Direct measurements of gross primary productivity (GPP) in the water column are essential, but can be spatially and temporally restrictive. Fast repetition rate fluorometry (FRRf) is a bio-optical technique based on chlorophyll a (Chl-a) fluorescence that can estimate the electron transport rate (ETRPSII) at photosystem II (PSII) of phytoplankton in real time. However, the derivation of phytoplankton GPP in carbon units from ETRPSII remains challenging because the electron requirement for carbon fixation (Фe,C), which is mechanistically 4 mol e− mol C−1 or above, can vary depending on multiple factors. In addition, FRRf studies are limited in freshwater lakes where phosphorus limitation and cyanobacterial blooms are common. The goal of the present study is to construct a robust Фe,C model for freshwater ecosystems using simultaneous measurements of ETRPSII by FRRf with multi-excitation wavelengths coupled with a traditional carbon fixation rate by the 13C method. The study was conducted in oligotrophic and mesotrophic parts of Lake Biwa from July 2018 to May 2019. The combination of excitation light at 444, 512 and 633 nm correctly estimated ETRPSII of cyanobacteria. The apparent range of Фe,C in the phytoplankton community was 1.1–31.0 mol e− mol C−1 during the study period. A generalised linear model showed that the best fit including 12 physicochemical and biological factors explained 67% of the variance in Фe,C. Among all factors, water temperature was the most significant, while photosynthetically active radiation intensity was not. This study quantifies the in situ FRRf method in a freshwater ecosystem, discusses core issues in the methodology to calculate Фe,C, and assesses the applicability of the method for lake GPP prediction.
Citation: Kazama T, Hayakawa K, Kuwahara VS, Shimotori K, Imai A, Komatsu K (2021) Development of photosynthetic carbon fixation model using multi-excitation wavelength fast repetition rate fluorometry in Lake Biwa. PLoS ONE 16(2): e0238013. https://doi.org/10.1371/journal.pone.0238013
Editor: Bruno Jesus, University of Nantes, FRANCE
Received: August 4, 2020; Accepted: January 19, 2021; Published: February 2, 2021
Copyright: © 2021 Kazama et al. This is an open access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited.
Data Availability: All relevant data are within the paper and its Supporting Information files.
Funding: TK, KH, KS and AI were supported by the Collaborative Research Fund from Shiga Prefecture entitled “Study on water quality and lake-bottom environment for protection of the soundness of water environment” under the Japanese Grant for Regional Revitalization, and the Environment Research and Technology Development Fund (No. 5-1607) of the Ministry of the Environment, Japan. https://www.kantei.go.jp/jp/singi/tiiki/tiikisaisei/souseikoufukin.html.
Competing interests: The authors have declared that no competing interests exist.
Phytoplankton are the most important primary producers in the aquatic food web . Changes in phytoplankton primary productivity can affect the food chain length [2, 3], material cycles [4, 5] and biomass of higher trophic organisms [6–8]. Phytoplankton community productivity is affected by various environmental factors and must rapidly respond to them [9–11] due to high growth rates and short generation times . To evaluate the effect of variability in environmental factors on aquatic communities and ecosystems, continuous observation of phytoplankton primary productivity is necessary [4, 7, 13]
Traditional chemical methods of measuring primary production, such as the 14C method , the 13C method [15, 16], the light-dark bottle method  and the 18O method , require handling a radioisotope (14C) and/or an incubation time of several hours. Thus, primary production studies using these techniques can be limiting when attempting to assess temporal and spatial variability. Fast repetition rate fluorometry (FRRf; Table 1), a chlorophyll a fluorescence-based method, has been developed as an advanced bio-optical technique for real-time measurement of phytoplankton primary productivity, mainly in marine ecosystems [19–27]. The FRRf method enables the induction and measurement of a range of chlorophyll a fluorescence yields and parameters specific to photosystem II (PSII) [19, 20, 28], and, in turn, enables estimation of the in vivo electron transport rate in PSII (ETRPSII) and gross primary productivity (GPP) by theoretical models of photosynthesis [19, 28, 29].
Previous studies demonstrated that GPP estimated from FRRf measurements correlated well with results from conventional methods, including the 13C method [25, 26, 30, 31] and the light-dark bottle method . However, FRRf measurements tended to overestimate GPP compared with the 14C and the 13C methods, while underestimating them when compared with the light-dark bottle and the 18O methods . These discrepancies in GPP measurements are dependent on the targeted products, namely, oxygen or particulate organic carbon, in the photosynthesis cycle . To account for the measurement discrepancies, recent studies have examined the electron requirement for carbon fixation (Фe,C, also called Kc) by comparing the FRRf-derived ETRPSII per unit volume (JVf) to the GPP rate by traditional methods [25–27, 34]. The Фe,C is affected by multiple spatiotemporal variations in physical and chemical factors [35–40], and by phytoplankton community composition [26, 41–44]. For example, Фe,C is higher in the open ocean than in coastal areas due to differences in the light environment conditions; light availability is higher in open oceans . Light availability can be affected by the concentrations of colored dissolved organic matter (CDOM), non-algal particles, and phytoplankton. Moreover, the vertical distribution of phytoplankton is markedly different in open-ocean and coastal areas, where the former has peak biomass located in a much deeper area with less CDOM and non-algal particles in the water column, allowing more light availability . More specifically, excess light energy enhances photo-oxidative damage and alternative electron transport such as the Mehler reaction, flavodi-iron protein-mediated electron flows and the plastiquinol terminal oxidase (PTOX) pathway, which can increase Фe,C [33, 45]. In addition to ambient light conditions, nutrients can also play an important role in determining Фe,C of the phytoplankton community [27, 39]. For example, Schuback et al.  described the negative relationships between Фe,C and nitrate concentrations in the Arctic Ocean, suggesting the variable effects of nutrient availability. The multitude of interacting factors affecting the value of Фe,C for converting JVf to GPP make it difficult to establish a general model applicable to different ecosystems . Therefore, to construct a robust JVf -GPP model, it is necessary to accumulate FRRf and its corresponding GPP data in various aquatic environments.
In terms of physicochemical and biological conditions, freshwater ecosystems differ considerably from marine ecosystems. For example, cyanobacteria (blue-green algae) can frequently form dense surface blooms in meso–eutrophic lakes [46, 47]. Previous studies have suggested that cyanobacterial blooms can significantly affect ETRPSII measurements due to spectral mismatch between FRRf excitation wavelengths and the absorption spectrum of cyanobacteria [21, 26, 36, 41, 48]. For example, Raateoja et al.  found that filamentous cyanobacteria Nodularia spumigena and Aphanizomenon sp. had absorption peaks around 630 nm, and the photosynthetic activity of these species could not be measured by FRRf with an excitation light around 475 nm (targeting Chl-a). Cyanobacteria have multiple absorption peaks around 500–570 nm and 630 nm based on antenna pigments . Moreover, the blue light (< 500 nm) absorbed by cyanobacterial antenna pigments does not make a major contribution to the reduction of the QA and PQ pool, and O2 evolution . Thus, it is critical that the FRRf excitation wavelengths correspond to the absorption spectrum of cyanobacteria (or the dominant group) for accurate estimation of primary productivity and model development in freshwater ecosystems [21, 41, 51].
Phytoplankton primary productivity is also more likely to be phosphorus-limited in freshwater ecosystems [52, 53], while more likely to be nitrogen-limited in marine environments [54, 55]. Whereas nitrogen limitation depresses cellular Chl-a concentration, phosphorus limitation inhibits RNA and ATP synthesis, which can affect protein synthesis and photochemical energy conversion in algae. [56, 57]. In fact, Фe,C of marine phytoplankton increases under nitrogen limitation [27, 39]. Regrettably, the influence of phosphorus stoichiometry on Фe,C in freshwater phytoplankton remains unknown, and FRRf studies in freshwater environments in general are still limited [58–60]. Owing to the differences between marine and freshwater ecosystems, it is essential to employ suitable excitation wavelength combinations and measure phosphorus concentration in the water column to correctly estimate both the ETRPSII and GPP of freshwater phytoplankton communities.
The goal of the present study is to construct a robust Фe,C model applicable to freshwater ecosystems using simultaneous measurements of ETRPSII by FRRf coupled with the traditional carbon fixation rate by the 13C method in Lake Biwa. In this context, we first evaluated the performance of FRRf with multi-excitation wavelengths (444, 512, and 633 nm; S1A Appendix) during cyanobacterial blooms. Then, we evaluated the relative importance of variable environmental and biological factors, including phosphorus concentration in the water column, by determining Фe,C by statistical models with multiple variables. This study shows the utility of in situ FRRf measurements using an excitation wavelength of 633 nm during cyanobacterial blooms, and the extent to which physicochemical factors and phytoplankton community composition influence Фe,C estimation.
Materials and methods
No permits were required for the described study, because the location was not privately-owned or protected, and the field studies did not involve endangered or protected species.
The study was conducted at Lake Biwa (670 m2 surface area with a mean depth of 43 m) on Honshu Island, Japan (Fig 1). The North Basin is a deep, oligotrophic area, while the South Basin is a shallow, mesotrophic area . Phytoplankton communities differ markedly between the two basins, especially in terms of cyanobacterial abundance . Sampling was carried out at the long-term survey stations, 12B (62 m depth) and 17B (89 m depth) in the North Basin, and at 6B (4 m depth) and 9B (5.6 m depth) in the South Basin, from July 2018 to May 2019 (Table 2). No permits were required to sample the lake in this study.
Vertical profiles of water temperature, pH, dissolved oxygen concentration, and specific conductivity were measured using a water quality sonde (EXO2; Xylem, Inc., Yellow Springs, OH, USA). At stations 12B and 17B, water samples were collected with a bucket at 0 m, with 10-L Niskin samplers at 2.5 m, and with 5-L Niskin bottles on a rosette sampler (AWS; JFE Advantech Co. Ltd., Kobe, Japan) at 5, 10, 15 and 20 m after in situ FRRf measurement (described below). Likewise, at stations 6B and 9B, water samples were collected with a bucket at 0 m, and with an electric pump at 2 and 3 m (6B) or 4 m (9B).
Macro-nutrients and dissolved inorganic carbon (DIC) concentrations were determined from an aliquot of a 100 mL subsample collected at each depth, and immediately filtered through a syringe-type membrane filter (0.2 μm pore size, Acrodisc syringe filter; Pall Corporation, Ann Arbor, MI, USA) using clean techniques. The filtered samples were stored at −20°C until nitrate, nitrite, ammonia and phosphate analyses using an ion chromatograph system (Dionex Integrion HPIC system; Thermo Scientific, Waltham, MA, USA). DIC was analysed using a total carbon analyzer (TOC-L; Shimadzu, Kyoto, Japan). For chlorophyll a (Chl-a) analysis, 50–200 mL samples were filtered onto a 25-mm glass-fibre filter (0.7 μm nominal pore size, GF/F; GE Healthcare, UK Inc., Little Chalfont, UK). Chl-a was extracted with N,N-dimethylformamide for 24 h in the dark  and then stored at −80°C. The Chl-a concentration was determined with a 10-AU fluorometer (Turner Designs, Sunnyvale, CA, USA).
We measured photosynthetically active radiation (PAR, 400–700 nm) underwater from a depth of 30 m to the surface using a 2π PAR sensor (CTG Ltd., West Molesey, UK) along with the FRR fluorometer. We determined the diffuse attenuation coefficient Kd (m−1) with an exponential function as follows: (1) where Ebot and Etop are incident PAR (μmol photon m−2 s−1) at the bottom and top of the sampling layer, respectively, and dZ is the thickness of the layer. When the logarithmic slope of Kd did not change with depth, it was calculated as EZ = E0 exp (–Kd×dZ), where E0 is PAR at 0 m. When the logarithmic slope of Kd significantly changed with depth, we divided the water column into two layers at the depth where Kd changed and calculated it for each layer (Table 2).
FRRf measurements and photophysiological parameters
In situ induced Chl-a fluorescence profiles were measured vertically with a multi-excitation wavelength fast repetition rate fluorometer (FRRf) system (FastOcean, S/N 17-0053-002; CTG Ltd., UK). The field-type FRRf was equipped with two chambers for ambient light and dark readings. To remove ambient light noise, an optical bandpass filter (<670 nm) was attached above the light chamber. The dark chamber has black housing and piping with a pump to ensure that samples are measured under completely dark conditions after 1–2 s of dark adaptation. Each chamber has three light-emitting diodes (LED) providing flash excitation energy centred at 444, 512 and 633 nm (S1A Appendix). Here, 444 nm (blue) corresponds to the absorption peak of Chl-a, while 512 nm (green) and 633 nm (orange) correspond to the absorption peaks of phycoerythrins and phycocyanins . We employed four LED combinations to evaluate the green and orange excitation flashes: (1) 444 nm, (2) 444 and 512 nm, (3) 444 and 633 nm, and (4) 444, 512 and 633 nm. We applied a single turnover method, which was consistent with a saturation phase (100 flashlets with 2 μs pitch) and a relaxation phase (40 flashlets with 50 μs pitch). This sequence was repeated eight times with a 100-ms interval for each LED combination. All combinations were repeated at least five times every 5 m from 20 to 10 m and every 2 m from 10 m to the surface at 12B and 17B, and every 0.5 m from the bottom to the surface layer at 6B and 9B during the up-cast, respectively. The power of flashlets (EFRRf) and the gain of the extra high tension of the photomultiplier tube (PMT eht) were optimised by FastPro8 software (version 1.0.50; CTG Ltd.). All FRRf measurements were performed between 09:30 and 11:30 (Table 2).
The concentration of PSII reaction centre (RCII, nmol m−3) was estimated fluorometrically according to Oxborough et al.  as follows: (2) where KR is an instrument-specific constant (photons m−3 s−1), Fo is the fluorescence intensity at the zeroth flashlet of a single turnover measurement when all RCII are open, and σPSII is the absorption cross section of PSII photochemistry in the dark (m2). A recent study showed that KR/EFRRf can vary among phytoplankton taxonomic groups and growth conditions, and affect the estimation of productivity . In this study, we did not examine sample-specific KR/EFRRf values. Instead, we used a constant value as in the work of Wei et al. , and taxonomic group and nutrients were assessed as the factors affecting Фe,C by a statistical model approach (mentioned below).
The RCII-specific rate of electron transport based on FRRf (Jf, μmol electrons nmol RCII−1 s−1) was calculated based on the Sigma Algorithm installed in FastPro8 [28, 36]: (3) where E is the incident PAR at each sampling depth (μmol photon m−2 s−1), σPSII′ is the absorption cross section of PSII photochemistry under ambient light (m2), and (1 − C) is the fraction of RCII in the open state, which is assumed to be qP (= (F´−FO´)/(Fm´−FO´)). Thus, the electron transport rate per water volume (JVf, μmol electrons m−3 s−1) was derived by Jf × RCII. Special permission is required for in situ bottle incubations in Lake Biwa, limiting our ability to conduct approximate time-dependent comparisons. Thus, we conducted bottle incubation measurements of carbon fixation and oxygen production rates after returning to the laboratory from 14:00 to 18:00 close to the same time of day (Table 2). Previous studies suggested that the diel changes in Jf are relatively small during the daytime [66, 67]. To check the diel changes in Jf of the phytoplankton community in Lake Biwa, we conducted extra measurements of the Jf in the laboratory (at the start of bottle incubation) using the Act2 system (CTG, Inc.) on 28th January, 19th April and 10th May in 2019, and confirmed that the Jf were quite comparable between in situ and laboratory conditions (S2 Appendix).
Phytoplankton can dissipate excessive energy as heat in PSII, and after PSII through alternative electron flows (AEFs) such as the Mehler reaction (for reviews, see [33, 68]). Among these, the proportion of heat dissipation relative to the total absorbed energy was estimated as the normalised Stern–Volmer quenching coefficient (NPQNSV), which is equal to FO′/Fv′ . This is commonly used to compare non-photochemical quenching among phytoplankton communities that have different light histories [27, 38, 70]. Finally, the maximum quantum efficiency of PSII was evaluated by Fv/Fm . It should be noted that, according to previous studies, PSII fluorescence of cyanobacteria could be lower under dark conditions due to the lag time associated with the transition from an illuminated to a dark state (State 1 to State 2) expressed in seconds to minutes [72–74]. Thus, when cyanobacteria are dominant in a community, FO and FO′ could be overestimated , and cause underestimation of qP but overestimation of NPQNSV and RCII.
Evaluation of excitation wavelength combination
To assess the performance of the four wavelength combinations in the natural phytoplankton communities, we compared the minimum fluorescence yield Fo measured at each wavelength combination during cyanobacterial blooms (at 9B on 28th August in 2018), and when diatoms and zygnematophytes dominated (at 12B on 13th September and at 6B on 18th September in 2018). We also compared electron transport rates estimated by FRRf (JVf, μmol e− m−3 s−1) and by the light-dark bottle method (JVO, μmol e− m−3 s−1)  to verify the accuracy of the estimated JVf.
The light-dark bottle method is known to underestimate GPP due to differences in respiration rate between dark and light conditions [77, 78], and oxygen oversaturation . Nevertheless, since the fixation of one molecule of CO2 theoretically requires at least four electrons through photosynthesis, the method is still practical to determine whether or not the JVf determined by the FRRf was underestimated. Water samples from each layer were poured into two or four 100-mL glass bottles. To measure the community respiration rate, another aliquot of sample water from each layer was poured into two 100-mL dark bottles. All bottles were incubated for 3 h in a growth chamber (HCLP-880PF; Nippon Medical and Chemical Instruments Co., Ltd., Osaka, Japan). Oxygen concentration of each bottle was measured by the optical oxygen spots and probe (Fibox 4; PreSens, Regensburg, Germany) before and after incubation. JVO was derived as follows: (4) where NPO is net oxygen evolution rate (mg O2 m−3 h−1), Rd is dark respiration rate (mg O2 m−3 h−1), and 3.47×10−2 is a conversion factor from hours to seconds, from mg O2 to μmol O2, and 4 mol e− for 1 mol O2 evolution. Plots of JVO against light intensity were fitted in a two-parameter model, as described by Webb et al. .
Additionally, quality control of all FRRf data measured with each excitation combination was assessed by the probability of an RCII being closed during the first flashlet of a single turnover saturation phase under dark (RσPSII) and ambient light (RσPSII′) by FastPro8 software. Although FastPro8 adjusted RσPSII and RσPSII′ around 0.05, these values changed in a manner dependent on depth, light environment, and phytoplankton community composition. Thus, we compared the number of successful observations, RσPSII and RσPSII ′, among four combinations after rejecting extremely low-quality data (RσPSII or RσPSII ′ <0.03 or >0.08).
Phytoplankton identification and enumeration
For enumerating phytoplankton, 50 mL of each sample was fixed with Lugol’s solution (1% final concentration). After 24 h of settling in the dark, the supernatant was removed gently and the sample was concentrated to 15 mL. Cells were counted under a light microscope at ×200 magnification where the size and volume of cells for each group were measured using cellSens software (Olympus, Tokyo, Japan) based on the work of Hillebrand et al. . All phytoplankton species were categorized into eight groups: diatoms, cyanophytes, small chlorophytes, zygnematophytes, cryptophytes, chrysophytes, dinoflagellates and euglenophytes. The phytoplankton community composition was assessed based on the carbon biomass converted from the biovolume .
13C uptake rate
Gross primary production per water mass (GPC, mg C m−3 h−1) was determined by a 13C-based method based on Hama et al. . Water samples from each layer were taken to the laboratory and poured into two or four 500-mL polycarbonate bottles (Nalgene, Rochester, NY, USA), and spiked with NaH13CO3 to a final concentration of ca. 10% of ambient total inorganic carbon . Incubations were initiated within 3 h after samples had been collected. Production experiments were conducted in incubators where the temperature and light environment were controlled in a growth chamber along with an oxygen evolution experiment. Incubation PAR levels were set as in Table 3. Incubation PAR intensity was manipulated using black mesh filters covering polycarbonate bottles. Incubation temperature was set to the mean of respective sampling depths. The samples from 12B on 23rd July and 17B on 30th July were incubated under ambient light percentages (described above) and temperature on the balcony of Lake Biwa Environmental Research Institute (Shiga, Japan). Although incubation temperature was not controlled on 23rd and 30th July, it changed <1.5°C during the incubations.
All incubations were conducted for 3 h. After each incubation period, water samples were filtered through pre-combusted (at 450°C for 4 h) 25-mm glass-fibre filters (0.7 μm nominal pore size, GF/F). The filters were stored at −20°C until final analysis. The carbon stable isotope ratio δ13C was measured using a Delta V Advantage isotope ratio mass spectrometer coupled with a Conflo IV interface and a Flash 2000 elemental analyzer (Thermo Fisher Scientific, Waltham, MA, USA) at the Isotope Research Institute (Yokohama, Japan). GPC was calculated according to Hama et al. . To compare with the measured Jf in Eq (3), GPC was converted to RCII-specific primary production rate (PBC, mg C nmol RCII−1 h−1) as follows: (5)
To account for the difference in spectral distribution and primary production response between ambient light field and artificial incubator light sources, we applied a spectral correction to the data set to reduce any possible discrepancies between the methods. First, to correct the differences in the spectral distribution of excitation flash of FRRf and ambient light in the water column, σPSII was adjusted by the spectral correction factor (SCF) following previous studies [27, 34]: (6) where is the Chl-a specific absorption spectrum of phytoplankton (m2 mg Chl-a−1), and Ein situ (λ) and EFRRf (λ) are the spectral distribution of irradiance in the water column and excitation flash of FRRf, respectively. The and Ein situ (λ) were estimated from models described in previous studies where the spectral irradiance in the water column was estimated as follows [84, 85]: (7) where λ is wavelength between 400 and 700 nm, aW, aCDOM and aNAP are absorption spectra of pure water, CDOM and non-algal particles, respectively (m−1), chl is Chl-a concentration (mg m−3) and z is depth (m). was estimated for each date and depth by Paavel’s model  for August, and Ylöstalo’s model  for other months, in accordance with the species composition of the phytoplankton community (S3 Appendix). In Lake Biwa, Anabaena affinis and Aphanothece sp. dominated >90% of the cyanobacterial biomass at 0 and 2 m, respectively, in August 2018. The former species has phycocyanin (PC) , whereas the latter has PC and phycoerythrin (PE) [88, 89]. Paavel et al.  described a summer cyanobacterial bloom that consisted of Anabaena, Aphanizomenon, and Gloeotrichia. The former two species have PC , and later species has PC and PE . We tested the of pure Anabaena  culture in August 2018 in Lake Biwa, but the SCF changed to only 3%. We believe that Paavel et al. coefficients are better for the abovementioned reason.
The aW was estimated by a common spectral model determined by Pope and Fry  (S4A Appendix). The aCDOM was estimated by the equation aCDOM = aCDOM (320) exp(-S(λ-320)) . We used previously measured, average values of limnetic sites from each basin, 1.03 and 2.28, for aCDOM (320) for the North Basin and the South Basin, and 0.017 for S [85, 92] (S4B Appendix). aNAP was estimated as aNAP = aNAP (440) exp(-S(λ-440)) . We used 0.264 for aNAP (440) and 0.004 for S as typical values for the area (S4C Appendix). The calculated Ein situ(λ,z) was adjusted with observed PAR intensity at each depth during each sampling date.
For the spectral distribution of incident sunlight E0 (λ) on each sampling date, we referred to the solar radiation spectrum database of central Japan in 2015 . To fit the incident angle of sunlight and the weather conditions on each sampling date, we used spectral data at 10 AM on 30th January, 9th February, 18th April, 17th May, 2nd and 31st July, 26th August, 7th and 19th September, 10th and 26th October, 10th November, and 9th and 19th December corresponding to each sampling date (S5 Appendix). For spectral irradiance during 13C incubation on 23rd and 30th July, we used spectral data at 4 PM on 2nd and 31st July from the database.
Calculated SCFs are listed in the S1 Table. The SCF for PAR intensity of each growth chamber was also adjusted with the spectral distribution of the light source (S1B Appendix) and in the same manner as in Eq (6).
Derivation of photosynthetic parameters
To calculate Фe,C (mol e− mol C−1) from Jf and PBC assessed at different light levels, photosynthesis versus irradiance curves (P-E curves) were obtained by curve-fitting using two P-E models. When Jf or PBC showed photoinhibition (i.e. decreasing Jf or PBC with increasing E after the light-saturated phase), P-E curves were fitted in a three-parameter model, as described in earlier studies [95–97]. When there was no photoinhibition, P-E curves were fitted in a two-parameter model as described by Webb et al. .
It should be noted that the phytoplankton community structures were occasionally different among the layers of the water column, but the relationships between Jf or PBC and E were well fitted in the photosynthesis models, as in previous studies [25, 30]. All parameters in the fitted models were calculated by function nls() in R ver. 3.4.3 . The PBC values corresponding to underwater E of in situ FRRf measurements were extracted from the P-E curves. PBC can be functioned by Jf with electron requirement for carbon fixation (Фe,C) as follows: (8) where 43.2 is the conversion factor from seconds to hours, and from μmol C to mg C.
Data transformation and GLM for Фe,C
Because FRRf measurements were inhibited by high light intensity (typically >1,000 μmol photons m−2 sec−1), presumably there were sampling biases between shallow and deep layers. To avoid such bias, we subsampled 240 observations from the data set on each sampling date by bootstrap sampling with replacements: 60 observations from four layers above the euphotic zone (0–3.75, 3.75–7.5, 7.5–12.5 and 12.5–17.5 m) for the North Basin and 80 observations from three layers (0–1, 1–3 and 3–5.5 m) for the South Basin. Here a total of 3360 observations (1680 observations for the North Basin and 1680 observations for the South Basin) were used in all analyses of this study.
As in Eq (8), Фe,C is defined as Jf /PBc × 43.2. We modelled Фe,C using a generalised linear model (GLM) with gamma error distribution and a log-link function using the glm() function in R. We treated Фe,C as the dependent variable and environmental factors as the explanatory variables. To avoid collinearity between the explanatory variables, Spearman’s ρ between all candidate factors was tested with a significance level of p < 0.05, and parameters with ρ ≥ 0.7 were regarded as collinear variables. We selected water temperature, PAR, turbidity, dissolved oxygen (DO), NH4, NO3 + NO2, PO4, Fv/Fm, σPSII, Chl-a, and the fractions of diatom, cyanobacteria and cryptophytes in the phytoplankton community as the explanatory variables in GLM. Explanatory variables were standardised (mean 0 and standard deviation 1) after log transformation. NH4 concentration and the fraction of phytoplankton group biomass lower than the detection limit were treated as 0.1 μmol L−1 and 0.1%, respectively. Multicollinearity of variables was further tested with the variance inflation factor (VIF)  using vif() in the package ‘car’  in R. A set of all possible sub-models was generated with the dredge() function in the package ‘MuMIn’ , and the sub-models were ranked based on the Akaike information criterion (AIC) .
Evaluation of excitation wavelength combination
Vertical profiles of temperature showed weak stratification at Station 9B on 28th August and at Station 12B on 13th September (Fig 2A and 2D), but not at Station 6B on 18th September (Fig 2G). Chl-a concentration reached 42 μg L−1 at 2 m at Station 9B due to a cyanobacterial bloom (Fig 2C). Vertical profiles of the minimum PSII fluorescence yield (Fo) showed variability among four combinations of excitation wavelengths during cyanobacterial blooms (Fig 2B), but not for communities dominated by diatoms and zygnematophytes (Fig 2E and 2H). For example, Fo values derived from excitation light at 444 nm and 444 + 512 nm were lower than those for excitation combinations of 444 + 633 nm and 444 + 512 + 633 nm when cyanobacteria were dominant at depths of 0 and 2 m at Station 9B (South Basin) in August (Fig 2B and 2C). On the other hand, there were no clear differences in Fo profiles at Station 12B (North Basin) on 13th September and Station 6B (South Basin) on 18th September when diatoms and zygnematophytes dominated (Fig 2E, 2F, 2H and 2I). Further, the relationship between JVf and PAR intensity showed the utility of 633 nm for revealing signatures of cyanobacterial photosynthesis (Fig 3). For example, JVf was clearly lower than JVO using excitation at 444 nm and 444 + 512 nm, but not at 444 + 633 nm and the combination of all three wavelengths at Station 9B on 28th August during a cyanobacterial bloom (Fig 3A). No clear differences in JVf were observed between the combinations of wavelengths at Station 12B on 13th September and Station 6B on 18th September 2018 (Fig 3B and 3C).
Panels showing PAR, water temperature, Chl-a (A, D, G), Fo (B, E, H) estimated by different combinations of excitation wavelength from the FRRf, and phytoplankton biomass (C, F, I) at Station 9B on 28th August (A, B, C), Station 12B on 13th September (D, E, F) and Station 6B on 18th September 2018 (G, H, I). Grey dashed lines denote 0 m.
JVf was estimated by different combinations of excitation wavelength from the FRRf relative to ambient PAR intensity at (A) Station 9B on 28th August, (B) Station 12B on 13th September and (C) Station 6B on 18th September. The JVO estimates from the light-dark bottle method are also shown. For JVO, PAR intensity was calculated by the light intensity of growth chambers and SCF (see Materials and methods). The fitted curve is given for JVO using a two-parameter model  to improve visibility.
The data quality of FRRf measurements during the study period showed reasonable stability (Table 4). Upon rejection of low-quality data (e.g. with RσPSII or RσPSII′ < 0.03 or > 0.08), the number of successful observations was found to be highest when PSII was excited with a combination of three wavelengths, followed by excitation light at 444 + 633 nm, 444 + 512 nm, and 444 nm. Median values of both RσPSII and RσPSII′ were also near the optimal value (0.05) when the three wavelengths were combined.
Development of Фe,C model
Environmental and biological conditions.
Ancillary measurements of water temperature, DO concentration, turbidity, Chl-a, NO2 + NO3, NH4 and PO4 concentrations from each sampling showed clear spatial and seasonal variability (Table 5). Water temperature varied from 7.5 to 30.2°C in the North Basin and 7.5 to 28.5°C in the South Basin throughout the study period (Table 5). NO2 + NO3 and NH4 concentrations were lower in summer and autumn, and higher in winter at both basins throughout the study period. PO4 did not show clear seasonal changes and was always lower than 0.04 μmol L−1 in both basins throughout the study period.
At all sampling dates, diatoms, zygnematophytes, cyanobacteria and cryptophytes were the dominant groups in the phytoplankton biomass (S6 Appendix). Zygnematophytes, mainly composed of Staurastrum dorsidentiferum, S. sebaldi and Micrasterias hardyi, were always found at all stations throughout the study period, except at Station 6B in December. Diatoms were dominant during summer to early autumn and reached 87% in the phytoplankton biomass at Station 6B in September (S6 Appendix). Cryptophytes were present at a relatively low proportion through the study period, except at Station 6B in December. Cyanobacteria were mainly composed of Anabaena (Dolichospermum) affinis and Aphanothece sp. and bloomed at Station 9B on 28th August. Small chlorophytes, crysophytes and dinoflagellates always made up less than 20% of the total phytoplankton biomass. Euglenophytes were very rare and accounted for less than 0.5%of the total biomass throughout the study period.
Spatiotemporal variation and GLM development for Фe,C.
To develop an optimal electron requirement for the carbon fixation (Фe,C) model, we used the data set that was obtained by the combination of three excitation wavelengths due to the quality and reliability (Figs 2 and 3). After bootstrap sampling, boxplots of median Фe,C were calculated for each sampling date (Fig 4). Фe,C changed temporally from 1.1 to 31.0 mol e− mol C−1 and was higher in spring and summer in both the North and South basins. The mean annual Фe,C values were 5.6 mol e− mol C−1 for the North Basin, 9.0 mol e− mol C−1 for the South Basin and 7.3 mol e− mol C−1 for all sampling stations.
Spatial and temporal variability of Фe,C of the phytoplankton community in the North Basin (A) and the South Basin (B) throughout the study period. The box plot shows the median (bold line), and 25th (Q1) and 75th (Q3) percentiles. The whiskers indicate 1.5 times the interquartile range (Q3−Q1) below and above Q1 and Q3. Outliers beyond the whiskers were plotted individually. Note: Фe,C values were derived from the data measured by the combination of three excitation wavelengths.
To select and define the explanatory variables for GLM, we examined correlations between Фe,C and all candidate environmental factors (Fig 5). Small chlorophytes, crysophytes and dinoflagellates were excluded because of their low proportions relative to the total phytoplankton biomass. Фe,C correlated positively with PAR, temperature, DO, NPQNSV, Chl-a, and σPSII, and negatively with maximum photochemical efficiency under dark conditions (Fv/Fm) throughout the study period. NPQNSV highly correlated with PAR and Fv/Fm (ρ = 0.70 and −0.96, respectively). RCII concentration highly correlated with Chl-a (ρ = 0.70), and diatoms and zygnematophytes also negatively correlated (ρ = −0.70) with each other. Based on the correlation matrix, we selected temperature, PAR, turbidity, DO, Fv/Fm, σPSII, NH4, NO2 + NO3, PO4, Chl-a, and fractions of diatoms, cyanobacteria, and cryptophytes in the phytoplankton biomass as explanatory variables for the GLM. The explanatory variable ‘PAR’ may include influences of both PAR and NPQNSV in the GLM due to the high correlation between the two. Similarly, the explanatory variable ‘diatoms’ in this analysis may include influences of both diatoms and zygnematophytes.
Coloured panels denote statistical significance (p < 0.05). Abbreviations of variables are as follows: Temp, water temperature; NTU, turbidity; Chl, Chl-a concentration; Diat, diatom; Cyano, cyanobacteria; Zyg, zygnematophytes; Cryp, cryptophytes.
Among all possible models, the best model with the lowest AIC was the full model without PAR (Table 6). All variables in the best model exhibited VIF < 10 and thus collinearity was negligible. The R2 for the best model was 0.67. Among the explanatory variables, temperature showed the highest significance in the best model (coefficient of 0.51), followed by cyanobacteria (coefficient of −0.20) and σPSII (coefficient of 0.17). The performances of more parsimonious models were examined to evaluate the laborious sampling effort of nutrients and microscopy analysis of phytoplankton assemblages. The lowest AIC models without nutrients (Model 2), and without nutrients and phytoplankton assemblages (Model 3) were employed. Model 2 included six variables (temperature, Fv/Fm, σPSII, cyanobacteria, diatoms and cryptophytes), while Model 3 included three variables (temperature, Fv/Fm and σPSII). The values for R2 for Model 2 and Model 3 were 0.61 and 0.42, respectively. The results of the other sub-models with and without standardisation of variables are listed in the (S2 and S3 Tables).
Recently, studies using FRRf with only one wavelength, around 450 nm, for primary production measurements have been successful [25, 26]. However, the absorption spectrum of phytoplankton is highly dependent on the construction of antenna pigments, and is quite different between cyanobacteria and the other phytoplankton groups . It is well known that the optimal excitation waveband of cyanobacteria is between 550 and 650 nm, while that of eukaryotic algae is between 400 and 550 nm [104, 105]. Therefore, the blue excitation flash at 444 nm can fail to saturate the RCII in cyanobacteria during a single turnover measurement of FRRf [41, 106], and thus underestimate Fo  and GPP  due to mismatch in wavelength between excitation wavelengths of the FRRf and the absorption spectrum of cyanobacteria. Indeed, the present study demonstrated that JVf measured with an excitation light of 444 nm (single source) or with excitation lights of 444 + 512 nm was considerably underestimated compared with that in measurements utilising 633 nm, particularly when cyanobacteria dominated (Fig 3). Although we estimated JVf by each combination of excitation wavelength with SCF, which was calculated from extrapolated a*phy, there might be large differences between modelled and actual a*phy around 633 nm, but not around 512 nm in the green part of the spectrum. This is because a*phy at 630 nm in August, when Anabaena spp. dominated, was estimated as 0.008−0.009 m−2 mg Chl-a−1 (S3 Appendix), while that of cultured Anabaena sp. was 0.028 m−2 mg Chl-a−1 . Further, a*phy of cyanobacteria can vary with taxonomic group  and nutrient availability [107, 108]. Our results suggest that, if the absorption spectrum cannot be measured in situ, the excitation light targeting phycobilin antenna pigments should be used to measure ETRPSII in communities where cyanobacteria dominate.
In this study, Фe,C in Lake Biwa ranged temporally from 1.1 to 31.0 mol e− mol C−1 (Fig 4). Although our Фe,C varied less than that reported in temperate ocean conditions (1.0 to 66.5 mol e− mol C−1 ), it was similar to those in an Atlantic Ocean transect (1.1 to 28.2 mol e− mol C−1 ) and Ariake Bay (1.2 to 26.6 mol e− mol C−1 ), and that in a shallow eutrophic lake (from 14.7 to 38.6 mol e− mol C−1 ). Considering that environmental conditions varied substantially among the sampling stations and seasons in this study, the range of our Фe,C reasonably represented variations in Lake Biwa, including its oligotrophic (North Basin) and mesotrophic (South Basin) areas.
It should be noted that, because we measured carbon fixation rates during the afternoon, there may have been diurnal variability of phytoplankton productivity. Previous studies reported that the carbon fixation rate of natural communities is ~1.3 times higher in the morning than in the afternoon because photoinhibition and nutrients depletion suppress community productivity in the afternoon [34, 109]. If we underestimated carbon fixation rates of the communities incubated in the growth chamber, the result might have overestimated Фe,C. However, Фe,C values were paradoxically smaller than theoretical values (4 mol e− mol C−1) during most of the observations (Fig 4), except on 28th August, 13th September, 10th and 25th October in 2018, and 19th April in 2019. Therefore, the influences of Фe,C overestimation may be minimal, and we may have actually underestimated Фe,C values throughout the study period. The smaller than theoretical Фe,C values can be due to underestimation of JVf, especially when cyanobacteria dominated [36, 104], and/or overestimation of carbon fixation rate due to bottle effects [26, 35, 43]. The former case is plausible because the GLM revealed that the effect of cyanobacteria on Фe,C was significantly negative (see below). The latter case is more likely in this study, due to mitigation of UV stresses in the growth chamber and an increasing growth rate of cells on bottle walls [110, 111]. It is also possible that the geometric properties of the incubation vessel can alter the light environment on each bottle, and cause calculation errors in ETRPSII and underestimation of Фe,C . In any case, although we applied relatively standard methods throughout the study, i.e., FRRf vs. bottle incubations with an isotopic tracer, the results showed Фe,C < 4, which may reflect core issues in this approach.
The Фe,C values < 4 have often been observed in laboratory cultures [43, 70], natural communities in open oceans [26, 40, 44], and coastal regions [25, 36, 39]. However, the analysis method for the low Фe,C values is not yet unified. Most of the studies included the low Фe,C values in the statistical analyses [36, 39, 40, 44, 70], while a few studies did not [25, 26]. In this study, we regarded all of the Фe,C values as apparent values as in the previous study  since the bottle incubation method can cause artifacts for all bottles. Thus, the low Фe,C values were included in the GLM analysis to clarify the apparent effect of environmental and biological factors on the variance of Фe,C.
The GLM determining Фe,C revealed that multiple physicochemical and biological factors, except PAR, were significant in Lake Biwa (Table 6). Previous studies primarily focused on the relationships between light environment, or NPQNSV and Фe,C [25, 27, 34, 38, 40, 65]. The NPQNSV is phenomenologically correlated with alternative electron flow (AEF) activity, which is activated by excess light and photodamage on PSII [1, 68, 112]. In the present study, PAR intensity was highly correlated with NPQNSV (Fig 5), and thus we incorporated PAR in GLM for Фe,C as a proxy of excess light and NPQNSV. Although PAR was not utilised in the development of the best model, water temperature, DO, Fv/Fm, σPSII, nutrient conditions and the compositions of the phytoplankton community were selected. Our results suggest that the light environment is not always the primary factor determining Фe,C; rather, water temperature plays a critical role in the electron requirement for carbon fixation.
Although the effects of temperature on Фe,C were not specifically addressed, the results from the present study can be used to discuss the mechanisms related to this relationship. First, increased temperature decreases the CO2 affinity of Rubisco through the acceleration of the O2 evolution rate and reduction of CO2 solubility [113, 114]. CO2 selectivity of Rubisco depends on its form : Form IA Rubisco (cyanobacteria) and form IB Rubisco (cyanobacteria and chlorophytes) have lower selectivity for CO2 than form ID Rubisco (diatoms). In Lake Biwa, cyanobacteria and zygnematophytes were dominant groups during summer and autumn (S6 Appendix). Thus, Rubisco CO2 affinity of the phytoplankton community in Lake Biwa might decrease following the increasing of water temperature and enhance Rubisco oxygenation (photorespiration). Second, to mitigate photorespiration, phytoplankton express CO2 concentration mechanisms (CCMs) . CCMs need ATP or NADPH, which are also needed for driving the Calvin–Benson cycle. Finally, increasing temperature may lead to a state of chronic photoinhibition through photodamage , as well as changes in species composition of the community . Thus, although we did not examine the interaction among all explanatory variables, temperature may have affected Фe,C vis-à-vis interaction with the other factors such as nutrient stoichiometry .
The relationships between multiple environmental factors other than light and Фe,C were reported in previous FRRf [35, 36, 40] and PAM studies [119, 120]. Lawrenz et al.  investigated the relationships between the Фe,C of marine phytoplankton and environmental conditions, and explored the best fitting models with 14 data sets from various geographical regions. They examined water temperature, salinity, optical depth, attenuation coefficient, Chl-a, NO3 and PO4 as explanatory variables, and showed that only water temperature, NO3 and PO4 significantly correlated with Фe,C in the data set. Their results support our best model, which included water temperature and nutrients. However, Lawrenz et al. also showed that the coefficients and significance of the identified parameters are quite dependent on the region of interest. Thus, future studies are necessary to examine the complex relationship among temperature, light and nutrient conditions in freshwater environments to delineate the specific conditions that explain Фe,C discrepancies.
Although three excitation wavelength combinations were used to evaluate the cyanobacterial photosynthesis correctly, the proportion of cyanobacteria in phytoplankton biomass was significant in determining the best Фe,C model (Table 6). The proportion of cyanobacteria within the community may cause differences in the light absorption characteristics between cyanobacteria and the other phytoplankton groups; cyanobacteria absorb only 25%–30% of light in PSII, while other phytoplankton absorb 48%–58% . Kromkamp et al. (2008) suggested that most of the Chl-a in cyanobacteria is associated with PSI rather than PSII, and detection-limited by fluorometry. Another explanation is underestimation of the RCII concentration under illuminated conditions (Eq 2). This can be caused by a decrease of FO under dark conditions due to changes in the fraction of excitation energy distribution between PSI and PSII (state transition) . The FRRf method primarily targets pigments associated with PSII; thus, the electron flow initiated by the excited PSI is difficult to evaluate. Johnsen et al.  suggested that the fraction of light absorption by PSII, or that of cellular Chl-a in PSII, can be a useful proxy as action spectra, or alternative to absorption spectra, to correct the effect of photoprotective carotenoids and PSI-PSII absorption variability. Considering the large differences in regulation of the distribution of light-harvesting pigments and excitation energy between cyanobacteria and eukaryotic algae, the action spectra proxies should provide more accurate measurement of GPP in future study. Further, evaluating the proportion of cyanobacteria in phytoplankton biomass will be crucial for correcting GPP estimation with ETRPSII in natural phytoplankton communities.
As expected, PO4 concentration negatively affected Фe,C (Table 6). This result was consistent with previous PO4 manipulation experiments conducted with marine phytoplankton . The effect of PO4 was, however, one of the lowest among all factors (Table 6). The low significance is likely due to the fact that the PO4 concentrations did not change drastically and were generally low (0.01–0.04 μmol L−1, Table 5) throughout the study period.
To verify the performance of the Фe,C models, we subsequently compared daily GPP estimated with FRRf (GPPf) and 13C (GPP13C) for the North and South basins on each sampling date. The RCII-specific primary production based on FRRf (PBf, mg C mmol RCII −1 h−1) was calculated from the Jf, and computed Фe,C with the best model, Model 2 and Model 3. The relationships between PBf and PAR were fitted in P-E curves with models [80, 95–97], as described in the materials and methods. Finally, daily GPPf and GPP13C were estimated as follows: (9) where RCIIZ is the RCII concentration at depth Z, L is the day length (h), and PBi(Z,t) is PBf or PB13C at depth Z and time t (h). The RCIIZ and PBi(Z,t) were calculated every 1.25 m for the North Basin and every 0.5 m for the South Basin based on average values of the observed data. Day length and daily PAR data were obtained from the Japan Meteorological Agency for the North Basin, and were measured by a PAR sensor (PAR-02D; Prede Co., Ltd., Tokyo, Japan) at Otsu for the South Basin.
The estimated GPP13C varied from 71 to 787 g C m−2 d−1, while GPPf with the best model, Model 2 and Model 3 varied from 86 to 630 g C m−2 d−1, 85 to 729 g C m−2 d−1 and 117 to 906 g C m−2 d−1, respectively (for date-specific values, see S4 Table). The GPPf using the best model relative to GPP13C varied from 0.48 to 1.46, suggesting that FRRf parameters with the best Фe,C model can reasonably reproduce GPP13C in Lake Biwa (Fig 6). Relative GPPf with Model 2 and Model 3, including fewer variables, also replicated GPP13C well, varying from 0.46 to 1.59 and 0.47 to 2.11, respectively. The comparative results suggest that, even if nutrients and phytoplankton biomass are not considered, GPP13C can be estimated using the FRRf parameters coupled with temperature for both oligotrophic and mesotrophic areas in Lake Biwa. This model parameterisation is significant for future applications in freshwater ecosystems where environmental conditions and phytoplankton communities can vary spatially and temporally.
In conclusion, the FRRf equipped with an excitation wavelength of 633 nm is effective in estimating ETRPSII for freshwater phytoplankton communities during cyanobacterial blooms. Contrary to our hypothesis, water temperature was the most important determinant factor, while phosphorus concentration was less effective in the Фe,C model in Lake Biwa. Further, GPP13C dynamics were effectively estimated from the ETRPSII using the best Фe,C model for both oligotrophic and mesotrophic areas in Lake Biwa. The parsimonious model, including only temperature and two photosynthetic parameters, also sufficiently reproduced GPP13C. These results must be interpreted with caution because although Фe,C should be mechanistically ≥ 4 mol e− mol C−1, our study showed Фe,C < 4 in 9 out of 14 observations. In this study, we define the observed Фe,C as apparent values that are included artifacts from methodological issues, such as bottle effects, which can be minimized by a relatively shorter incubation time (~2 h) . Moreover, studies are needed to develop the incubation-free techniques, such as cellular NADP(H) measurement . In this study, the phytoplankton community was verified through microscopy, but fluorometric characteristics from the FRRf may also allow researchers to determine phytoplankton assemblages at high in situ spatial and temporal resolution , and thus simplify the GPP measurements during cyanobacterial blooms. This study provides strong validation for measurements of primary productivity by FRRf in lakes with large spatiotemporal variabilities of phytoplankton assemblages and environmental conditions from oligo- to mesotrophic lake (or lacustrine) environments. Further, a recent study reported that net primary productivity can also be measured by FRRf when fluorescence induction and relaxation (FIRe) techniques are applied . This suggests that the application of FRRf enables real-time measurements of the PSII photochemical characteristics and the carbon metabolism of phytoplankton simultaneously. In the future, bio-optical measurements will allow researchers to disentangle the causality between anthropogenic nutrient control and fish catch [13, 61, 126], and between climate change and the production of higher trophic levels [7, 127].
S1 Table. Spectral correction factor (SFC) for JVf estimation on each sampling date.
S2 Table. All GLM sub-models with standardisation of variables.
S3 Table. All GLM sub-models without standardisation of variables.
S4 Table. GPP (g C m−2 d−1) estimated by 13C and FRRf with Фe,C models on each sampling date.
Spectral distribution of (A) excitation flash of FastOcean (B) light source of growth chamber.
S2 Appendix. Scatter plots of Jf in situ in the morning, and in the laboratory in the afternoon (at the start of the incubation experiments).
The combination of three excitation wavelengths was used. For Jf, PAR intensity was corrected by white background light intensity of the Act2 system and SCF (see Materials and methods). The fitted curve is given by a two-parameter model .
S3 Appendix. Modelled absorption spectra for various Chl-a concentrations.
Modelled absorption spectra of (A) pure water, (B) CDOM and (C) non-algal particles.
Spectral distribution of incident sunlight at 10:00 in (A) April to September, (B) October to February and (C) at 4 PM in July in 2015. Each spectrum distribution was referenced to calculate the spectral correction on each sampling date as in Eq (7).
We would like to thank Dr. Takamaru Nagata in LBERI and Dr. Hiroki Haga in Lake Biwa Museum for sharing their ship time and valuable support during sampling. We sincerely thank Dr. Satoshi Nakada and Maho Iwaki for providing PAR profile data, and Hirokazu Teraishi for assisting with the chemical analysis. The authors would like to thank Enago (www.enago.jp) for the English language review.
- 1. Falkowski PG, Raven JA. Aquatic photosynthesis, 2nd edition. New Jersey: Princeton University Press; 2007. Available: http://site.ebrary.com/id/10789806
- 2. Oksanen L, Fretwell SD, Arruda J, Niemela P. Exploitation ecosystems in gradients of primary productivity. Am Nat. 1981;118: 240–261.
- 3. Power M. Top‐Down and Bottom‐Up Forces in Food Webs: Do Plants Have Primacy. Ecology. 1992;73: 733–746.
- 4. Falkowski PG, Barber RT, Smetacek V. Biogeochemical controls and feedbacks on ocean primary production. Science. 1998;281: 200.
- 5. Field CB. Primary Production of the Biosphere: Integrating Terrestrial and Oceanic Components. Science. 1998;281: 237–240.
- 6. Pauly D, Christensen V. Primary production required to sustain global fisheries. Nature. 1995;374: 255. https://doi.org/10.1038/374255a0
- 7. Chassot E, Bonhommeau S, Dulvy NK, Mélin F, Watson R, Gascuel D, et al. Global marine primary production constrains fisheries catches. Ecol Lett. 2010;13: 495–505.
- 8. Hatton IA, McCann KS, Fryxell JM, Davies TJ, Smerlak M, Sinclair ARE, et al. The predator-prey power law: Biomass scaling across terrestrial and aquatic biomes. Science. 2015;349.
- 9. Schindler DW. Factors regulating phytoplankton production and standing crop in the world’s freshwaters: Freshwater phytoplankton production. Limnol Oceanogr. 1978;23: 478–486.
- 10. Carpenter SR, Kitchell JF, Hodgson JR, Cochran PA, Elser JJ, Elser MM, et al. Regulation of lake primary productivity by food web structure. Ecology. 1987;68: 1863–1876.
- 11. Elser JJ, Bracken MES, Cleland EE, Gruner DS, Stanley HW, Helmut H, et al. Global analysis of nitrogen and phosphorus limitation of primary producers in freshwater, marine and terrestrial ecosystems. Ecol Lett. 2007;10: 1135–1142.
- 12. Reynolds CS. The ecology of phytoplankton. Cambridge: Cambridge University Press; 2006.
- 13. Capuzzo E, Lynam CP, Barry J, Stephens D, Forster RM, Greenwood N, et al. A decline in primary production in the North Sea over 25 years, associated with reductions in zooplankton abundance and fish stock recruitment. Glob Change Biol. 2017 [cited 23 Nov 2017].
- 14. Nielsen ES. The use of radio-active carbon (C14) for measuring organic production in the sea. ICES J Mar Sci. 1952;18: 117–140.
- 15. Slawyk G, Collos Y, Auclair J-C. The use of the 13C and 15N isotopes for the simultaneous measurement of carbon and nitrogen turnover rates in marine phytoplankton. Limnol Oceanogr. 1977;22: 925–932.
- 16. Hama T, Miyazaki T, Ogawa Y, Iwakuma T, Takahashi M, Otsuki A, et al. Measurement of photosynthetic production of a marine phytoplankton population using a stable 13C isotope. Mar Biol. 1983;73: 31–36.
- 17. Strickland JHD, Parsons TR. A practical handbook of seawater analysis, 2nd edn. Bull Fish Res Board Can. 1972;167: 1–310.
- 18. Bender ML, Grande KD. Production, respiration, and the isotope geochemistry of O2 in the upper water column. Glob Biogeochem Cycles. 1987;1: 49–59.
- 19. Kolber Z, Falkowski PG. Use of active fluorescence to estimate phytoplankton photosynthesis in situ. Limnol Oceanogr. 1993;38: 1646–1665.
- 20. Kolber ZS, Prášil O, Falkowski PG. Measurements of variable chlorophyll fluorescence using fast repetition rate techniques: defining methodology and experimental protocols. Biochim Biophys Acta BBA—Bioenerg. 1998;1367: 88–106.
- 21. Suggett DJ, Kraay G, Holligan P, Davey M, Aiken J, Geider R. Assessment of photosynthesis in a spring cyanobacterial bloom by use of a fast repetition rate fluorometer. Limnol Oceanogr. 2001;46: 802–810.
- 22. Melrose DC, Oviatt CA, O’Reilly JE, Berman MS. Comparisons of fast repetition rate fluorescence estimated primary production and 14C uptake by phytoplankton. Mar Ecol Prog Ser. 2006;311: 37–46.
- 23. Corno G, Letelier RM, Abbott MR, David MK. Assessing primary production variability in the north pacific subtropical gyre: a comparison of fast repetition rate fluorometry and 14C measurements. J Phycol. 2006;42: 51–60.
- 24. Robinson C, Tilstone GH, Rees AP, Smyth TJ, Fishwick JR, Tarran GA, et al. Comparison of in vitro and in situ plankton production determinations. Aquat Microb Ecol. 2009;54: 13–34.
- 25. Zhu Y, Ishizaka J, Tripathy SC, Wang S, Mino Y, Matsuno T, et al. Variation of the photosynthetic electron transfer rate and electron requirement for daily net carbon fixation in Ariake Bay, Japan. J Oceanogr. 2016;72: 761–776.
- 26. Zhu Y, Ishizaka J, Tripathy S, Wang S, Sukigara C, Goes J, et al. Relationship between light, community composition and the electron requirement for carbon fixation in natural phytoplankton. Mar Ecol Prog Ser. 2017;580: 83–100.
- 27. Schuback N, Hoppe CJM, Tremblay J-É, Maldonado MT, Tortell PD. Primary productivity and the coupling of photosynthetic electron transport and carbon fixation in the Arctic Ocean. Limnol Oceanogr. 2017;62: 898–921.
- 28. Oxborough K, Moore CM, Suggett DJ, Lawson T, Hoi GC, Geider RJ. Direct estimation of functional PSII reaction center concentration and PSII electron flux on a volume basis: a new approach to the analysis of Fast Repetition Rate fluorometry (FRRf) data. Limnol Oceanogr Methods. 2012;10: 142–154.
- 29. Smyth TJ, Pemberton KL, Aiken J, Geider RJ. A methodology to determine primary production and phytoplankton photosynthetic parameters from Fast Repetition Rate Fluorometry. J Plankton Res. 2004;26: 1337–1350.
- 30. Tripathy SC, Ishizaka J, Fujiki T, Shibata T, Okamura K, Hosaka T, et al. Assessment of carbon- and fluorescence-based primary productivity in Ariake Bay, southwestern Japan. Estuar Coast Shelf Sci. 2010;87: 163–173.
- 31. Komatsu K, Imai A, Tomioka N, Takamura N, Nakagawa M, Satou T, et al. Method development for determining primary production rate by fast repetition rate fluorometry (FRRF). J Jpn Soc Civ Eng Ser G Environ Res. 2015;71: III_309–III_314.
- 32. Regaudie-de-Gioux A, Lasternas S, Agustí S, Duarte CM. Comparing marine primary production estimates through different methods and development of conversion equations. Front Mar Sci. 2014;1: 19.
- 33. Hughes D, Campbell D, Doblin MA, Kromkamp J, Lawrenz E, Moore CM, et al. Roadmaps and detours: active chlorophyll-a assessments of primary productivity across marine and freshwater systems. Environ Sci Technol. 2018.
- 34. 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.
- 35. Lawrenz E, Silsbe G, Capuzzo E, Ylöstalo P, Forster RM, Simis SGH, et al. Predicting the electron requirement for carbon fixation in seas and oceans. Stal LJ, editor. PLoS ONE. 2013;8: e58137. pmid:23516441
- 36. Robinson C, Suggett DJ, Cherukuru N, Ralph PJ, Doblin MA. Performance of fast repetition rate fluorometry based estimates of primary productivity in coastal waters. J Mar Syst. 2014;139: 299–310.
- 37. Silsbe GM, Smith REH, Twiss MR. Quantum efficiency of phytoplankton photochemistry measured continuously across gradients of nutrients and biomass in Lake Erie (Canada and USA) is strongly regulated by light but not by nutrient deficiency. Can J Fish Aquat Sci. 2015;72: 651–660.
- 38. Schuback N, Schallenberg C, Duckham C, Maldonado MT, Tortell PD. Interacting effects of light and iron availability on the coupling of photosynthetic electron transport and CO2-assimilation in marine phytoplankton. Cockshutt AM, editor. PLOS ONE. 2015;10: e0133235. pmid:26171963
- 39. Hughes DJ, Varkey D, Doblin MA, Ingleton T, Mcinnes A, Ralph PJ, et al. Impact of nitrogen availability upon the electron requirement for carbon fixation in Australian coastal phytoplankton communities. Limnol Oceanogr. 2018;63: 1891–1910.
- 40. Ryan-Keogh TJ, Thomalla SJ, Little H, Melanson J-R. Seasonal regulation of the coupling between photosynthetic electron transport and carbon fixation in the Southern Ocean. Limnol Oceanogr. 2018;63: 1856–1876.
- 41. Raateoja M, Seppälä J, Ylöstalo P. Fast repetition rate fluorometry is not applicable to studies of filamentous cyanobacteria from the Baltic Sea. Limnol Oceanogr. 2004;49: 1006–1012.
- 42. Suggett DJ, MacIntyre HL, Geider RJ. Evaluation of biophysical and optical determinations of light absorption by photosystem II in phytoplankton: Evaluation of light absorption by PSII. Limnol Oceanogr Methods. 2004;2: 316–332.
- 43. Suggett DJ, MacIntyre HL, Kana TM, Geider RJ. Comparing electron transport with gas exchange: parameterising exchange rates between alternative photosynthetic currencies for eukaryotic phytoplankton. Aquat Microb Ecol. 2009;56: 147–162.
- 44. Kulk G, van de Poll WH, Buma AGJ. Photophysiology of nitrate limited phytoplankton communities in Kongsfjorden, Spitsbergen: Photophysiology of Arctic phytoplankton. Limnol Oceanogr. 2018 [cited 30 Aug 2018].
- 45. Roach T, Krieger-Liszkay AK. Regulation of photosynthetic electron transport and photoinhibition. Curr Protein Pept Sci. 2014;15: 351–362. pmid:24678670
- 46. Oliver RL, Ganf GG. Freshwater Blooms. In: Whitton BA, Potts M, editors. The Ecology of Cyanobacteria: Their Diversity in Time and Space. Dordrecht: Springer; 2002. pp. 149–194. https://doi.org/10.1007/0-306-46855-7_6
- 47. Paerl HW, Scott JT, McCarthy MJ, Newell SE, Gardner WS, Havens KE, et al. It takes two to tango: when and where dual nutrient (N & P) reductions are needed to protect lakes and downstream ecosystems. Environ Sci Technol. 2016;50: 10805–10813.
- 48. Kaiblinger C, Dokulil MT. Application of fast repetition rate fluorometry to phytoplankton photosynthetic parameters in freshwaters. Photosynth Res. 2006;88: 19–30.
- 49. Wojtasiewicz B, Stoń-Egiert J. Bio-optical characterization of selected cyanobacteria strains present in marine and freshwater ecosystems. J Appl Phycol. 2016;28: 2299–2314. pmid:27471342
- 50. Subramaniam A, Carpenter EJ, Karentz D, Falkowski PG. Bio-optical properties of the marine diazotrophic cyanobacteria Trichodesmium spp. I. Absorption and photosynthetic action spectra. Limnol Oceanogr. 1999;44: 608–617.
- 51. Houliez E, Simis S, Nenonen S, Ylöstalo P, Seppälä J. Basin-scale spatio-temporal variability and control of phytoplankton photosynthesis in the Baltic Sea: The first multiwavelength fast repetition rate fluorescence study operated on a ship-of-opportunity. J Mar Syst. 2017;169: 40–51.
- 52. Conley DJ, Paerl HW, Howarth RW, Boesch DF, Seitzinger SP, Havens KE, et al. Ecology: controlling eutrophication: nitrogen and phosphorus. Science. 2009;323: 1014–1015. pmid:19229022
- 53. Karlsson J, Byström P, Ask J, Ask P, Persson L, Jansson M. Light limitation of nutrient-poor lake ecosystems. Nature. 2009;460: 506–509. pmid:19626113
- 54. Howarth RW. Nutrient limitation of net primary production in marine ecosystems. Annu Rev Ecol Syst. 1988;19: 89–110.
- 55. Howarth RW, Marino R. Nitrogen as the limiting nutrient for eutrophication in coastal marine ecosystems: Evolving views over three decades. Limnol Oceanogr. 2006;51: 364–376.
- 56. Sterner RW, Elser JJ. Ecological stoichiometry: the biology of elements from molecules to the biosphere. Princeton, New Jersey, USA: Princeton University Press; 2002.
- 57. Raven JA. RNA function and phosphorus use by photosynthetic organisms. Front Plant Sci. 2013;4. pmid:23355843
- 58. Pemberton KL, Smith RE, Silsbe GM, Howell T, Watson SB. Controls on phytoplankton physiology in Lake Ontario during the late summer: evidence from new fluorescence methods. Can J Fish Aquat Sci. 2007;64: 58–73.
- 59. Kaiblinger C, Greisberger S, Teubner K, Dokulil MT. Photosynthetic efficiency as a function of thermal stratification and phytoplankton size structure in an oligotrophic alpine lake. Hydrobiologia. 2007;578: 29–36.
- 60. Kromkamp JC, Dijkman NA, Peene J, Simis SGH, Gons HJ. Estimating phytoplankton primary production in Lake IJsselmeer (The Netherlands) using variable fluorescence (PAM-FRRF) and C-uptake techniques. Eur J Phycol. 2008;43: 327–344.
- 61. Kawanabe H, Nishino M, Maehata M, editors. Lake Biwa: interactions between nature and people. Dordrecht; New York; London: Springer; 2012.
- 62. Nishino M. Ecological Changes in Lake Biwa. In: Kawanabe H, Nishino M, Maehata M, editors. Lake Biwa: Interactions between Nature and People. Dordrecht: Springer; 2012. pp. 155–238. https://doi.org/10.1007/978-94-007-1783-1_3
- 63. Suzuki R, Ishimaru T. An improved method for the determination of phytoplankton chlorophyll using N, N-dimethylformamide. J Oceanogr Soc Jpn. 1990;46: 190–194.
- 64. Boatman TG, Geider RJ, Oxborough K. Improving the accuracy of single turnover active fluorometry (STAF) for the estimation of phytoplankton primary productivity (phytoPP). Front Mar Sci. 2019;6.
- 65. Wei Y, Zhao X, Sun J, Liu H. Fast repetition rate fluorometry (FRRF) derived phytoplankton primary productivity in the Bay of Bengal. Front Microbiol. 2019;10. pmid:31244786
- 66. Longstaff BJ, Kildea T, Runcie JW, Cheshire A, Dennison WC, Hurd C, et al. An in situ study of photosynthetic oxygen exchange and electron transport rate in the marine macroalga Ulva lactuca (Chlorophyta). Photosynth Res. 2002;74: 281–293. pmid:16245139
- 67. Cosgrove J, Moheimani NR, Borowitzka MA. Diurnal patterns in phytoplankton photosynthesis, Fremantle Harbour. J R Soc West Aust. 2015;98: 19–27.
- 68. Nawrocki WJ, Tourasse NJ, Taly A, Rappaport F, Wollman F-A. The plastid terminal oxidase: its elusive function points to multiple contributions to plastid physiology. Annu Rev Plant Biol. 2015;66: 49–74. pmid:25580838
- 69. McKew BA, Davey P, Finch SJ, Hopkins J, Lefebvre SC, Metodiev MV, et al. The trade-off between the light-harvesting and photoprotective functions of fucoxanthin-chlorophyll proteins dominates light acclimation in Emiliania huxleyi (clone CCMP 1516). New Phytol. 2013;200: 74–85. pmid:23790241
- 70. Hoppe CJM, Holtz L-M, Trimborn S, Rost B. Ocean acidification decreases the light-use efficiency in an Antarctic diatom under dynamic but not constant light. New Phytol. 2015;207: 159–171. pmid:25708812
- 71. Kitajima M, Butler WL. Quenching of chlorophyll fluorescence and primary photochemistry in chloroplasts by dibromothymoquinone. Biochim Biophys Acta. 1975;376: 105–115. pmid:1125215
- 72. Kirilovsky D. Modulating energy arriving at photochemical reaction centers: orange carotenoid protein-related photoprotection and state transitions. Photosynth Res. 2015;126: 3–17. pmid:25139327
- 73. Aspinwall CL, Sarcina M, Mullineaux CW. Phycobilisome mobility in the Cyanobacterium Synechococcus sp. PCC7942 is influenced by the trimerisation of photosystem I. Photosynth Res. 2004;79: 179. pmid:16228392
- 74. Joshua S, Mullineaux CW. Phycobilisome diffusion is required for light-state transitions in cyanobacteria. Plant Physiol. 2004;135: 2112–2119. pmid:15286286
- 75. Campbell D, Hurry V, Clarke AK, Gustafsson P, Öquist G. Chlorophyll fluorescence analysis of cyanobacterial photosynthesis and acclimation. Microbiol Mol Biol Rev. 1998;62: 667–683. pmid:9729605
- 76. Wetzel RG, Likens GE. Limnological analyses. New York, NY: Springer; 2010. Available: http://dx.doi.org/10.1007/978-1-4757-3250-4
- 77. Luz B, Barkan E, Sagi Y, Yacobi YZ. Evaluation of community respiratory mechanisms with oxygen isotopes: A case study in Lake Kinneret. Limnol Oceanogr. 2002;47: 33–42.
- 78. Pringault O, Tassas V, Rochelle-Newall E. Consequences of respiration in the light on the determination of production in pelagic systems. Biogeosciences. 2007;4: 105–114.
- 79. Sorokin YI. The Radiocarbon Method to Estimate Primary Production in Aquatic Environments. In: Sorokin YI, editor. Radioisotopic Methods in Hydrobiology. Berlin, Heidelberg: Springer; 1999. pp. 21–99. https://doi.org/10.1007/978-3-642-59934-7_2
- 80. Webb WL, Newton M, Starr D. Carbon dioxide exchange of Alnus rubra. Oecologia. 1974;17: 281–291. pmid:28308943
- 81. Hillebrand H, Dürselen C-D, Kirschtel D, Pollingher U, Zohary T. Biovolume calculation for pelagic and benthic microalgae. J Phycol. 1999;35: 403–424.
- 82. Menden-Deuer S, Lessard EJ. Carbon to volume relationships for dinoflagellates, diatoms and other protist plankton. Limnol Oceanogr. 2000;45: 569–579.
- 83. Miyajima T, Yamada Y, Wada E, Nakajima T, Koitabashi T, Hanba YT, et al. Distribution of greenhouse gases, nitrite, and δ13C of dissolved inorganic carbon in Lake Biwa: Implications for hypolimnetic metabolism. Biogeochemistry. 1997;36: 205–221.
- 84. Belzile C, Vincent WF, Howard‐Williams C, Hawes I, James MR, Kumagai M, et al. Relationships between spectral optical properties and optically active substances in a clear oligotrophic lake. Water Resour Res. 2004;40.
- 85. Kirk JTO. Light and photosynthesis in aquatic ecosystems. 3rd ed. Cambridge, UK; New York: Cambridge University Press; 2011.
- 86. Paavel B, Kangro K, Arst H, Reinart A, Kutser T, Nõges T. Parameterization of chlorophyll-specific phytoplankton absorption coefficients for productive lake waters. J Limnol. 2016;75.
- 87. Ylöstalo P, Kallio K, Seppälä J. Absorption properties of in-water constituents and their variation among various lake types in the boreal region. Remote Sens Environ. 2014;148: 190–205.
- 88. Hirose H, Kumano S, Madono K. Spectroscopic studies on phycoerythrins from cyanophycean and rhodophycean algae with special reference to their phylogenetical relations. Bot Mag Tokyo. 1969 [cited 1 Oct 2020]. Available: https://agris.fao.org/agris-search/search.do?recordID=US201301211892
- 89. Rohatgi A, Singh SP. Isolation and characterization of pigment mutants of the blue-green alga Aphanothece stagnina. Mol Gen Genet MGG. 1979;169: 59–62.
- 90. Wyman M, Fay P, Fogg GE. Underwater light climate and the growth and pigmentation of planktonic blue-green algae (Cyanobacteria) I. The influence of light quantity. Proc R Soc Lond B Biol Sci. 1986;227: 367–380.
- 91. Pope RM, Fry ES. Absorption spectrum (380–700 nm) of pure water. II. Integrating cavity measurements. Appl Opt. 1997;36: 8710–8723. pmid:18264420
- 92. Belzile C, Vincent WF, Kumagai M. Contribution of absorption and scattering to the attenuation of UV and photosynthetically available radiation in Lake Biwa. Limnol Oceanogr. 2002;47: 95–107.
- 93. Terrel MM, Fukushima T, Matsushita B, Yoshimura K, Imai A. Long-term light environment variability in Lake Biwa and Lake Kasumigaura, Japan: modeling approach. Limnology. 2012;13: 237–252.
- 94. New Energy and Industrial Technology Development Organization (NEDO). Solar radiation spectrum database. 2016. Available: http://app0_2.infoc.nedo.go.jp/
- 95. Peeters JCH, Eilers P. The relationship between light intensity and photosynthesis—A simple mathematical model. Hydrobiol Bull. 1978;12: 134–136.
- 96. Aiba S. Growth kinetics of photosynthetic microorganisms. Microbial Reactions. 1982. pp. 85–156.
- 97. Megard RO, Tonkyn DW, Senft WH II. Kinetics of oxygenic photosynthesis in planktonic algae. J Plankton Res. 1984;6: 325–337.
- 98. R Development Core Team. R: A Language and environment for statistical computing. Vienna, Austria; 2020. Available: http//www.R-project.org/
- 99. O’brien RM. A caution regarding rules of thumb for variance inflation factors. Qual Quant. 2007;41: 673–690.
- 100. Fox J, Weisberg S, Price B, Adler D, Bates D, Baud-Bovy G, et al. car: Companion to Applied Regression. 2019. Available: https://CRAN.R-project.org/package=car
- 101. Barton K. MuMIn: multi-model inference v1.15.1. 2015. Available: https://cran.r-project.org/web/packages/MuMIn/index.html
- 102. Akaike H. Information theory and an extension of the maximum likelihood principle. 2nd Int Symp Inf Theory. 1973; 267–281.
- 103. Johnsen G, Sakshaug E. Biooptical characteristics of PSII and PSI in 33 species (13 pigment groups) of marine phytoplankton, and the relevance for pulse-amplitude-modulated and fast-repetition-rate fluorometry. J Phycol. 2007;43: 1236–1251.
- 104. Simis SGH, Huot Y, Babin M, Seppälä J, Metsamaa L. Optimization of variable fluorescence measurements of phytoplankton communities with cyanobacteria. Photosynth Res. 2012;112: 13–30. pmid:22403036
- 105. Schubert H, Schiewer U, Tschirner E. Fluorescence characteristics of cyanobacteria (blue-green algae). J Plankton Res. 1989;11: 353–359.
- 106. Suggett DJ, Moore CM, Hickman AE, Geider RJ. Interpretation of fast repetition rate (FRR) fluorescence: signatures of phytoplankton community structure versus physiological state. Mar Ecol Prog Ser. 2009;376: 1–19.
- 107. Bricaud A, Babin M, Morel A, Claustre H. Variability in the chlorophyll-specific absorption coefficients of natural phytoplankton: Analysis and parameterization. J Geophys Res Oceans. 1995;100: 13321–13332.
- 108. Stæhr PA, Markager S. Parameterization of the chlorophyll a-specific in vivo light absorption coefficient covering estuarine, coastal and oceanic waters. Int J Remote Sens. 2004;25: 5117–5130.
- 109. Zhao Y, Quigg A. Study of photosynthetic productivity in the Northern Gulf of Mexico: Importance of diel cycles and light penetration. Cont Shelf Res. 2015;102: 33–46.
- 110. Carpenter EJ, Lively JS. Review of Estimates of Algal Growth Using 14C Tracer Techniques. In: Falkowski PG, editor. Primary Productivity in the Sea. Boston, MA: Springer US; 1980. pp. 161–178. https://doi.org/10.1007/978-1-4684-3890-1_9
- 111. Venrick EL, Beers JR, Heinbokel JF. Possible consequences of containing microplankton for physiological rate measurements. J Exp Mar Biol Ecol. 1977;26: 55–76.
- 112. Saroussi SI, Wittkopp TM, Grossman AR. The type II NADPH dehydrogenase facilitates cyclic electron flow, energy-dependent quenching, and chlororespiratory metabolism during acclimation of Chlamydomonas reinhardtii to nitrogen deprivation. Plant Physiol. 2016;170: 1975. pmid:26858365
- 113. Ogren WL. Photorespiration:pathways, regulation, and modification. Annu Physiol. 1984;35: 415–442.
- 114. Hagemann M, Weber AP, Eisenhut M. Photorespiration: origins and metabolic integration in interacting compartments. J Exp Bot. 2016;67: 2915–2918.
- 115. Iñiguez C, Capó‐Bauçà S, Niinemets Ü, Stoll H, Aguiló‐Nicolau P, Galmés J. Evolutionary trends in RuBisCO kinetics and their co-evolution with CO2 concentrating mechanisms. Plant J. 2020;101: 897–918. pmid:31820505
- 116. Giordano M, Beardall J, Raven JA. CO 2 concentrating mechanisms in algae: mechanisms, environmental modulation, and evolution. Annu Rev Plant Biol. 2005;56: 99–131. pmid:15862091
- 117. Yellowlees D, Warner M. Photosynthesis in Symbiotic Algae. In: Larkum AWD, Douglas SE, Raven JA, editors. Photosynthesis in Algae. Dordrecht: Springer Netherlands; 2003. pp. 437–455. https://doi.org/10.1007/978-94-007-1038-2_19
- 118. Fernández‐González C, Pérez‐Lorenzo M, Pratt N, Moore CM, Bibby TS, Marañón E. Effects of temperature and nutrient supply on resource allocation, photosynthetic strategy, and metabolic rates of Synechococcus sp. J Phycol. 2020;56: 818–829. pmid:32130730
- 119. Napoléon C, Claquin P. Multi-parametric relationships between PAM measurements and carbon incorporation, an in situ approach. PLOS ONE. 2012;7: e40284. pmid:22911698
- 120. Morelle J, Schapira M, Orvain F, Riou P, Lopez PJ, Pierre-Duplessix O, et al. Annual phytoplankton primary production estimation in a temperate estuary by coupling pam and carbon incorporation methods. Estuaries Coasts. 2018;41: 1337–1355.
- 121. Napoléon C, Raimbault V, Claquin P. Influence of nutrient stress on the relationships between PAM measurements and carbon incorporation in four phytoplankton species. PLOS ONE. 2013;8: e66423. pmid:23805221
- 122. Milligan AJ, Halsey KH, Behrenfeld MJ. Advancing interpretations of 14C-uptake measurements in the context of phytoplankton physiology and ecology. J Plankton Res. 2015;37: 692–698.
- 123. Jones BM, Halsey KH, Behrenfeld MJ. Novel incubation-free approaches to determine phytoplankton net primary productivity, growth, and biomass based on flow cytometry and quantification of ATP and NAD(H). Limnol Oceanogr Methods. 2017;15: 928–938.
- 124. Rolland A, Rimet F, Jacquet S. A 2-year survey of phytoplankton in the Marne Reservoir (France): A case study to validate the use of an in situ spectrofluorometer by comparison with algal taxonomy and chlorophyll a measurements. Knowl Manag Aquat Ecosyst. 2010; 02.
- 125. Gorbunov MY, Falkowski PG. Using chlorophyll fluorescence kinetics to determine photosynthesis in aquatic ecosystems. Limnol Oceanogr. n/a.
- 126. Yanagi T. Oligotrophication in the Seto Inland Sea. In: Yanagi T, editor. Eutrophication and Oligotrophication in Japanese Estuaries: The present status and future tasks. Dordrecht: Springer; 2015. pp. 39–67. https://doi.org/10.1007/978-94-017-9915-7_3
- 127. Ware DM, Thomson RE. Bottom-up ecosystem trophic dynamics determine fish production in the Northeast Pacific. Science. 2005;308: 1280–1284. pmid:15845876