Advertisement
Browse Subject Areas
?

Click through the PLOS taxonomy to find articles in your field.

For more information about PLOS Subject Areas, click here.

  • Loading metrics

Photoinactivation of Photosystem II in Prochlorococcus and Synechococcus

Photoinactivation of Photosystem II in Prochlorococcus and Synechococcus

  • Cole D. Murphy, 
  • Mitchell S. Roodvoets, 
  • Emily J. Austen, 
  • Allison Dolan, 
  • Audrey Barnett, 
  • Douglas A. Campbell
PLOS
x

Abstract

The marine picocyanobacteria Synechococcus and Prochlorococcus numerically dominate open ocean phytoplankton. Although evolutionarily related they are ecologically distinct, with different strategies to harvest, manage and exploit light. We grew representative strains of Synechococcus and Prochlorococcus and tracked their susceptibility to photoinactivation of Photosystem II under a range of light levels. As expected blue light provoked more rapid photoinactivation than did an equivalent level of red light. The previous growth light level altered the susceptibility of Synechococcus, but not Prochlorococcus, to this photoinactivation. We resolved a simple linear pattern when we expressed the yield of photoinactivation on the basis of photons delivered to Photosystem II photochemistry, plotted versus excitation pressure upon Photosystem II, the balance between excitation and downstream metabolism. A high excitation pressure increases the generation of reactive oxygen species, and thus increases the yield of photoinactivation of Photosystem II. Blue photons, however, retained a higher baseline photoinactivation across a wide range of excitation pressures. Our experiments thus uncovered the relative influences of the direct photoinactivation of Photosystem II by blue photons which dominates under low to moderate blue light, and photoinactivation as a side effect of reactive oxygen species which dominates under higher excitation pressure. Synechococcus enjoyed a positive metabolic return upon the repair or the synthesis of a Photosystem II, across the range of light levels we tested. In contrast Prochlorococcus only enjoyed a positive return upon synthesis of a Photosystem II up to 400 μmol photons m-2 s-1. These differential cost-benefits probably underlie the distinct photoacclimation strategies of the species.

Introduction

Synechococcus and Prochlorococcus picocyanobacteria numerically dominate the open ocean phytoplankton community [1,2]. Synechococcus is most abundant in mesotrophic open ocean surface waters and coastal regions, and at lower abundances in nutrient-depleted areas [1,3]. Strains of Synechococcus tolerate a range of temperatures [4,5] and can thus extend to high latitudes. Synechococcus strains also vary in pigment composition allowing them to exploit different spectral niches [6,7]. Prochlorococcus is adapted to warm, stratified, oligotrophic tropical, and subtropical marine areas [1,8]. In areas where Synechococcus and Prochlorococcus co-occur, Prochlorococcus is typically more abundant. The two species have a high surface to volume ratio due to their small diameters of 0.5–0.8 μm for Prochlorococcus and 0.8–1.2 μm for Synechococcus. The smaller size of Prochlorococcus minimizes pigment package effects [9,10] giving it high optical absorption efficiency per pigment, that allows it to live deep in the water column, down to 200m [6,11]. This is optimal for photon capture but also leaves them vulnerable to photo-induced damage [12,13] since they lack the optical thickness for pigment screening [10]. Thus in addition to their ecological prominence Synechococcus and Prochlorococcus are intriguing minimal model species to study photosynthesis and photoacclimation in the absence of confounding biooptical complexities.

In oxygenic photoautotrophs pigment-proteins associated with Photosystem II (PSII) transfer excitation energy to the chlorophyll molecule P680, generating its excited state, P680* [14,15]. P680* then transfers the excited electron by reducing a phaeophytin (Phe) intermediate and drops to its oxidized ground state, P680+. The excited electrons are passed from Phe- to QA and then to bound plastoquinone molecule QB which migrates to join the mobile plastoquinone (PQ) pool of the thylakoid membrane, eventually passing the electrons to the Cytochrome b6f complex. The PQ pool can become saturated with electrons [4] if incoming excitation outruns downstream electron flow [1618]. The P680+ radical is a strong oxidant and can cause irreversible damage to its surrounding proteins and pigments if it is not quickly reduced [19] by electrons from water within the oxygen-evolving complex of PSII [1618].

Synechococcus and Prochlorococcus are characterized by different pigment-proteins to harvest light energy and protect PSII from photodamage. Synechococcus has an extra-membrane antenna complex, the phycobilisome, made up of phycocyanin rods that radiate from allophycocyanin core proteins. Core-membrane linker proteins bind the phycobilisome to the thylakoid membrane and transfer harvested light energy to chlorophyll a and carotenoids in the PSII complex [2022]. The connectivity of the phycobilisome to the reaction centre can be regulated in some strains of Synechococcus [23,24] by an orange-carotenoid protein which mediates non-photochemical quenching of excitation [22,23,25,26].

Prochlorococcus instead uses intra-membrane prochlorophyte chlorophyll binding (Pcb) proteins as its light-harvesting complex. The Pcb proteins contain chlorophyll derivatives, di-vinyl chlorophyll a and di-vinyl chlorophyll b, that are specific to Prochlorococcus and have slightly different, blue-enhanced absorption spectra compared to the mono-vinyl chlorophyll a found in Synechococcus [2729]. Prochlorococcus lacks the orange carotenoid protein but there is phenomenological evidence for some limited capacity for non-photochemical quenching even in Prochlorococcus [30] (K. Xu & D.A. Campbell, unpub.). Although non-photochemical quenching lowers the photochemical yield of PSII during periods of excess incident light, in cyanobacteria the non-photochemical quenching is relaxed within minutes upon return to more favorable light conditions [18,31]. In an alternate strategy cyanobacteria, including Prochlorococcus, can mediate pseudo-cyclic flows of electrons from PSII back to oxygen through multiple pathways [11,3239] to control feedback inhibition of electron transport and thus lower the risk of reactive oxygen species production.

Light is essential for oxygenic photosynthesis, and oxygen is a product, but both have the potential to damage PSII protein subunits. The PsbA protein subunit of PSII is particularly susceptible to irreversible damage leading to the inactivation of the PSII complex [40]. The oxygen evolving complex of PSII can be inactivated by a photon in the UV or blue range directly absorbed by the Mn4Ca cluster [41]. Without the oxygen evolving complex extracting electrons from water, the P680+ radical cannot be rapidly reduced and may cause irreversible oxidative damage to the PsbA protein through uncontrolled oxidation of amino acids [42,43]. In samples dominated by this photoinactivation mechanism the rate constant of photoinhibition increases linearly with increasing irradiance [44,45]. Furthermore, Mn absorbance in the visible range is sufficient to account for the quantum, “per-photon”, yield of photoinhibition [18,41,4648].

A second photoinactivation mechanism involves production of the reactive oxygen species singlet oxygen (1O2) [4852] by a a normal triplet-state oxygen molecule reacting with a triplet excited state sensitizer molecule, the 3P680 state of chlorophyll, yielding 1O2 and the singlet ground state of the sensitizer molecule, P680 [48,53]. As electrons are then passed from one molecule to the next of the photosynthetic electron transport chain, short-lived radical intermediate states are generated. In PSII, if electron acceptors are available, electron transfer will happen before the radical intermediate can interact with anything else [18]. However, as the PQ pool becomes fully reduced, forward electron transport may be blocked at the level of QA or QB [18,50,54,55]. After primary charge separation a short lived 3[P680+Pheo-] charge pair is formed in its triplet ground state [56,57]. 3P680 thus occurs even under normal conditions and increases when forward electron flow slows through limitations downstream of QA or QB [58,59]. Triplet chlorophyll, 3Chl, a functional equivalent of 3P680, also occurs in the PSII antenna light harvesting complex in reactions independent of electron transport events [18,52,54,60,61] but proportional to the effective size of the photosynthetic antenna, which determines the average duration of excitation migration through the antenna.

Both the direct absorbance and inactivation of the Mn4Ca complex and reactive oxygen dependent photoinactivations occur [41,55,62,63] but show differing responses to incident light. The extinction coefficient (or target size) for a photon hitting the Mn4Ca complex is constant and so the probability of a single photon causing a photoinactivation should be independent of incident light level, while the rate of photoinactivation should show a simple linear dependence upon treatment light level. Furthermore, because Mn has higher absorbance in the blue and UV wavelength range and low absorbance in the red wavelength range, the probability of a photoinactivation is higher for a blue photon than for a red photon, no matter the spectral properties of the light harvesting antenna [18,41,64,65]. The probability of direct photoinactivation will, however, vary depending upon the optical screening and package effects around PSII which alter the achieved light incident upon the Mn4Ca complex. Since package effect varies with cell size larger cells show a lower probability of direct photoinactivation [65,66].

In contrast, the probability of generation of 1O2 shows a positive dependence upon increasing incident light level, which drives saturation of electron carriers out of PSII, leading to an increased probability of reactive oxygen species production [18]. Furthermore the antenna size of the PSII light harvesting complex will positively affect the per-photon probability of photoinactivation of PSII [67] since a larger antenna size supports greater photon capture, resulting in increased excitation pressure at a given light level [16,18,48].

Fig 1 presents a schematic overview of these fluxes and fates of excitonic energy within PSII, drawing upon concepts reviewed elsewhere [18,44,52,62,68]. Incident photons are absorbed by antenna pigment proteins, whose spectral properties vary depending upon the taxon and acclimation state of the cell. Within the antenna complex both regulated and non-regulated processes [69] lead to dissipation of a variable fraction of the excitons as heat. A quantitatively minor fraction of excitons are also dissipated from the antenna as fluorescence, contributing to FO level emission. The remaining, variable, fraction of excitons are transferred into the inner antenna of the PSII reaction centre, which is highly conserved across taxa. Of these excitons a small fraction are again dissipated as fluorescence from the pigments of the reaction centre, contributing to FO level emission but also to the variable fluorescence FV emitted by closed PSII centres. The remaining fraction of the excitons provoke PSII photochemistry, parameterized as σPSII (A2 quanta-1) [7072], the effective absorption cross section for PSII photochemistry. PSII photochemistry can lead to charge separation and electron transport, parameterized as the yield ΦPSII, or to fast recombinations resulting in heat or delayed light emission [52]. If excitation delivery is high relative to downstream electron transport excited intermediates can accumulate [18]. This provokes production of singlet oxygen (1O2), which leads to an increase in the probability of PSII inactivation, herein parameterized as the yield for inactivation of PSII by a photon delivered through the PSII antenna, Φi PSII. Φi PSII is thus predicted to increase with rising excitation pressure [62,68]. A few short wavelength photons can also be directly absorbed by the manganese cluster of the oxygen evolving complex, leading to photoinactivation whose probability per photon does not change with excitation pressure [41,48,62,73]. Under low to moderate blue light this direct path can dominate the effective absorption cross for inactivation of PSII on the basis of incident photons, parameterized as σi (A2 quanta-1) [44,66,74,75]. The relative magnitudes of the two categories of photoinactivation thus depends upon the spectral quality of the light relative to the antenna spectra of the organism, and upon the physiological state of the organism [76], which influences excitation pressure and capacities for reactive oxygen species detoxification.

thumbnail
Fig 1. Conceptual overview of fates of photons in Photosystem II.

Incident photons (downward waves) are differentially absorbed (ā*) depending upon the particular absorbance spectra of the antenna pigment protein complexes serving PSII, indicated as a green trapezoid to reflect the diversity of antenna pigments and protein structures across taxa. A variable fraction of the excitons is dissipated as heat (yellow-orange arrow, NPQ); a further small fraction of excitons are dissipated as fluorescence emitted from the antenna (red arrow). The remaining excitons are transferred into the inner antenna of the PSII reaction centre (downward red arrows). Of these excitons a small but variable fraction are again dissipated as fluorescence (red arrow) from the pigments of the reaction centre. The remaining excitons provoke PSII photochemistry (σPSII; A2 quanta-1) leading to charge separation and electron transport with a variable yield (ΦPSII), or to fast recombinations resulting in heat emission (yellow-orange arrow, NPQ). If excitation is high relative to downstream electron transport excited intermediates can accumulate. This provokes production of singlet oxygen (1O2), which leads to an increase in the probability of PSII inactivation, herein parameterized Φi PSII, a dimensionless yield for inactivation of a PSII by a photon delivered through the PSII antenna. Short wavelength photons can also be directly absorbed by the manganese cluster of the oxygen evolving complex (thin violet wave), leading to direct photoinactivation. This figure is based upon concepts reviewed in [18,44,52,62,68].

https://doi.org/10.1371/journal.pone.0168991.g001

Whatever the photoinactivation mechanism(s), as light level increases so will the rate of inactivation of PSII centers which must be countered through removal of inactive PSII proteins and synthesis of new ones to maintain photosynthetic activity. A damaged PsbA protein is degraded by the FtsH and/or Deg proteases [7779], allowing the reconstitution and re-activation of the PSII center with a newly synthesized PsbA. Cells respond to increasing light by activating repair mechanisms including the up-regulation of psbA transcript levels, the gene encoding the PsbA protein [48,8083]. Most cyanobacteria, although not Prochlorococcus, have small psbA gene families encoding two or more isoforms of the PsbA proteins with different photochemical properties [8486] which are differentially induced depending upon irradiance and physiological state. The very repair cycle needed to regenerate PSII is itself strongly sensitive to inhibition by reactive oxygen [8790] so net photoinhibition can result from both direct photoinactivation and from concomitant inhibition of the counteracting repair processes.

Photoinactivation and the regeneration of PSII through the PSII repair cycle imposes a significant metabolic burden upon the organism [9194], which in turn places ecological limits upon their achieved niches and productivity [95,96]. Given the ecological importance of Synechococcus and Prochlorococcus, and their differential strategies to manage and exploit excitation [8,9597] we sought to characterize the photoinactivation of PSII in these species. We used controlled culturing to grow representative strains of Synechococcus and Prochlorococcus under low and higher light. We then tracked their susceptibility to photoinactivation of PSII under a range of light levels, when counteracting PSII repair was blocked. We used a blue light treatment as an approximation of the blue-enriched light field in marine waters, and a red light treatment because the comparison with blue light was likely to be mechanistically informative [41,48,68]. We then used the composition of PSII and standard pathways to estimate the metabolic return on investment for repair or synthesis of a PSII, for each species under a range of light levels.

Materials & Methods

Culturing Conditions and Growth Rates

Synechococcus sp. WH8102 was grown in PCR-S11 media [98] while Prochlorococcus marinus MED4 was grown in Pro99 media [99,100]. Semi-continuous cultures for each species were maintained at low light (30 or 75 μmol photons m-2 s-1) or high light (260 μmol photons m-2 s-1) at 23–24°C under fluorescent lights with a 12:12 light:dark cycle with transitions from dark to light at 08:00 hours. A first round of semi-continuous cultures was grown in 50 mL tubes with plastic caps allowing airflow. A second round of semi-continuous cultures was grown in clear 6-well plates with each well containing 6.5 mL of culture. Data from both rounds of semi-continuous culturing was pooled for this manuscript after analyses of variance showed no significant effect of culture round upon measured variables (data not presented).

The growth of the cultures was tracked daily by fluorescence emission (Molecular Devices SpectraMax Gemini EM, Sunnyvale, California). Prochlorococcus was excited at 440 nm and the fluorescence emission was read at 680 nm. Synechococcus was excited at 550 nm and the fluorescence emission was read at 650 nm. For both genera the Relative Fluorescence Units (RFU) of their emission was tracked over elapsed time to calculate exponential growth rates for each sample using the equation: (1) Where RFUt is the fluorescence reading at elapsed time “t” and RFU0 is the fluorescence reading at time 0. The cultures were kept in exponential growth phase by 1 in 5 dilutions with fresh media every 5–7 days. Cultures were diluted and/ or harvested near the end of exponential phase to harvest the most biomass possible while the culture was still in exponential phase.

Photosystem II Physiological Characterization

The photoinactivation treatments and measurements were carried out in Photon Systems Instruments FL3500 super-heads (Drasov, Czech Republic) with a lab-built aluminum plug for temperature control. For each treatment, a 2 mL sample was loaded into a cuvette with a micro stir-bar and plugged to hold the temperature at 23–24°C through circulation of cooling fluid through the aluminum plug. The super-head provided three capacities: firstly, application of sub-saturating flashlets of adjustable light level of 1.2 μs duration in red (655 nm LED) or blue (455 nm LED); secondly, detection of the fluorescence emission resulting from the flashlets; and thirdly, delivery of actinic light of adjustable intensity in red or blue (Table 1). We used the super-head flashlet capacity to perform fast repetition rate (FRR) chlorophyll fluorescence induction profiles, which were fit to a four parameter model (Table 2) to quantify PSII physiology [70] using PSIWORX-R data handling and fitting software implemented in the R environment (A. Barnett, http://sourceforge.net/projects/psiworx). The FRR induction curves were driven by a train of 40 flashlets of 1.2 μs each separated by 2.0 μs dark, for a cumulative flashlet train duration of 128 μs, shorter than the 200–500 μs for transfer of an electron from Qa to Qb, and almost 1 order of magnitude less than the subsequent ~1000 μs that it takes for the bound Qb pool of PSII to equilibrate with the plastoquinone pool [16,70]. FRR inductions were measured in the presence of background actinic light, and then again 2 s after the end of actinic light exposures.

Whole-Cell Spectroscopy

An absorbance spectrum was taken for each sample using an Olis CLARiTY DSPC spectrophotometer (Bogart, Georgia). The integrating, internally reflective DSPC cavity records accurate absorbance spectra from dilute suspensions of phytoplankton cells with high light scattering relative to low absorbance. Spectra were taken in the visible range, λ = 390–750 nm, at 1 nm intervals. Spectra of media blanks were subtracted from their respective genera and a conversion was performed to correct for chamber reflectivity using Fry’s Method [101]. This data transform takes the total absorbance spectra from the integrating, internally reflective cavity, and corrects it to the equivalent absorbance expected from a hypothetical 1 cm path length spectrophotometer cuvette measurement without scattering. Fig 2A compares typical absorbance spectra for Prochlorococcus and Synehococcus with the emission wavelength profiles of the LED lamps used to provide the light treatments.

thumbnail
Fig 2. Cellular absorbance, light treatment color and protocol.

(A) Whole Cell Absorbance Spectra of Synechococcus sp. WH8102 and Prochlorococcus marinus MED4. The relative emission spectra of the actinic blue and red LED used to induce photoinactivation (Fig 2B) in Synechococcus and Prochlorococcus are overlaid on the absorbance spectra, normalized to their red chlorophyll a peak. (B) Light intensity and measurement timing through the duration of a representative light treatment experiment. The pre-zero dotted line indicates the growth light for the culture; 75 in this representative figure; 30 or 260 μmol photons m-2 s-1 in other experiments. Each treatment time course then consisted of 10 sequential periods of 327 s, shown by the solid black line. The first 327 s period was in the dark, the second period was under the growth irradiance for the particular sample. The third to ninth treatment periods, shown here at 700 μmol photons m-2 s-1, were at irradiance and colour combinations shown in Table 1. The tenth period was a low light recovery phase of 20 μmol photons m-2 s-1. The black triangle indicates a Fast Repetition chlorophyll fluorescence induction measurement taken after the initial dark period, using 40 flashlets of 1.2 μs duration, spaced by 2 μs darkness, which cumulatively delivered a single turnover saturating flash over 128 μs. From this induction curve we used PSIWORX-R script to extract estimates for F0, FM and σPSII. Each green triangle thereafter indicates the timing of a chlorophyll fluorescence induction measurement taken after an illuminated period, represented in the inset above the treatment trace. At each measurement point we captured an induction applied in the presence of continuing actinic irradiance to extract estimates for FS, FM′ and σPSII′. We then interrupted the actinic irradiance for 2 s of darkness to allow PSII centres to re-open, followed by another fluorescence induction to extract estimates for F0′, FM′ (2s) and σPSII′(2s). The post-induction fluorescence relaxation phase of the full Fast Repetition and Relaxation fluorescence profile is omitted from this schematic diagram for clarity.

https://doi.org/10.1371/journal.pone.0168991.g002

Photoinactivation Treatments

To measure photoinactivation the overlapping effects of the PSII repair cycle and non-photochemical quenching must both be considered [44,68]. Lincomycin at a final concentration of 500 μg mL-1, was used to inhibit prokaryotic ribosomes and thereby block the PSII repair cycle during the photoinactivation treatments [48,73,97,102]. Samples were subjected to light shift treatments of 10 consecutive periods of 327 s each, totaling 3270 s at a range of levels of blue or red treatment light (Table 1). The choice of 327 s was imposed by a limitation on the maximum time between sequential measurements in the software control of the fluorometer. Fig 2B presents a schematic overview of the photoinactivation treatment and measurement protocol. A FRR measurement was taken 2s after each illumination period and analyzed to extract photophysiological parameters (Table 2) including σPSII′2s and FV′2s/FM′2s estimates corresponding to their respective preceding period.

The initial dark period allowed for the measurement of σPSII after relaxation of any non-photochemical quenching induced by growth conditions. FV′2s/FM′2s taken after 327 s under the sample growth light gave the maximal photochemical yield of PSII in the light acclimated state. FV′2s/FM′2s measured after each of 8 successive 327 s periods under the treatment light tracked the maximum photochemical yield in response to the light shift treatment. Finally, the terminal tenth low light period from 2943 to 3270 s then allowed the sample to reverse any changes caused by sustained NPQ which persisted through the 2s dark periods before measurements, but which could relax over the final 327 s under low light in the absence of protein synthesis, blocked by lincomycin. The influence of sustained NPQ on photochemical yield was then estimated as: (2) where Influence of Sustained NPQ was forced to be ≥0. The Influence of Sustained NPQ on photoinhibition were then corrected by adding the value to FV′2s/FM′2s measured after each treatment light interval. Therefore, we attributed any remaining decline in the maximum photochemical yield of (+) lincomycin samples to photoinactivation, which did not reverse in the absence of protein synthesis under the final 327 s of low light (Fig 2B). For the cultures in this study this correction had little influence on the subsequent curve fits, although in other taxa sustained NPQ is a significant factor confounding estimations of the photoinactivation of PSII [103].

Quantitation of Photoinactivation

The corrected FV′2s/FM′2s values were then plotted against cumulative incident photons for the treatment light period. (3) Where cumulative incident photons had units of quanta m-2, treatment light level had units of μmol photons m-2 s-1, and the duration of each period was a constant 327 s.

A single-phase exponential decay curve was fit to the data using the following equation: (4) where σi is a target size parameterization [44,66,74] of the probability of a photoinactivation per incident photon with units of m2 quanta-1. Higher σi values indicate a higher probability of photoinactivation per incident photon, and a lower σi indicates a lower susceptibility to photoinactivation per incident photon. Fig 3A presents representative photoinactivation curves measured in the presence of lincomycin, under red or blue light treatments.

thumbnail
Fig 3. Representative photoinactivation treatment data.

Prochlorococcus marinus MED4 was grown under 260 μmol photons m-2 s-1 and then treated under 1200 μmol photons m-2 s-1 of red light (red squares) or 1200 μmol photons m-2 s-1 of blue light (blue squares) following the protocol outlined in Fig 2A. For non-least squares non-linear modelling of the data (nlsLM, R) [104] each FV′ 2s/FM′ 2s derived from an individual Fast Repetition and Relaxation chlorophyll fluorescence induction after 2 s of darkness following actinic light conditions (Fig 2A, inset) was weighted by the inverse of its 95% confidence interval (plotted as error bars on the points) to account for variability in the precision of individual estimates of FV′ 2s/FM′ 2s. (A) The decay of the quantum yield of PSII (FV′ 2s/FM′ 2s) (Fig 2A, inset), plotted versus time and cumulative incident photons since the start of the treatment. The decay of FV′ 2s/FM′ 2s was fit (solid lines) to the annotated equation to extract σi, a target size parameterization of the probability of an incident photon inducing photoinactivation of PSII. In these examples the σi was 1.65 × 10−5 Å2 PSII-1 under red light treatment (red diamonds) and 1.23 × 10−4 Å2 PSII-1 under blue light treatment (blue squares). 95% C.I. on the fit plotted as dotted lines. (B) The decay of FV′ 2s/FM′ 2s (solid lines) against cumulative photons delivered to PSII photochemistry, estimated as cumulative incident photons multiplied by the effective absorption cross section of the sample, σPSII′ 2s. The decay is fit to the annotated equation to extract Φi PSII, the probability of photoinactivation by a photon delivered to PSII through the antenna. The fitted values of Φi PSII were 2.8 × 10−7 PSII photon -1 under red light treatment (red diamonds) and 7.2 × 10−7 PSII photon -1 under blue light treatment (blue squares). 95% C.I. on the fit plotted as dotted lines.

https://doi.org/10.1371/journal.pone.0168991.g003

Correcting σi for Photons Delivered to PSII

To correct for effects on σi caused by spectral or regulatory differences in delivery of excitation to PSII through the light harvesting antennae, susceptibility to photoinactivation was recalculated using cumulative photons delivered to PSII, as opposed to the previous σi calculation using cumulative photons incident upon the cells. A single-phase exponential decay was used to calculate the yield of photoinactivation of PSII on the basis of photons delivered to PSII (Φi PSII): (5)

The parameter Φi PSII is a formally dimension-less yield (PSII inactivated photon-1 = quanta quanta-1) that expresses the number of PSII photoinactivation events per photon delivered to PSII through the effective absorption cross section for PSII photochemistry. We earlier expressed a conceptually similar concept [44] as the ratio of the effective absorption cross section for PSII photochemistry, σPSII to the effective absorption cross section for photoinactivation, σi. Herein we used time-specific σPSII′2s values measured every 327 s throughout the light-shift photoinactivation treatment to give the effective absorption cross section of PSII over that 327 s, in order to calculate the photons delivered to PSII over that period. Fig 3B presents representative photoinactivation curves measured in the presence of lincomycin, under red or blue light treatments plotted versus cumulative photons delivered to PSII.

Testing the Response of Φi PSII to PSII Closure

If photoinactivation is driven by reactive oxygen by-products of excitation and electron fluxes through PSII [18,52,105] the susceptibility to photoinactivation should increase as excitation of PSII increases relative to electron transport away from PSII. To determine whether excitation pressure, the balance between excitation delivery to PSII, and electron flow away from PSII [106], indeed affected susceptibility to photoinactivation [18,52] we used the parameter 1 –qP [107] (6) where a value of 0 indicates all PSII are open and ready to accept excitation and a value of 1 indicates all PSII are closed and thus more susceptible to generation of reactive oxygen species. We calculated 1 –qP for a given treatment after the initial 327 s exposure to the treatment light, as the value remained relatively unchanged thereafter with further treatment light exposure (data not shown). In these calculations we used a calculated F0′ (Table 2) [108,109].

PSII Electron Transport versus Electron Equivalents to Recycle PSII

In order to determine the number of photochemical events performed per s by PSII under the treatment light, we used the effective absorption cross section of PSII under treatment light after 2 s of darkness (σPSII′ 2s), the proportion of open PSII when exposed to treatment light (qP) and the intensity of the treatment light (I) [113,114]: (7)

In order to determine the number of photoinactivation events per PSII per s, we multiplied the effective cross section for photoinactivation (σi) (Å2quanta-1) by the intensity of the treatment light (I) (1 μmol photons m-2 s-1 = 6.022 × 10−3 quanta Å-2 s-1). We then estimated the investment in metabolic electron equivalents of ATP and reductant needed in order to either synthesize a complete de novo PSII (1.96 × 105 e-/PSII), or to recycle most PSII protein subunits while proteolytically degrading and re-synthesizing the equivalent of new PsbA and PsbD proteins (5.77 × 103 e-/(PsbA + PsbD)).

We arrived at these metabolic electron equivalent costs by summing the amino acid composition of the proteins of PSII [92,115] and accounting for the ATP costs of ribosomal protein synthesis [116118], the electron and ATP costs for assimilation of CO2 and NO3- to amino acids [119121], and the ATP costs for FtsH protease turnover of PsbA and PsbD subunits [122,123]. We converted ATP costs to electron equivalents with the textbook ratio of 1.33 e-/ATP for respiratory electron transport. These approximations serve to place the cost of PSII inactivation on a common denominator for comparison with electron generation by PSII.

Results & Discussion

σi varies with Treatment Light Intensity and with Excitation Pressure on PSII

σi estimates were derived from individual photoinactivation time courses in the presence of lincomycin (Fig 3A) for combinations of species, growth light level, treatment light colour and treatment light intensity (Table 1). Fig 4 presents these estimates of σi plotted versus the treatment light intensity. For fitting of regressions each σi estimate was weighted by the inverse of its 95% confidence interval, plotted as error bars on the points, to account for variability in the precision of individual estimates of σi (Fig 3A).

thumbnail
Fig 4. σi plotted against treatment light intensities.

For regressions each σi derived from an individual treatment time course (ex. Fig 3A) was weighted by the inverse of its 95% confidence interval (error bars on the points) to account for variability in the precision of individual estimates of σi. (A) σi from treatments of Synechococcus sp. WH8102 under a range of light levels. σi2 photon-1) estimates derived from red light treatment (open red symbols) fell on a single regression against treatment light intensity (μmol photons m-2 s-1) for cultures grown under both low (red open inverted triangles) or high (red open diamonds) light; (solid red line, slope = 5.620 × 10−8 ± 1.212 × 10−8, intercept = 4.850 × 10−6 ± 1.027 × 10−5 (not significantly different from zero, p>0.05), R2 = 0.6616, dotted red lines denote 95% confidence intervals on the regression). σi estimates derived from blue light treatment (open blue symbols) fell on different regressions for cultures grown under low light (blue open triangles) (solid blue line, slope = 5.200 × 10−8 ± 1.814 × 10−8, intercept = 1.586 × 10−4 ± 1.146 × 10−5, R2 = 0.2401, dotted lines show 95% confidence intervals on the regression), or for cultures grown under high light (blue open squares) (slope = 1.008 × 10−7 ± 1.626 × 10−8, intercept = 3.749 × 10−5 ± 1.011 × 10−5, R2 = 0.846) (S1 Statistics). (B) σi from treatments of Prochlorococcus marinus MED4 measured under a range of treatment irradiances. σi estimates derived from red light treatment fell on a single regression (solid red line, slope not significantly different from zero, p>0.05; intercept = 2.130 × 10−5 ± 9.023 × 10−6, R2 = 0.05971, dotted red lines denote 95% confidence intervals) for cultures grown under either low (red inverted triangles) or high (red diamonds) light. σi estimates derived from blue light treatment fell on a single regression (solid blue line, slope = 4.013 × 10−8 ± 1.714 × 10−8, intercept = 1.191 × 10−4 ± 1.214 × 10−5, R2 = 0.2437, dotted blue lines denote 95% confidence intervals) for cultures grown under low (blue triangles) or high (blue squares) growth light (S2 Statistics).

https://doi.org/10.1371/journal.pone.0168991.g004

Under red light σi was low for both Synechococcus and Prochlorococcus. For Synechococcus the Y intercept of the regression of σi versus treatment light intensity was not significantly different from 0, but there was a significant increase in photoinactivation with increasing intensity of red light treatment. In Prochlorococcus the Y intercept was small and there was no significant increase in σi with increasing intensity of red light treatment. Under blue light treatment σi was significantly higher than under red light, consistent with expectations [41,48,65,68,124,125]. Synechococcus cultures grown under high light fell on regression with intercept and slope distinct from Synechococcus cultures grown under lower light. When treated under blue light the Prochlorococcus low light and higher light grown cultures all fell on a common regression but there was an increase in σi with increasing intensity of blue light treatment.

The absorbance spectra of the cultures varied with species (Fig 2A) and with growth light (data not shown). The photosynthetic physiologies of the species are also distinct with evidence for down-stream limitations on the rate of electron transport away from PSII in Prochlorococcus when compared to Synechococcus [11,126,127]. Therefore a given treatment light level or colour could have differing functional implications for the cell depending upon species and prior light regime [76]. We therefore decided to replot the σi estimates versus the excitation pressure upon PSII imposed by each given combination of treatment light intensity and colour (Fig 5A and 5B). These replots show patterns very similar to the plots of σi versus treatment light intensity (Fig 4A and 4B), except that under red light treatment Prochlorococcus shows a small positive response of σi to increasing excitation pressure.

thumbnail
Fig 5. σi versus excitation pressure on Photosystem II.

σi plotted against excitation pressure, measured as 1—qP after 300 s of treatment light exposure. Under red or blue treatment light, qP showed remained nearly steady from 327 s onwards (data not shown) so the plotted values for 1—qP were taken after the first period of 327 exposure to treatment light. For regressions each σi derived from an individual treatment timecourse (Fig 3A) was weighted by the inverse of its 95% confidence interval (error bars on the points) to account for variability in the precision of individual estimates of σi. (A) σi from Synechococcus sp. WH8102. σi estimates derived from red light treatments fell on a single regression (solid red line, slope = 1.103 × 10−4 ± 2.670 × 10−5, intercept not significantly different from zero, p>0.05; R2 = 0.6079, dotted red lines denote 95% confidence intervals on the regression). for Synechococcus cultures grown under low (red open inverted triangles) or high (red open diamonds) growth light. For σi estimates derived from blue light treatment, low light grown cultures (blue open triangles) fell upon a regression (solid blue line, slope = 2.349 × 10−4 ± 4.437 × 10−5, intercept = 9.742 × 10−6 ± 1.540 × 10−5, R2 = 0.3813, dotted lines show 95 % confidence intervals), while the high light grown cultures (open blue squares) fell upon a different regression (solid blue line, slope = 1.332 × 10−4 ± 3.326 × 10−5, intercept not significantly different from zero, p>0.05; R2 = 0.8001, dotted lines show 95 % confidence intervals on the regression) (S3 Statistics). (B) σi from Prochlorococcus marinus MED4. σi estimates derived from red light treatment (low light grown cultures, red inverted triangles; high light grown cultures, red diamonds) fell on a single regression (solid red line, slope = 3.484 × 10−5 ± 1.222 × 10−5, intercept not significantly different from zero, p>0.05;, R2 = 0.5755, dotted red lines denote 95 % confidence intervals). σi estimates derived from blue light treatment (low light grown cultures, blue triangles; high light grown cultures, blue squares) fell on a single regression (solid blue line, slope = 1.262 × 10−4 ± 5.667 × 10−5, intercept not significantly different from zero, p>0.05; R2 = 0.2259, dotted blue lines denote 95 % confidence intervals) (S4 Statistics).

https://doi.org/10.1371/journal.pone.0168991.g005

The Y intercepts on these plots represent the inherent photoinactivation potential of an incident photon in the absence of any excitation pressure, and therefore in the absence of any electron transport or risk of reactive oxygen generation by PSII or related electron flows. Under red light treatment both Synechococcus and Prochlorococcus show Y intercepts not significantly different from 0 for these plots of σi versus increasing excitation pressure. Thus at the Y intercept, in the absence of electron transport, red photons show no detectable intrinsic toxicity to PSII. The low level of photoinactivation under red light is thus quantitatively attributable to by-products of electron transport through PSII.

Under blue light treatments Synechococcus grown under lower light, and Prochlorococcus, σi shows Y intercepts significantly higher than 0, demonstrating an intrinsic toxicity of blue light to PSII [48,62,68,124], even in the absence of electron flow and its concomitant reactive oxygen species byproducts. Synechococcus grown under higher light showed low (Fig 4A) or insignificant (Fig 5A) Y intercepts for σi, and thus showed a lower intrinsic susceptibility to blue light photoinactivation, which could relate to expression of alternate isoforms of the PsbA protein [8486] in Synechococcus.

The rising slopes of σi with increasing excitation pressure upon PSII represent the outcome of a complex balance among multiple paths [18,52,105] of potential reactive oxygen species production related to electron fluxes (Fig 1) and the counteracting detoxification mechanisms whose presence and induction can vary both with species and with prior growth conditions [8,76].

Φi PSII versus Excitation Pressure on PSII to Reconcile Species and Growth Light Effects

We next asked whether the photoinactivation patterns could be reconciled by considering the yield of photoinactivation on the basis of photons delivered to PSII via the light harvesting antenna. We therefore estimated a new parameterization, Φi PSII to express the yield of photoinactivation of PSII relative to photons driving PSII photochemistry, as measured by the effective absorption cross section for photochemistry, σPSII. For plots of Φi PSII versus excitation pressure (Fig 6) Synechococcus and Prochlorococcus from both low and higher prior growth lights all fell on a common regression under red light treatment, and on a common regression for blue light treatment. The two treatment lights gave equivalent slopes with increasing excitation pressure, but were distinguised by a higher Y intercept for blue light treatments. Thus the intrinsic toxicity of blue light, likely through direct photoinactivation of the manganese cluster of PSII [41,48] manifests as a strong potential for photoinactivation by blue photons even when electron flow through PSII is negligible. With rising excitation pressure both blue and red light drive comparable increases in photoinactivation, when expressed on the basis of excitation actually delivered to PSII photochemistry, rather than on the basis of incident photons. The relative importance of these distinct photoinactivation paths [62,68] will depend upon cellular absorbance spectra and the light level, but more particularly upon the physiological excitation pressure upon PSII, a proxy for the probability of generation of reactive oxygen species. Under physiologically low to moderate levels of light direct photoinactivation by blue light can dominate, and can be parameterized as a simple target size [66,7375]. This conditions would often prevail in marine systems. As excitation pressure rises either through increasing light in near-surface environments or through factors that restrict the down-stream removal of electrons from PSII [39,106] the reactive oxygen species -dependent photoinactivation paths related to electron transport will increase and even predominate. These patterns become apparent across spectrally diverse species with different growth histories by expressing photoinactivation on the basis of photons delivered to PSII, plotted versus excitation pressure, rather than the treatment light level per se.

thumbnail
Fig 6. Φi PSII versus excitation pressure on Photosystem II.

Synechococcus sp. WH8102 (open symbols) and Prochlorococcus marinus MED4 (closed symbols) fell on a common regression for Φi PSII (PSII photon-1) measured under red light treatment (solid red line, slope = 3.142 × 10−7 ± 1.110 × 10−7, intercept = 1.968 × 10−7 ± 7.308 × 10−8, R2 = 0.2968, dotted red lines denote 95% confidence intervals). Synechococcus sp. WH8102 and Prochlorococcus marinus MED4 also fell on a common regression Φi PSII measured under blue light treatment (solid blue line, slope = 3.731 × 10−7 ± 4.921 × 10−8, intercept = 4.046 × 10−7 ± 3.458 × 10−8, R2 = 0.5156, dotted red lines denote 95% confidence intervals on the regressions). Species had no statistically significant effect on the regressions of Φi PSII versus excitatation pressure, nor did low (circles) versus high (squares) growth light when either species or growth light was including in a linear model of the data as a binary interaction term, using ‘lm’ in R [128] (S5 Statistics).

https://doi.org/10.1371/journal.pone.0168991.g006

For regressions each Φi PSII derived from an individual treatment time course (Fig 3B) was weighted by the inverse of its 95% confidence interval (error bars on the points) to account for variability in the precision of individual estimates of Φi PSII.

The Return on Investment for Photosystem II in the Face of Photoinactivation

The inactivation of PSII and the counteracting repair processes impose a significant, and variable, metabolic burden upon photoautotrophs [9194,119] that interacts with nutrient supply [129,130] and with cell size [66]. We thus sought to use the optically simple Synechococcus and Prochlorococcus to compare the photochemical return on investment from a PSII, to the costs for net biosynthesis of a PSII from inorganic precursors, or to the costs to degrade and replace the PsbA and PsbD subunits of the complex (Fig 7). Our present analyses is restricted to nutrient replete cultures, but nutrient limitation likely interacts with these processes [131,132]. Photochemical events through PSII were estimated as (σPSII′ 2s) × qP × E. Photoinactivation events were estimated as σi × E and then multiplied by the e- equivalent cost for biosynthesis of PSII or by the e- equivalent cost for turnover of PsbA/PsbD. PSII Electron transport at a given treatment light level was consistently higher in Synechococcus than in Prochlorococcus, consistent with larger σPSII and greater down stream capacity for electron fluxes in Synechococcus [127]

thumbnail
Fig 7. Rates of electron transfer through Photosystem II versus Treatment Light intensity, compared to electron equivalent cost for Photosystem II synthesis or recycling.

Photochemical events (larger circles) were estimated as σPSII′ 2s × qP × E. Photoinactivation eventswere estimated as σi × E and multiplied by the e- equivalent cost for biosynthesis of PSII (smaller black circles; shaded grey segment) or by the e- equivalent cost for turnover of PsbA/PsbD (+ or ×; black segment along X axes). (A) Synechococcus under blue light. (B) Prochlorococcus under blue light. (C) Synechococcus under red light. (D) Prochlorococcus under red light.

https://doi.org/10.1371/journal.pone.0168991.g007

Fig 7 plots a narrow black segment along the X axes to show the low metabolic cost needed to repair a photoinactivated PSII through degradation and re-synthesis of new PsbA/PsbD proteins. Across the tested range of blue or red treatment light levels Synechococcus PSII electron transport stayed well above this cost to repair a photoinactivated PSII, so PSII repair was always a metabolically viable strategy for our Synechococcus cultures, at least when growing under nutrient repletion. In contrast in Prochlorococcus much lower PSII electron transport, possibly limited by downstream metabolic capacity [127] means that the photochemical return from a PSII drops to levels similar to the metabolic cost to repair a PSII at light levels of ~1200 μmol photons m-2 s-1 for red or for blue treatment lights. The wider grey segment shows the metabolic cost for net biosynthesis of a new PSII from inorganic precursors at a rate sufficient to counter photoinactivation. Again, Synechococcus enjoys a positive net return on newly synthesized PSII up to and beyond 1200 μmol photons m-2 s-1, under both blue and red treatment lights, at least when growing under nutrient repletion and near-optimal temperatures. In marked contrast for Prochlorococcus under blue light the net cost to biosynthesize a new PSII exceeds the anticipated photochemical return from the new PSII at light levels above ~300 μmol photons m-2 s-1. Under the informative but less ecophysiologically relevant red light the lower rates of photoinactivation mean Prochlorococcus enjoys a positive return upon a new PSII up to light levels of ~1200 μmol photons m-2 s-1. These contrasting patterns in Synechococcus and Prochlorococcus support findings [8] that Synechococcus tends towards active mechanisms to cope with increasing excitation. In contrast Prochlorococcus tends to merely endure transient exposure to excess excitation and might trend towards mixotrophy under some conditions [133] when maintaining photosynthesis becomes untenable. These contrasting patterns also underlie findings of different excitation tolerance thresholds for the different picocyanobacteria [95,96], and their niche partitioning [97].

Acknowledgments

The authors thank Dr. M. Thaler, Laval University, for advice on R coding, and M. Corkum and N. Donaher of Mount Allison University for microbial culturing support. Chris MacKay of Tantramar Interactive prepared Fig 1.

Author Contributions

  1. Conceptualization: DC CM MR.
  2. Data curation: CM EA MR AB DC.
  3. Formal analysis: CM EA DC MR.
  4. Funding acquisition: DC.
  5. Investigation: CD MR AD DC.
  6. Methodology: DC MR CD EA.
  7. Project administration: DC.
  8. Resources: DC.
  9. Software: AB EA MR CD AD DC.
  10. Supervision: DC.
  11. Visualization: CM DC MR AB EA.
  12. Writing – original draft: DC CD MR.
  13. Writing – review & editing: DC CD EA.

References

  1. 1. Partensky F, Blanchot J, Vaulot D. Differential distribution and ecology of Prochlorococcus and Synechococcus in oceanic waters: a review. Bulletin-Institut Oceanographique Monaco-Numero Special. 1999;19: 457–476.
  2. 2. Scanlan DJ. Physiological diversity and niche adaptation in marine Synechococcus. Advances in Microbial Physiology. Academic Press; 2003. pp. 1–64. http://www.sciencedirect.com/science/article/pii/S006529110347001X
  3. 3. Zwirglmaier K, Jardillier L, Ostrowski M, Mazard S, Garczarek L, Vaulot D, et al. Global phylogeography of marine Synechococcus and Prochlorococcus reveals a distinct partitioning of lineages among oceanic biomes. Environmental Microbiology. 2008;10: 147–161. pmid:17900271
  4. 4. Mackey KRM, Paytan A, Caldeira K, Grossman AR, Moran D, McIlvin M, et al. Effect of Temperature on Photosynthesis and Growth in Marine Synechococcus spp. PLANT PHYSIOLOGY. 2013;163: 815–829. pmid:23950220
  5. 5. Paulsen ML, Doré H, Garczarek L, Seuthe L, Müller O, Sandaa R-A, et al. Synechococcus in the Atlantic Gateway to the Arctic Ocean. Frontiers in Marine Science. 2016;3.
  6. 6. Moore LR, Goericke R, Chisholm SW. Comparative physiology of Synechococcus and Prochlorococcus: influence of light and temperature on growth, pigments, fluorescence and absorptive properties. MEPS. 1995;116: 259–275.
  7. 7. Not F, Massana R, Latasa M, Marie D, Colson C, Eikrem W, et al. Late summer community composition and abundance of photosynthetic picoeukaryotes in Norwegian and Barents Seas [Internet]. 2005 [cited 10 Feb 2014]. http://digital.csic.es/handle/10261/27514
  8. 8. Mella-Flores D, Six C, Ratin M, Partensky F, Boutte C, Le Corguille G, et al. Prochlorococcus and Synechococcus have Evolved Different Adaptive Mechanisms to Cope with Light and UV Stress. Front Microbiol. 2012;3.
  9. 9. Finkel Z. Light Absorption and Size Scaling of Light-Limited Metabolism in Marine Diatoms. 2007; 1–10.
  10. 10. Kirk JTO. Light and photosynthesis in aquatic ecosystems. 2nd ed. Cambridge [England]; New York, NY, USA: Cambridge University Press; 1994.
  11. 11. Grossman AR, Mackey KRM, Bailey S. A Perspective on Photosynthesis in the Oligotrophic Oceans: Hypotheses Concerning Alternate Routes of Electron Flow. Journal of Phycology. 2010;46: 629–634.
  12. 12. Llabrés M, Agustí S. Effects of ultraviolet radiation on growth, cell death and the standing stock of Antarctic phytoplankton. Aquatic Microbial Ecology. 2010;59: 151–160.
  13. 13. Llabrés M, Agustí S. Picophytoplankton cell death induced by UV radiation: Evidence for oceanic Atlantic communities. Limnology and Oceanography. 2006;51: 21–29.
  14. 14. Bennett DIG, Amarnath K, Fleming GR. A Structure-Based Model of Energy Transfer Reveals the Principles of Light Harvesting in Photosystem II Supercomplexes. J Am Chem Soc. 2013;135: 9164–9173. pmid:23679235
  15. 15. Croce R, van Amerongen H. Light-harvesting and structural organization of Photosystem II: From individual complexes to thylakoid membrane. Journal of Photochemistry and Photobiology B: Biology. 2011;104: 142–153.
  16. 16. Falkowski PG. Aquatic photosynthesis. 2nd ed. Princeton: Princeton University Press; 2007.
  17. 17. Renger G. Light induced oxidative water splitting in photosynthesis: Energetics, kinetics and mechanism. Journal of Photochemistry and Photobiology B: Biology. 2011;104: 35–43.
  18. 18. Vass I. Molecular mechanisms of photodamage in the Photosystem II complex. Biochimica et Biophysica Acta (BBA)—Bioenergetics. 2012;1817: 209–217.
  19. 19. Rappaport F, Guergova-Kuras M, Nixon PJ, Diner BA, Lavergne J. Kinetics and Pathways of Charge Recombination in Photosystem II. Biochemistry. 2002;41: 8518–8527. pmid:12081503
  20. 20. Gantt E, Conti SF. Granuels Associated with the Chloroplast Lamellae of Porphyridium cruentum. J Cell Biol. 1966;29: 423–434. pmid:5962937
  21. 21. Redlinger T, Gantt E. A Mr 95,000 polypeptide in Porphyridium cruentum phycobilisomes and thylakoids: Possible function in linkage of phycobilisomes to thylakoids and in energy transfer. Proc Natl Acad Sci U S A. 1982;79: 5542–5546. pmid:16593227
  22. 22. Wilson A, Ajlani G, Verbavatz J-M, Vass I, Kerfeld CA, Kirilovsky D. A Soluble Carotenoid Protein Involved in Phycobilisome-Related Energy Dissipation in Cyanobacteria. Plant Cell. 2006;18: 992–1007. pmid:16531492
  23. 23. Boulay C, Abasova L, Six C, Vass I, Kirilovsky D. Occurrence and function of the orange carotenoid protein in photoprotective mechanisms in various cyanobacteria. Biochimica et Biophysica Acta (BBA)—Bioenergetics. 2008;1777: 1344–1354.
  24. 24. Kirilovsky D, Kerfeld CA. The Orange Carotenoid Protein: a blue-green light photoactive protein. Photochemical & Photobiological Sciences. 2013;12: 1135.
  25. 25. Gorbunov MY, Kuzminov FI, Fadeev VV, Kim JD, Falkowski PG. A kinetic model of non-photochemical quenching in cyanobacteria. Biochimica et Biophysica Acta (BBA)—Bioenergetics. 2011;1807: 1591–1599.
  26. 26. Kirilovsky D. Modulating energy arriving at photochemical reaction centers: orange carotenoid protein-related photoprotection and state transitions. Photosyn Res. 2015;126: 3–17. pmid:25139327
  27. 27. Roche JL, van der Staay GWM, Partensky F, Ducret A, Aebersold R, Li R, et al. Independent evolution of the prochlorophyte and green plant chlorophyll a/b light-harvesting proteins. Proc Natl Acad Sci U S A. 1996;93: 15244–15248. pmid:8986795
  28. 28. Ting CS, Rocap G, King J, Chisholm SW. Cyanobacterial photosynthesis in the oceans: the origins and significance of divergent light-harvesting strategies. Trends in Microbiology. 2002;10: 134–142. pmid:11864823
  29. 29. Wiethaus J, Busch AWU, Dammeyer T, Frankenberg-Dinkel N. Phycobiliproteins in Prochlorococcus marinus: Biosynthesis of pigments and their assembly into proteins. European Journal of Cell Biology. 2010;89: 1005–1010. pmid:20724022
  30. 30. Bailey S, Mann NH, Robinson C, Scanlan DJ. The occurrence of rapidly reversible non-photochemical quenching of chlorophyll a fluorescence in cyanobacteria. FEBS Letters. 2005;579: 275–280. pmid:15620726
  31. 31. Muller P, Li X, Niyogi KK. Non-Photochemical Quenching. A Response to Excess Light Energy. Plant Physiol. 2001;125: 1558–1566. pmid:11299337
  32. 32. Allahverdiyeva Y, Mustila H, Ermakova M, Bersanini L, Richaud P, Ajlani G, et al. Flavodiiron proteins Flv1 and Flv3 enable cyanobacterial growth and photosynthesis under fluctuating light. Proceedings of the National Academy of Sciences. 2013;110: 4111–4116.
  33. 33. Bagby SC, Chisholm SW. Response of Prochlorococcus to varying CO2:O2 ratios. The ISME Journal. 2015;9: 2232–2245. pmid:25848872
  34. 34. Bailey S, Grossman A. Photoprotection in Cyanobacteria: Regulation of Light Harvesting. Photochemistry and Photobiology. 2008;84: 1410–1420. pmid:19067963
  35. 35. Bersanini L, Battchikova N, Jokel M, Rehman A, Vass I, Allahverdiyeva Y, et al. Flavodiiron Protein Flv2/Flv4-Related Photoprotective Mechanism Dissipates Excitation Pressure of PSII in Cooperation with Phycobilisomes in Cyanobacteria. Plant Physiology. 2014;164: 805–818. pmid:24367022
  36. 36. Campbell D, Clarke A, Gustafsson P, Oquist G. Oxygen-dependent electron flow influences photosystem II function and psbA gene expression in the cyanobacterium Synechococcus sp PCC 7942. Physiologia Plantarum. 1999;105: 746–755.
  37. 37. Mustila H, Paananen P, Battchikova N, Santana-Sánchez A, Muth-Pawlak D, Hagemann M, et al. The Flavodiiron Protein Flv3 Functions as a Homo-Oligomer During Stress Acclimation and is Distinct from the Flv1/Flv3 Hetero-Oligomer Specific to the O2 Photoreduction Pathway. Plant and Cell Physiology. 2016;57: 1468–1483. pmid:26936793
  38. 38. Park YI, Chow WS, Osmond CB, Anderson JM. Electron transport to oxygen mitigates against the photoinactivation of Photosystem II in vivo. Photosynthesis Research. 1996;50: 23–32. pmid:24271819
  39. 39. Zhang P, Allahverdiyeva Y, Eisenhut M, Aro E-M. Flavodiiron Proteins in Oxygenic Photosynthetic Organisms: Photoprotection of Photosystem II by Flv2 and Flv4 in Synechocystis sp. PCC 6803. Finkel Z, editor. PLoS ONE. 2009;4: e5331. pmid:19390625
  40. 40. Andersson B, Salter H, Virgin I, Vass I, Styring S. Photodamage to photosystem II—primary and secondary events. Journal of Photochemistry and Photobiology B: Biology. 1992;15: 15–31.
  41. 41. Hakala M, Tuominen I, Keränen M, Tyystjärvi T, Tyystjärvi E. Evidence for the role of the oxygen-evolving manganese complex in photoinhibition of Photosystem II. Biochimica et Biophysica Acta (BBA)—Bioenergetics. 2005;1706: 68–80.
  42. 42. Mayes SR, Cook KM, Self SJ, Zhang Z, Barber J. Deletion of the gene encoding the Photosystem II 33 kDa protein from Synechocystis sp. PCC 6803 does not inactivate water-splitting but increases vulnerability to photoinhibition. Biochimica et Biophysica Acta (BBA)—Bioenergetics. 1991;1060: 1–12.
  43. 43. Rova EM, Ewen BM, Fredriksson P-O, Styring S. Photoactivation and Photoinhibition Are Competing in a Mutant of Chlamydomonas reinhardtii Lacking the 23-kDa Extrinsic Subunit of Photosystem II. J Biol Chem. 1996;271: 28918–28924. pmid:8910540
  44. 44. Campbell DA, Tyystjärvi E. Parameterization of photosystem II photoinactivation and repair. Biochim Biophys Acta. 2012;1817: 258–265. pmid:21565161
  45. 45. Chow W, Fan D-Y, Oguchi R, Jia H, Losciale P, Park Y-I, et al. Quantifying and monitoring functional photosystem II and the stoichiometry of the two photosystems in leaf segments: approaches and approximations. Photosynth Res. 2012;113: 63–74. pmid:22638914
  46. 46. Bornman JF. New trends in photobiology: Target sites of UV-B radiation in photosynthesis of higher plants. Journal of Photochemistry and Photobiology B: Biology. 1989;4: 145–158.
  47. 47. Pessarakli M. Handbook of Photosynthesis, Second Edition. CRC Press; 2005.
  48. 48. Tyystjärvi E. Photoinhibition of Photosystem II. Int Rev Cell Mol Biol. 2013;300: 243–303. pmid:23273864
  49. 49. Jung J, Kim H-S. The Chromophores as Endogenous Sensitizers Involved in the Photogeneration of Singlet Oxygen in Spinach Thylakoids. Photochemistry and Photobiology. 1990;52: 1003–1009.
  50. 50. Krieger-Liszkay A, Fufezan C, Trebst A. Singlet oxygen production in photosystem II and related protection mechanism. Photosynth Res. 2008;98: 551–564. pmid:18780159
  51. 51. Santabarbara S, Cazzalini I, Rivadossi A, Garlaschi FM, Zucchelli G, Jennings RC. Photoinhibition in vivo and in vitro Involves Weakly Coupled Chlorophyll—Protein Complexes. Photochemistry and Photobiology. 2002;75: 613–618. pmid:12081323
  52. 52. Vass I. Role of charge recombination processes in photodamage and photoprotection of the photosystem II complex. Physiologia Plantarum. 2011;142: 6–16. pmid:21288250
  53. 53. Schweitzer C, Schmidt R. Physical Mechanisms of Generation and Deactivation of Singlet Oxygen. Chemical Reviews. 2003;103: 1685–1758. pmid:12744692
  54. 54. Krieger-Liszkay A. Singlet oxygen production in photosynthesis. J Exp Bot. 2005;56: 337–346.
  55. 55. Vass I, Styring S, Hundal T, Koivuniemi A, Aro E-M, Andersson B. Reversible and irreversible intermediates during photoinhibition of photosystem II: stable reduced QA species promote chlorophyll triplet formation. PNAS. 1992;89: 1408–1412. pmid:11607279
  56. 56. Hoff AJ. Magnetic field effects on photosynthetic reactions. Quarterly Reviews of Biophysics. 1981;14: 599–665. pmid:7034037
  57. 57. Katz JJ, Norris JR, Shipman LL, Thurnauer MC, Wasielewski MR. Chlorophyll Function in the Photosynthetic Reaction Center. Annual Review of Biophysics and Bioengineering. 1978;7: 393–434. pmid:208458
  58. 58. Schatz GH, Brock H, Holzwarth AR. Kinetic and Energetic Model for the Primary Processes in Photosystem II. Biophysical Journal. 1988;54: 397–405. pmid:19431730
  59. 59. van Mieghem FJE, Brettel K, Hillman B, Kamlowski A, Rutherford AW, Schlodder E. Charge Recombination Reactions in Photosystem II. 1. Yields, Recombination Pathways, and Kinetics of the Primary Pair. Biochemistry. 1995;34: 4798–4813. pmid:7718587
  60. 60. Frank HA, Cogdell RJ. Carotenoids in Photosynthesis. Photochemistry and Photobiology. 1996;63: 257–264. pmid:8881328
  61. 61. Rinalducci S, Pedersen JZ, Zolla L. Formation of radicals from singlet oxygen produced during photoinhibition of isolated light-harvesting proteins of photosystem II. Biochimica et Biophysica Acta (BBA)—Bioenergetics. 2004;1608: 63–73.
  62. 62. Oguchi R, Terashima I, Kou J, Chow WS. Operation of dual mechanisms that both lead to photoinactivation of Photosystem II in leaves by visible light. Phys Plant. 2011;142: 47–55.
  63. 63. van Mieghem FJE, Nitschke W, Mathis P, Rutherford AW. The influence of the quinone-iron electron acceptor complex on the reaction centre photochemistry of Photosystem II. Biochimica et Biophysica Acta (BBA)—Bioenergetics. 1989;977: 207–214.
  64. 64. Ohnishi N, Allakhverdiev SI, Takahashi S, Higashi S, Watanabe M, Nishiyama Y, et al. Two-Step Mechanism of Photodamage to Photosystem II: Step 1 Occurs at the Oxygen-Evolving Complex and Step 2 Occurs at the Photochemical Reaction Center. Biochemistry. 2005;44: 8494–8499. pmid:15938639
  65. 65. Wu H, Cockshutt AM, McCarthy A, Campbell DA. Distinctive Photosystem II Photoinactivation and Protein Dynamics in Marine Diatoms. Plant Physiology. 2011;156: 2184–2195. pmid:21617029
  66. 66. Key T, Mccarthy A, Campbell D, Six C, Roy S, Finkel Z. Cell size trade-offs govern light exploitation strategies in marine phytoplankton. Environmental Microbiology. 2010;12: 95–104. pmid:19735282
  67. 67. Park YI, Chow WS, Anderson JM. Antenna size dependency of photoinactivation of photosystem II in light-acclimated pea leaves. Plant Physiology. 1997;115: 151–157. pmid:12223796
  68. 68. Zavafer A, Chow WS, Cheah MH. The action spectrum of Photosystem II photoinactivation in visible light. Journal of Photochemistry and Photobiology B: Biology. 2015;152: 247–260.
  69. 69. Kramer DM, Johnson G, Kiirats O, Edwards GE. New fluorescence parameters for the determination of QA redox state and excitation energy fluxes. Photosynth Res. 2004;79: 209–218. pmid:16228395
  70. 70. Kolber ZS, Prášil O, Falkowski PG. Measurements of variable chlorophyll fluorescence using fast repetition rate techniques: defining methodology and experimental protocols. Biochimica et Biophysica Acta (BBA)—Bioenergetics. 1998;1367: 88–106.
  71. 71. Ley AC, Mauzerall DC. Absolute absorption cross-sections for Photosystem II and the minimum quantum requirement for photosynthesis in Chlorella vulgaris. Biochimica et Biophysica Acta (BBA)—Bioenergetics. 1982;680: 95–106.
  72. 72. Mauzerall D, Greenbaum NL. The absolute size of a photosynthetic unit. Biochimica et Biophysica Acta (BBA)—Bioenergetics. 1989;974: 119–140.
  73. 73. Tyystjärvi E, Aro E-M. The rate constant of photoinhibition, measured in lincomycin-treated leaves, is directly proportional to light intensity. Proc Natl Acad Sci U S A. 1996;93: 2213–2218. pmid:11607639
  74. 74. Oliver RL, Whittington J, Lorenz Z, Webster IT. The influence of vertical mixing on the photoinhibition of variable chlorophyll a fluorescence and its inclusion in a model of phytoplankton photosynthesis. J Plankton Res. 2003;25: 1107–1129.
  75. 75. Sinclair J, Park YI, Chow WS, Anderson JM. Target theory and the photoinactivation of Photosystem II. Photosynthesis Research. 1996;50: 33–40. pmid:24271820
  76. 76. Blot N, Mella-Flores D, Six C, Corguillé GL, Boutte C, Peyrat A, et al. Light History Influences the Response of the Marine Cyanobacterium Synechococcus sp. WH7803 to Oxidative Stress. Plant Physiol. 2011;156: 1934–1954. pmid:21670225
  77. 77. Komenda J. The FtsH Protease slr0228 Is Important for Quality Control of Photosystem II in the Thylakoid Membrane of Synechocystis sp. PCC 6803. Journal of Biological Chemistry. 2005;281: 1145–1151. pmid:16286465
  78. 78. Komenda J, Tichy M, Prasil O, Knoppova J, Kuvikova S, de Vries R, et al. The Exposed N-Terminal Tail of the D1 Subunit Is Required for Rapid D1 Degradation during Photosystem II Repair in Synechocystis sp PCC 6803. The Plant Cell. 2007;19: 2839–2854. pmid:17905897
  79. 79. Nixon PJ, Michoux F, Yu J, Boehm M, Komenda J. Recent advances in understanding the assembly and repair of photosystem II. Ann Bot. 2010;106: 1–16. pmid:20338950
  80. 80. Herranen M, Aro E-M, Tyystjärvi T. Two distinct mechanisms regulate the transcription of photosystem II genes in Synechocystis sp. PCC 6803. Physiologia Plantarum. 2001;112: 531–539. pmid:11473713
  81. 81. Tyystjärvi T, Mulo P, Aro E-M. D1 polypeptide degradation may regulate psbA gene expression at transcriptional and translational levels in Synechocystis sp. PCC 6803. Photosynth Res. 1996;47: 111–120. pmid:24301819
  82. 82. Tyystjärvi T, Tuominen I, Herranen M, Aro E-M, Tyystjärvi E. Action spectrum of psbA gene transcription is similar to that of photoinhibition in Synechocystis sp. PCC 6803. FEBS Letters. 2002;516: 167–171. pmid:11959126
  83. 83. Tyystjärvi T, Tyystjärvi E, Ohad I, Aro E-M. Exposure of Synechocystis 6803 cells to series of single turnover flashes increases the psbA transcript level by activating transcription and down-regulating psbA mRNA degradation. FEBS Letters. 1998;436: 483–487. pmid:9801173
  84. 84. Campbell D, Bruce D, Carpenter C, Gustafsson P, Oquist G. Two forms of the photosystem II D1 protein alter energy dissipation and state transitions in the cyanobacterium Synechococcus sp PCC 7942. Photosynthesis Research. 1996;47: 131–144. pmid:24301821
  85. 85. Campbell D, Eriksson M, Oquist G. The cyanobacterium Synechococcus resists UV-B by exchanging photosystem II reaction-center D1 proteins. Proceedings of the National Academy of Sciences. 1998;95: 364–369.
  86. 86. Sicora C, Appleton S, Brown C, Chung J, Chandler J, Cockshutt A, et al. Cyanobacterial psbA families in Anabaena and Synechocystis encode trace, constitutive and UVB-induced D1 isoforms. BBA—Bioenerg. 2006;1757: 47–56.
  87. 87. Allakhverdiev SI, Murata N. Environmental stress inhibits the synthesis de novo of proteins involved in the photodamage—repair cycle of Photosystem II in Synechocystis sp. PCC 6803. Biochimica et Biophysica Acta (BBA)—Bioenergetics. 2004;1657: 23–32.
  88. 88. Nishiyama Y, Murata N. Revised scheme for the mechanism of photoinhibition and its application to enhance the abiotic stress tolerance of the photosynthetic machinery. Appl Microbiol Biotechnol. 2014; 1–20.
  89. 89. Nishiyama Y, Allakhverdiev SI, Murata N. Inhibition of the repair of Photosystem II by oxidative stress in cyanobacteria. Photosynth Res. 2005;84: 1–7. pmid:16049747
  90. 90. Nishiyama Y, Allakhverdiev S, Murata N. A new paradigm for the action of reactive oxygen species in the photoinhibition of photosystem II. Biochimica et Biophysica Acta. 2006;1757: 742–749. pmid:16784721
  91. 91. Dau H, Zaharieva I. Principles, Efficiency, and Blueprint Character of Solar-Energy Conversion in Photosynthetic Water Oxidation. Acc Chem Res. 2009;42: 1861–1870. pmid:19908828
  92. 92. Li G, Brown CM, Jeans J, Donaher N, McCarthy A, Campbell DA. The Nitrogen Costs of Photosynthesis in a Diatom under Current and Future pCO2. New Phytologist. 2015;205: 533–543. pmid:25256155
  93. 93. Raven JA. A cost-benefit analysis of photon absorption by photosynthetic unicells. New Phytologist. 1984;98: 593–625.
  94. 94. Raven JA. The cost of photoinhibition. Physiologia Plantarum. 2011;142: 87–104. pmid:21382037
  95. 95. Neale PJ, Thomas BC. Inhibition by Ultraviolet and Photosynthetically Available Radiation Lowers Model Estimates of Depth-Integrated Picophytoplankton Photosynthesis: Global Predictions for Prochlorococcus and Synechococcus. Global Change Biology. 2016;
  96. 96. Neale PJ, Pritchard AL, Ihnacik R. UV effects on the primary productivity of picophytoplankton: biological weighting functions and exposure response curves of Synechococcus. Biogeosciences. 2014;11: 2883–2895.
  97. 97. Six C, Finkel ZV, Irwin AJ, Campbell DA. Light Variability Illuminates Niche-Partitioning among Marine Picocyanobacteria. Plos One. 2007;2.
  98. 98. Rippka R, Coursin T, Hess W, Lichtlé C, Scanlan DJ, Palinska KA, et al. Prochlorococcus marinus Chisholm et al. 1992 subsp. pastoris subsp. nov. strain PCC 9511, the first axenic chlorophyll a2/b2-containing cyanobacterium (Oxyphotobacteria). Int J Syst Evol Microbiol. 2000;50: 1833–1847. pmid:11034495
  99. 99. Lin S. Algal Culturing Techniques. Journal of Phycology. 2005;41: 906–908.
  100. 100. Moore LR, Post AF, Rocap G, Chisholm SW. Utilization of different nitrogen sources by the marine cyanobacteria Prochlorococcus and Synechococcus. Limnology and oceanography. 2002;47: 989–996.
  101. 101. Crespi JM. Some guidelines for the practical application of Fry’s method of strain analysis. Journal of Structural Geology. 1986;8: 799–808.
  102. 102. Bachmann KM, Ebbert V, Adams WW III, Verhoeven AS, Logan BA, Demmig-Adams B. Effects of lincomycin on PSII efficiency, non-photochemical quenching, D1 protein and xanthophyll cycle during photoinhibition and recovery. Funct Plant Biol. 2004;31: 803–813.
  103. 103. Ni G, Zimbalatti G, Murphy CD, Barnett AB, Arsenault CM, Li G, et al. Arctic Micromonas uses protein pools and non-photochemical quenching to cope with temperature restrictions on Photosystem II protein turnover. Photosynthesis Research. 2016;
  104. 104. Elzhov TV, Mullen KM, Spiess A-N, Bolker B. minpack.lm: R interface to the Levenberg-Marquardt nonlinear least-squares algorithm found in MINPACK, plus support for bounds [Internet]. 2013. http://CRAN.R-project.org/package=minpack.lm
  105. 105. Vass I, Cser K. Janus-faced charge recombinations in photosystem II photoinhibition. TIPS. 2009;14: 200–205.
  106. 106. Huner NP, Öquist G, Sarhan F. Energy balance and acclimation to light and cold. Trends in Plant Science. 1998;3: 224–230.
  107. 107. van Kooten O, Snel JFH. The use of chlorophyll fluorescence nomenclature in plant stress physiology. Photosynthesis Research. 1990;25: 147–150. pmid:24420345
  108. 108. Oxborough K, Baker NR. Resolving chlorophyll a fluorescence images of photosynthetic efficiency into photochemical and non-photochemical components—calculation of qP and Fv-/Fm-; without measuring Fo-; Photosynthesis Research. 1997;54: 135–142.
  109. 109. Ware MA, Belgio E, Ruban AV. Photoprotective capacity of non-photochemical quenching in plants acclimated to different light intensities. Photosynthesis Research. 2015;126: 261–74. pmid:25702085
  110. 110. Murphy C, Ni G, Li G, Barnett A, Xu K, Grant-Burt J, et al. Quantitating active Photosystem II reaction centre content from fluorescence induction transients. Limnology and Oceanography: Methods. 2016;
  111. 111. Ware MA, Belgio E, Ruban AV. Photoprotective capacity of non-photochemical quenching in plants acclimated to different light intensities. Photosynth Res. 2015;126: 261–274. pmid:25702085
  112. 112. Maxwell D, Falk S, Huner N. Photosystem II Excitation Pressure and Development of Resistance to Photoinhibition (I. Light-Harvesting Complex II Abundance and Zeaxanthin Content in Chlorella vulgaris). Plant Physiology. 1995;107: 687–694. pmid:12228392
  113. 113. Suggett D, MacIntyre H, Kana T, Geider R. Comparing electron transport with gas exchange: parameterising exchange rates between alternative photosynthetic currencies for eukaryotic phytoplankton. AME. 2009;56: 147–162.
  114. 114. Suggett DJ, Moore CM, Geider RJ. Estimating Aquatic Productivity from Active Fluorescence Measurements. In: Suggett DJ, Prášil O, Borowitzka MA, editors. Chlorophyll a Fluorescence in Aquatic Sciences: Methods and Applications. Dordrecht: Springer Netherlands; 2010. pp. 103–127. http://link.springer.com/10.1007/978-90-481-9268-7_6
  115. 115. Umena Y, Kawakami K, Shen J-R, Kamiya N. Crystal structure of oxygen-evolving photosystem II at a resolution of 1.9 A. Nature. 2011;473: 55–60. pmid:21499260
  116. 116. Amthor J. The McCree—de Wit—Penning de Vries—Thornley Respiration Paradigms: 30 Years Later. Annals of Botany. 2000;86: 1–20.
  117. 117. Hachiya T, Terashima I, Noguchi K. Increase in respiratory cost at high growth temperature is attributed to high protein turnover cost in Petunia hybrida petals. Plant, Cell & Environment. 2007;30: 1269–1283.
  118. 118. Vries FWTPD. The Cost of Maintenance Processes in Plant Cells. Ann Bot. 1975;39: 77–92.
  119. 119. Miyata K, Noguchi K, Terashima I. Cost and benefit of the repair of photodamaged photosystem II in spinach leaves: roles of acclimation to growth light. Photosynth Res. 2012;113: 165–180. pmid:22797856
  120. 120. Noguchi K, Nakajima N, Terashima I. Acclimation of leaf respiratory properties in Alocasia odora following reciprocal transfers of plants between high- and low-light environments. Plant, Cell and Environment. 2001;24: 831–839.
  121. 121. Zerihun A, McKenzie BA, Morton JD. Photosynthate costs associated with the utilization of different nitrogen-forms: influence on the carbon balance of plants and shoot-root biomass partitioning. New Phytologist. 1998;138: 1–11.
  122. 122. Bruckner RC, Gunyuzlu PL, Stein RL. Coupled Kinetics of ATP and Peptide Hydrolysis by Escherichia coli FtsH Protease. Biochem. 2003;42: 10843–10852.
  123. 123. Campbell DA, Hossain Z, Cockshutt AM, Zhaxybayeva O, Wu H, Li G. Photosystem II protein clearance and FtsH function in the diatom Thalassiosira pseudonana. Photosynth Res. 2013;115: 43–54. pmid:23504483
  124. 124. Tyystjarvi E. Photoinhibition of Photosystem II and photodamage of the oxygen evolving manganese cluster. Coordination Chemistry Reviews. 2008;252: 361–376.
  125. 125. Vassiliev IR, Prasil O, Wyman KD, Kolber Z, H AK Jr, Prentice JE, et al. Inhibition of PS II photochemistry by PAR and UV radiation in natural phytoplankton communities. Photosynth Res. 1994;42: 51–64. pmid:24307468
  126. 126. Bailey S, Melis A, Mackey KRM, Cardol P, Finazzi G, van Dijken G, et al. Alternative photosynthetic electron flow to oxygen in marine Synechococcus. Biochimica et Biophysica Acta (BBA)—Bioenergetics. 2008;1777: 269–276.
  127. 127. Zorz JK, Allanach JR, Murphy CD, Roodvoets MS, Campbell DA, Cockshutt AM. The RUBISCO to Photosystem II Ratio Limits the Maximum Photosynthetic Rate in Picocyanobacteria. Life. 2015;5: 403–417. pmid:25658887
  128. 128. R Core Team. R: A Language and Environment for Statistical Computing [Internet]. Vienna, Austria: R Foundation for Statistical Computing; 2015. http://www.R-project.org/
  129. 129. Loebl M, Cockshutt AM, Campbell DA, Finkel ZV. Physiological basis for high resistance to photoinhibition under nitrogen depletion in Emiliania huxleyi. Limnol Oceanogr. 2010;55: 2150–2160.
  130. 130. Gao K, Xu J, Gao G, Li Y, Hutchins DA, Huang B, et al. Rising CO2 and increased light exposure synergistically reduce marine primary productivity. Nature Clim Change. 2012;2: 519–523.
  131. 131. Behrenfeld MJ, Maran E, Siegel DA, Hooker SB. Photoacclimation and nutrient-based model of light-saturated photosynthesis for quantifying oceanic primary production. Mar Ecol Prog Ser. 2002;228: 103–117.
  132. 132. Schuback N, Flecken M, Maldonado MT, Tortell PD. Diurnal variation in the coupling of photosynthetic electron transport and carbon fixation in iron-limited phytoplankton in the NE subarctic Pacific. Biogeosciences. 2016;13: 1019–1035.
  133. 133. Gómez-Baena G, López-Lozano A, Gil-Martínez J, Lucena J, Diez J, Candau P, et al. Glucose Uptake and Its Effect on Gene Expression in Prochlorococcus. PLoS ONE. 2008;3: e3416. pmid:18941506