, coincidentally specific to each strain, and may be reflective of each strain's environmental niche and/or obligate cellular requirements.

Photosynthesis, biosynthesis and central metabolism

The exposure of all three strains to lower P_i concentrations appears to have had little effect upon the photosynthetic machinery (Figure 4A and Additional file 1: Table S1). This is unusual, as P_i depleted conditions have been previously noted to directly affect both photosystems in cyanobacteria [21, 23, 28]. In contrast, it is interesting to note that, for MIT9312, both Rubisco subunits (RbcL and RbcS) are noticeably lower in abundance (Figure 3B). This suggests that there is a progressive strategy within the cell when acclimating to lowered P_i, whereby photosynthesis is initially dissociated from glycolysis, to then strategically break down the photosynthetic apparatus. This is a reasonable conclusion, considering a P_i-induced organised break down of phycobilisomes has been previously observed in Synechococcus sp. PCC 7942 [29], chlorosis has been observed in thermophillicSynechococcus under P_i-stress [28], and a strategic approach to a reduction in photosynthetic function has been hypothesised in MED4 [21]. Indeed, within WH8102 it appears that PSII was degraded before PSI, allowing continued cyclic photophosphorylation-based ATP generation to continue [23]. In this context, this could explain why an essential chlorophyll biosynthetic protein (ChlP) appears to be less abundant within P_i-deplete MIT9312 cells (Figure 4B). However, it would be parsimonious to also expect a concurrent reduction in the light harvesting protein (Pcb) within P_i-deplete MIT9312, which was noticed in MED4 [21], but there is no change. The reason for this is not clear.

Figure 4
**Relative abundances of proteins associated with (A) photosynthesis, (B) biosynthesis, (C) uncategorised and (D) transcription, translation and stress from MIT9312 (blue circles) and SS120 (crosses)**. Dotted lines represent the abundance limits of 1.6 and 0.6. Error bars represent one standard error.

When considering NATL2A solely, there appear to be a few subtle discrepancies in protein abundances between stressed and non-stressed cultures. Fumerase (FumC) is an enzyme associated with both the tricarboxylic acid (TCA) cycle and arginine/proline biosynthesis, and appears to be more abundant within NATL2A cells when P_i-deplete (Additional file 1: Table S1). As NATL2A has an incomplete TCA cycle, it is safe to assume that its function within the cell is within arginine and proline metabolism. Also, the acyl carrier protein (AcpP) is an essential component of fatty acid biosynthesis, and is more abundant in P_i-deplete NATL2A cells (Additional file 1: Table S1). Fatty acids are for the most part used within either fuel storage or membrane manufacture. However it may be misleading to arrive at the conclusion that this is a specific cellular response to lower P_i concentrations. It is possibly a function of apparently slightly elevated (albeit not significant) growth within NATL2A P_i-deplete cultures, and as such could reflect comparatively greater metabolic activity. Nevertheless, this explanation cannot immediately address the lower abundance of CobJ, a Precorrin-3B C17-methyltransferase region-containing protein (Additional file 1: Table S1), part of the aerobic vitamin B12 biosynthesis pathway within P_i-stressed cells. However, B12 synthesis is a sub pathway offshoot from the main chlorophyll biosynthetic pathway, and as such may reflect a metabolic preference for chlorophyll production that, again, may be representative of faster growing populations.

An interesting observation is the abundance of CitT within P_i-stressed SS120 cells (Figure 3A). This protein functions as a di/tricarboxylate transporter, which implies that the cells are scavenging lysed cellular material from the environment. That stressed SS120 cells appear to be preferentially acquiring tricarboxylic acid intermediates when growing in P_i-deplete conditions, and not upregulatingPstS, is puzzling. However, it may indicate that this strain may be supplementing an affected glycolysis pathway through acquiring external carbon sources, and that this is more evidence that the cells response to an environmental stress is an iterative, evolving process. SS120 may simply have not initiated transcription of PstS in sufficiently detectable quantities. Indeed, even in starvation experiments pstSexperession is far from an immediate response [14, 23].

Other proteins

An interesting observation is the presence of LuxR, the response regulatory family protein involved in quorum sensing within bacteria, in NATL2A cells (Additional file 1: Table S1). To our knowledge, this is the first instance of observing proteins putatively indicated in quorum sensing capability in any marine cyanobacteria. However, we were unable to locate any LuxI homologues, an essential protein required for effective quorum sensing, within NATL2A (data not shown). However LuxR is known to be a transcriptional regulator activated when cell concentrations of a particular trigger compound (usually N-(3-oxohexanoyl)-_L-homoserine lactone, which is generated through the enzymatic functioning of LuxI) reach particular levels. As such, we speculate that the protein acts as a density-dependant transcriptional regulator, but for an unknown function, and through another trigger compound.

Conclusions

Prochlorococcus are now widely considered to be evolutionarily adept at environmental niche domination, particularly within nutrient poor oligotrophic waters. The genus is typified by genomes characterised by hypervariable genomic islands [17], which are thought to contain genes obtained through phage-mediated horizontal gene transfer, and infer niche-specific advantages such as nutrient acquisition and phage resistance. Our results reinforce previous results concerning the importance of phosphate concentrations to specific strains, but also highlight the possibility of the cells employing a progressive acclimation strategy. It appears that Prochlorococcus strains evolutionarily adapted to life in a P_i-deplete environment respond to phosphate fluctuations through a succession of cellular processes, such as the upregulation of P_i acquisition mechanisms, a dissociation of photosynthesis from central metabolic pathways, and a staggered breakdown of the photosystems allowing prolonged photophosphorylated ATP generation. This progressive response allows the cell to react quickly to any subsequent increases in ambient P_i concentrations. It is our hypothesis that HL strains are also particularly sensitive to changes in P_i, and that ambient phosphate concentrations initiate a strong response regardless of being predominantly growth limited elsewhere.

We also note that our results strongly infer that the induction of P_i acquisition mechanisms are concentration specific between strains, particularly considering the absence of any stress response of the LL strain SS120 compared to MIT9312 when grown from identical initial concentration levels.

Methods

For a complete description of the Materials and Methods used please refer to the (Additional file 3: Material and Methods). In brief, however, biological triplicates of all three strains (MIT9312, NATL2A and SS120 (CCMP, Maine)) were grown under 2 separate conditions: P_i replete (Pro99 media with 50 μM NaH₂PO₄ [30]) and P_i deplete (Pro99 media with 10 μM NaH₂PO₄), and moderate white light intensities (30, 10 and 20 μE m^-2 s^-1 respectively), in a 13:11 h light:dark regime at 23°C.

For the proteomic analysis, the cells were harvested once measured optical densities reached 0.4 (after which populations had been observed to crash), and proteins were extracted from the three biological replicates for each phenotype [31]. 100 μg of protein from each replicate was then reduced, alkylated, digested and labelled with 8-plex iTRAQ reagents according to the manufacturer's (ABSciex, Framingham, MA) protocol. The labelled replicates were then pooled before primary strong cation exchange (SCX) fractionation [21]. Mass spectrometric analysis of the SCX fractions was performed with a QStar XL Hybrid ESI Quadrupole time-of-flight tandem mass spectrometer, ESI-qQ-TOF-MS/MS (Applied Biosystems; MDS Sciex, Concord, Ontario, Canada), coupled with an online capillary liquid chromatography system (Ultimate 3000, Dionex/LC Packings, The Netherlands) [21, 22]. Preliminary data analysis, protein identification and quantitation were carried out using the PHENYX [Geneva Bioinformatics (GeneBio), Geneva, Switzerland] software platform.

Declarations

Acknowledgements

The authors wish to acknowledge the provision of an EPSRC studentship, Advanced Research Fellowship for CAB (EP/E053556/01) and further EPSRC funding (GR/S84347/01 and EP/E036252/1). We also acknowledge the Provasoli-Guillard National Center for Culture of Marine Phytoplankton for the kind provision of cells. Thanks also to Adam Martiny for additional input.

Electronic supplementary material

12999_2011_8_MOESM1_ESM.XLS Additional file 1: Table S1. Full list of identified proteins and peptides for all 3 strains used in this study. (XLS 130 KB)

12999_2011_8_MOESM2_ESM.DOC Additional file 2: Figure S1. Virtual 2D gel representations of proteins identified from MIT9312 (top left), NATL2A (top right), and SS120 (bottom left). (DOC 246 KB)

12999_2011_8_MOESM3_ESM.DOC Additional file 3: Materials and methods [32–34]. (DOC 49 KB)

Below are the links to the authors’ original submitted files for images.

12999_2011_8_MOESM4_ESM.pdf Authors’ original file for figure 1

12999_2011_8_MOESM5_ESM.pdf Authors’ original file for figure 2

12999_2011_8_MOESM6_ESM.pdf Authors’ original file for figure 3

12999_2011_8_MOESM7_ESM.pdf Authors’ original file for figure 4

Authors’ Affiliations

(1)

ChELSI Institute, Department of Chemical and Biological Engineering, University of Sheffield, Sheffield, UK

References

Ammerman JW, Hood RR, Case DA, Cotner JB: Phosphorus deficiency in the Atlantic: An emerging paradigm in oceanography. Eos Trans Am Geophys Union. 2003, 84: 165-170.View ArticleGoogle Scholar
Thingstad TF, Krom MD, Mantoura RF, et al: Nature of phosphorus limitation in the ultraoligotrophic eastern Mediterranean. Science. 2005, 309: 1068-1071. 10.1126/science.1112632.View ArticleGoogle Scholar
Thingstad TF, Zweifel UL, Rassoulzadegan F: P limitation of heterotrophic bacteria and phytoplankton in the northwest Mediterranean. Limnol Oceanogr. 1998, 43: 88-94. 10.4319/lo.1998.43.1.0088.View ArticleGoogle Scholar
Chisholm SW, Olson RJ, Zettler ER, Goericke R, Waterbury JB, Welschmeyer NA: A novel free-living prochlorophyte abundant in the oceanic euphotic zone. Nature. 1988, 334: 340-343. 10.1038/334340a0.View ArticleGoogle Scholar
Partensky F, Hess WR, Vaulot D: Prochlorococcus, a marine photosynthetic prokaryote of global significance. Microbiol Mol Biol Rev. 1999, 63: 106-127.Google Scholar
Moore LR, Chisholm SW: Photophysiology of the marine cyanobacterium Prochlorococcus: ecotypic differences among cultured isolates. Limnol Oceanogr. 1999, 44: 628-638. 10.4319/lo.1999.44.3.0628.View ArticleGoogle Scholar
Moore LR, Rocap G, Chisholm SW: Physiology and molecular phylogeny of coexisting Prochlorococcus ecotypes. Nature. 1998, 393: 464-467. 10.1038/30965.View ArticleGoogle Scholar
Rocap G, Distel DL, Waterbury JB, Chisholm SW: Resolution of Prochlorococcus and Synechococcus ecotypes by using 16S-23S ribosomal DNA internal transcribed spacer sequences. Appl Environ Microbiol. 2002, 68: 1180-1191. 10.1128/AEM.68.3.1180-1191.2002.View ArticleGoogle Scholar
Partensky F, Garczarek L: Prochlorococcus: Advantages and Limits of Minimalism. Ann Rev Marine Sci. 2009, 2: 305-331.View ArticleGoogle Scholar
Coleman ML, Chisholm SW: Ecosystem-specific selection pressures revealed through comparative population genomics. ProcNatlAcadSci. 2010, 107: 18634-18639.View ArticleGoogle Scholar
Dufresne A, Garczarek L, Partensky F: Accelerated evolution associated with genome reduction in a free-living prokaryote. Genome Biol. 2005, 6: R14-10.1186/gb-2005-6-2-r14.View ArticleGoogle Scholar
Van Mooy BA, Rocap G, Fredricks HF, Evans CT, Devol AH: Sulfolipids dramatically decrease phosphorus demand by picocyanobacteria in oligotrophic marine environments. Proc Natl Acad Sci USA. 2006, 103: 8607-8612. 10.1073/pnas.0600540103.View ArticleGoogle Scholar
Johnson ZI, Zinser ER, Coe A, McNulty NP, Woodward EM, Chisholm SW: Niche partitioning among Prochlorococcus ecotypes along ocean-scale environmental gradients. Science. 2006, 311: 1737-1740. 10.1126/science.1118052.View ArticleGoogle Scholar
Martiny AC, Coleman ML, Chisholm SW: Phosphate acquisition genes in Prochlorococcus ecotypes: evidence for genome-wide adaptation. Proc Natl Acad Sci USA. 2006, 103: 12552-12557. 10.1073/pnas.0601301103.View ArticleGoogle Scholar
Moore LR, Ostrowski M, Scanlan DJ, Feren K, Sweetsir T: Ecotypic variation in phosphorus-acquisition mechanisms within marine picocyanobacteria. AquatMicrobEcol. 2005, 39: 257-269.Google Scholar
Martiny AC, Huang Y, Li W: Occurrence of phosphate acquisition genes in Prochlorococcus cells from different ocean regions. Environ Microbiol. 2009, 11: 1340-1347. 10.1111/j.1462-2920.2009.01860.x.View ArticleGoogle Scholar
Coleman ML, Sullivan MB, Martiny AC, Steglich C, Barry K, Delong EF, Chisholm SW: Genomic islands and the ecology and evolution of Prochlorococcus. Science. 2006, 311: 1768-1770. 10.1126/science.1122050.View ArticleGoogle Scholar
Copeland A, Lucas S, Lapidus A, Barry K, Detter JC, Hammon N, Israni S, Pitluck S, Thiel J, Schmutz J, Larimer F, Land M, Kyrpides N, Lykidis A, Richardson P: Complete sequence of Prochlorococcus marinus str. MIT. 2005, 9312-UnpublishedGoogle Scholar
Kettler GC, Martiny AC, Huang K, Zucker J, Coleman ML, Rodrigue S, Chen F, Lapidus A, Ferriera S, Johnson J, et al: Patterns and implications of gene gain and loss in the evolution of Prochlorococcus. PLoS Genet. 2007, 3: e231-10.1371/journal.pgen.0030231.View ArticleGoogle Scholar
Dufresne A, Salanoubat M, Partensky F, Artiguenave F, Axmann IM, Barbe V, Duprat S, Galperin MY, Koonin EV, Le Gall F, Makarova KS, Ostrowski M, Oztas S, Robert C, Rogozin IB, Scanlan DJ, Tandeau de Marsac N, Weissenbach J, Wincker P, Wolf YI, Hess WR: Genome sequence of the cyanobacterium Prochlorococcus marinus SS120, a nearly minimal oxyphototrophic genome. Proc Natl Acad Sci USA. 2003, 100 (17): 10020-10025. 10.1073/pnas.1733211100.View ArticleGoogle Scholar
Fuszard MA, Wright PC, Biggs CA: Cellular acclimation strategies of a minimal picocyanobacterium to phosphate stress. FEMS MicrobiolLett. 2010, 306: 127-134. 10.1111/j.1574-6968.2010.01942.x.View ArticleGoogle Scholar
Pandhal J, Wright PC, Biggs CA: A quantitative proteomic analysis of light adaptation in a globally significant marine cyanobacterium Prochlorococcus marinus MED4. J Proteome Res. 2007, 6: 996-1005. 10.1021/pr060460c.View ArticleGoogle Scholar
Tetu SG, Brahamsha B, Johnson DA, Tai V, Phillippy K, Palenik B, Paulsen IT: Microarray analysis of phosphate regulation in the marine cyanobacterium Synechococcus sp. WH8102. ISME J. 2009, 3: 835-849. 10.1038/ismej.2009.31.View ArticleGoogle Scholar
Huber AL, Hamel KS: Phosphatase activities in relation to phosphorus nutrition in Nodularia spumigen (Cyanobacteriaceae). Hydrobiologia. 1985, 123: 81-88. 10.1007/BF00006617.View ArticleGoogle Scholar
Natesan R, Shanmugasundaram S: Extracellular phosphate solubilization by the cyanobacterium Anabaena ARM310. J Biosci. 1989, 14: 203-208. 10.1007/BF02716680.View ArticleGoogle Scholar
Scanlan DJ, Mann NH, Carr NG: The response of the picoplanktonic marine cyanobacterium Synechococcus species WH7803 to phosphate starvation involves a protein homologous to the periplasmic phosphate-binding protein of Escherichia coli. Mol Microbiol. 1993, 10: 181-191. 10.1111/j.1365-2958.1993.tb00914.x.View ArticleGoogle Scholar
Scanlan DJ, West NJ: Molecular ecology of the marine cyanobacterial genera Prochlorococcus and Synechococcus. FEMS Microbiol Ecol. 2002, 40: 1-12. 10.1111/j.1574-6941.2002.tb00930.x.View ArticleGoogle Scholar
Adams MM, Gomez-Garcia MR, Grossman AR, Bhaya D: Phosphorus Deprivation Responses and Phosphonate Utilization in a Thermophilic Synechococcus sp. from Microbial Mats. J Bacteriol. 2008, 190: 8171-8184. 10.1128/JB.01011-08.View ArticleGoogle Scholar
Collier JL, Grossman AR: Chlorosis induced by nutrient deprivation in Synechococcus sp. strain PCC 7942: not all bleaching is the same. J Bacteriol. 1992, 174: 4718-4726.Google Scholar
Moore LR, Post AF, Rocap G, Chisholm SW: Utilization of Different Nitrogen Sources by the Marine Cyanobacteria Prochlorococcus and Synechococcus. LimnolOceanogr. 2002, 47: 989-996.Google Scholar
Meijer EA, Wijffels RH: Development of a Fast, Reproducible and Effective Method for the Extraction and Quantification of Proteins of Micro-algae. Biotechnol Tech. 1998, 12: 353-358. 10.1023/A:1008814128995.View ArticleGoogle Scholar
Moore LR, Goericke R, Chisholm SW: Comparative physiology of Synechococcus and Prochlorococcus: Influence of light and temperature on growth, pigments, fluorescence and absorptive properties. Mar Ecol Prog Ser. 1995, 116: 259-276.View ArticleGoogle Scholar
Ow SY, Noirel J, Cardona T, Taton A, Lindblad P, Stensjo K, Wright PC: Quantitative Overview of N2 Fixation in Nostoc punctiforme ATCC 29133 through Cellular Enrichments and iTRAQ Shotgun Proteomics. Journal Proteome Research. 2009, 8: 187-198. 10.1021/pr800285v.View ArticleGoogle Scholar
Team RDC: R: A Language and Environment for Statistical Computing. 2011, R Foundation for Statistical Computing: Vienna, AustriaGoogle Scholar

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