Search tips
Search criteria 


Logo of scirepAboutEditorial BoardFor AuthorsScientific Reports
Sci Rep. 2017; 7: 6868.
Published online 2017 July 31. doi:  10.1038/s41598-017-07195-8
PMCID: PMC5537254

Effects of elevated CO2 on phytoplankton during a mesocosm experiment in the southern eutrophicated coastal water of China


There is a growing consensus that the ongoing increase in atmospheric CO2 level will lead to a variety of effects on marine phytoplankton and ecosystems. However, the effects of CO2 enrichment on eutrophic coastal waters are still unclear, as are the complex mechanisms coupled to the development of eutrophication. Here, we report the first mesocosm CO2 perturbation study in a eutrophic subtropical bay during summer by investigating the effect of rising CO2 on a model artificial community consisting of well-characterized cultured diatoms (Phaeodactylum tricornutum and Thalassiosira weissflogii) and prymnesiophytes (Emiliania huxleyi and Gephyrocapsa oceanica). These species were inoculated into triplicate 4 m3 enclosures with equivalent chlorophyll a (Chl-a) under present and higher partial pressures of atmospheric CO2 (pCO2 = 400 and 1000 ppmv). Diatom bloom events were observed in all enclosures, with enhanced organic carbon production and Chl-a concentrations under high CO2 treatments. Relative to the low CO2 treatments, the consumption of the dissolved inorganic nitrogen and uptake ratios of N/P and N/Si increased significantly during the bloom. These observed responses suggest more extensive and complex effects of higher CO2 concentrations on phytoplankton communities in coastal eutrophic environments.


At present, one of the most far-reaching global perturbations of the marine environment is caused by the massive invasion of fossil fuel CO2 into the ocean, making it the second largest sink for anthropogenic carbon dioxide after the atmosphere itself1. CO2 dissolved in seawater forms free H+ ions, lowering ocean pH and shifting dissolved inorganic carbon away from carbonate (CO3 2−) towards more bicarbonate (HCO3 ) and CO2. This global effect of anthropogenic CO2 emissions on ocean carbonate chemistry is of concern because it is already lowering the pH of the oceans, which may have ramifications for the growth, productivity and dominance of individual organisms or whole marine ecosystems2.

It has been suggested that the consequences of global ocean acidification will become more acute in the coastal zone, due to the decomposition of organic matter produced in eutrophic waters3. Coastal areas are complex and dynamic places in which environmental factors typically exhibit great spatial and temporal variability. For example, CO2 partial pressures (pCO2) in the inner estuary of the highly eutrophic Pearl River was found to range from 3380 to 4785 µatm in the summer, with a pH of 7.0–7.24. Meanwhile, in a concurrent bloom in the outer estuary of the Pearl River pCO2 dropped rapidly to ~200 µatm, and pH rose to as high as 8.65. This is mainly due to a variety of biogeochemical processes in coastal water, not from changes of CO2 in atmospheric concentrations. Terrigenous inputs, upwelling effects and biological activities (algal blooms, bacterial respiration) play important roles on the variations of pCO2 and pH in the water. The coastal acidification has been predicted to be over 10% faster compared to pelagic waters, as the decomposition of organic carbon by bacteria leads to an extra increase in CO2 concentration, usually associated with the processes of phytoplankton blooms and hypoxia in estuaries during summer3. Thus, although the partial pressure of CO2 in some stages of eutrophication is lower than the anthropogenically-influenced atmospheric pCO2, eutrophic coastal waters will still be under the influence of high pCO2 in the future3.

Efforts to understand potential consequences and feedbacks of increasing CO2 have been employed using both laboratory and mesocosm studies over scales ranging from genetic to ecosystem levels6, 7. Among the laboratory tests to investigate biological responses to ocean acidification, diazotrophic cyanobacteria, diatoms and prymnesiophytes (coccolithophores) are the most studied groups8, 9. In eutrophic coastal waters, diatoms and prymnesiophytes are dominant groups8, and responsible for a large fraction of oceanic primary production, playing an important role in marine ecosystems. Some typical species, such as Phaeodactylum tricornutum and Emiliania huxleyi, have been intensively studied with respect to their modes of C acquisition and various responses to changes in seawater CO2 at physiological, biochemical and molecular levels2, 10. However, since a majority of laboratory studies have investigated responses of single species, the knowledge obtained is difficult to extrapolate to these species’ responses to ocean acidification in natural complex environments. On the other hand, there are too many species in natural communities, including phytoplankton, zooplankton, and bacteria. In addition, natural communities in coastal waters have to confront to the complex influences of both natural change and human activities2. Therefore, we presently know little about how these organism responses scale up to the community and ecosystem levels and what the consequences are for marine food webs and biogeochemical cycles6, 7, 11. One way to bridge this gap between single species studies and highly complex natural communities is to test the mechanistic effects of global change factors on relatively less complex artificial communities composed of a few key phytoplankton groups12.

Mesocosm approaches are useful to shorten this gap between laboratory tests and in-situ investigations, and mixtures of well-studied phytoplankton species should be studied at mesocosm level to evaluate competition and succession under elevated CO2. Laboratory cultures are normally kept under stable conditions (e.g. constant light, temperature), while mesocosm enclosures are exposed to varying or fluctuating environmental factors, such as solar radiation and diel changes of temperature. Therefore, mesocosm enclosures are designed to approximate natural conditions in which environmental factors can be manipulated and closely monitored, and so provide a powerful tool to understand and forecast the effects of environmental changes on pelagic communities and the associated impacts on biogeochemical cycling6. In spite of this, recent findings show that there are still many unanswered questions using these approaches7. For example in mesocosm enclosures in the southern Norway, the inferred cumulative C:N stoichiometry of organic production increased with CO2 treatments at initial CO2 partial pressures of 350, 700 and 1,050 ppmv from 6.3 to 7.1 to 8.3 at the height of the bloom, respectively9. This suggests that ocean acidification may modify the stoichiometry of pelagic primary production which consumed up to 39% more dissolved inorganic carbon at increased pCO2 compared to the ambient level, whereas nutrient drawdown remained similar1, 9. However, considerable uncertainty about this finding was shown in other mesocosm tests (Table S1). During a CO2 perturbation study in Kongsfjorden on the west coast of Spitsbergen (Norway), carbon to nutrient uptake ratios were lower or higher than Redfield proportions during different phases of the experiment13. Another mesocosm study in the coastal waters of Korea also found the stoichiometry of elemental assimilation was insensitive to increasing pCO2 concentration and was close to the Redfield ratio of ~6.614, 15. In addition, effects of ocean acidification on phytoplankton uptake stoichiometry in coastal waters may result in a series of complicated changes in biogeochemical cycles10, such as altering the potential for phytoplankton growth limitation by nutrient elements such as P or Si over different spatial and temporal scales. Therefore, in highly productive coastal ecosystems, which support fisheries and other ecosystem services, unpredictable effects of ocean acidification ought to be intensively studied, since the biogeochemical response to increasing CO2 is obviously more complex than has been suggested from previous studies7, 10, 13, 16.

Under eutrophic conditions, nutrient limitation of phytoplankton growth could be alleviated and CO2 might be a limiting factor, especially during algal blooms. Subsequently, it is reasonable to hypothesize that growth of phytoplankton in eutrophic waters could be enhanced under elevated CO2 levels. In this study, we conducted a mesocosm CO2 perturbation study in a eutrophic subtropical bay in China during early summer, to investigate the effect of rising CO2 on a model phytoplankton community consisting of four well-studied phytoplankton isolates. These results are then used to discuss the following questions: i) What is the effect of high CO2 partial pressure on the growth of phytoplankton in eutrophic coastal waters? ii) How does elevated CO2 affect the competition between diatoms and prymnesiophytes (coccolithophores), the two most studied taxonomic groups in response to ocean acidification? and iii) Will the effects of high pCO2 on phytoplankton uptake stoichiometry in coastal waters alter the potential for limitation by nutrients such as N, P, or Si?


Temporal evolution of the carbon dioxide system

The vertical variations on temperature and salinity in the enclosures were less than 0.1 °C and 0.1, respectively, indicating that the water was well mixed (Fig. S2). During the 15 days, there was a clear increase in temperature (mean value increase 2 °C) but only a slight increase in salinity (mean value increase 0.1). The initial dissolved inorganic carbon (DIC), total alkalinity (TA) and pH in the water were 2036 ± 9 (mean ± SD, the same below), 1907 ± 8 µmol kg−1 and 7.75 ± 0.01, respectively (Fig. 1). Consequently, the initial pCO2 in the water was 805 ± 22 µatm (Fig. 2a), indicating it was in fact already influenced by acidification, with a low pH and quite high DIC (Fig. 1). As expected, the initial concentrations of dissolved organic carbon (DOC) were quite high (day 1, 227 ± 15 µM).

Figure 1
Temporal variations of concentrations of dissolved inorganic carbon (DIC, panel a), total alkalinity (TA, b) and pH (c) in 6 enclosures perturbed by bubbling with ambient air (400 ppmv CO2, Low CO2 level) or an air/CO2 mixture at a concentration ...
Figure 2
Temporal variations of the CO2 partial pressure in the seawater (pCO2, μatm, panel a) in 6 enclosures perturbed by bubbling with ambient air (400 ppmv CO2, Low CO2 level) or an air/CO2 mixture at a concentration of 1000 ppmv CO ...

Gradually with aeration from the CO2 enrichlors (400 and 1000 ppmv, HC and LC), there were significant differences between high and low CO2 treatments in pH, DIC and pCO2 in the water in the first 4 days (Fig. 2b, all p < 0.05). The mean pCO2 levels in the HC and LC treatments were 879.15 ± 145.76 and 658.05 ± 113.98 ppmv, with a significant differences of 221.10 ppmv in the first 4 days (Fig. 2b).

Along with the growth of phytoplankton and consequent depletion of nutrients, pH value increased in all enclosures (Fig. 1c). The pCO2 values dropped rapidly to ~200 µatm, and pH rose to over 8.5, indicating the impact of biological activity was first order. During the growth of phytoplankton, they were aerated continuously by different CO2 enrichments. Although lower pH values and higher pCO2 in the early phase were observed, quite high pH values (8.90 ± 0.06) and low pCO2 (31 ± 2 µatm) in the HC enclosures were observed on day 10 (Fig. 1).

Temporal evolution of nutrients

The initial filtered bay water used for the experiment was highly eutrophic, with nutrient concentrations in the initial waters of 30.48 ± 0.29, 53.32 ± 1.10 3.42 ± 0.05 and 45.92 ± 0.39 µM for NO3  + NO2 (NOx), NH4 +, PO4 3− and SiO3 2−, respectively (Figs 3 and and4).4). The composition of the dissolved inorganic nitrogen pool (DIN, NOx + NH4 +) indicates a very high proportion of NH4 + (Fig. 3). DIN concentrations dropped sharply after day 3 due to phytoplankton uptake, and the final drawdown in the HC treatment was significantly larger than that of the LC treatment (Fig. 3a, p < 0.01). Early in the nitrogen uptake process the preferential uptake of NH4 + is obvious, as the decrease of NOx started only when NH4 + reached a minimum on day 7 (Fig. 3b). The DIN drawdown difference between treatments was due to the fact that the NOx was not exhausted under the LC scenario (Fig. 3c).

Figure 3
Temporal variations of concentrations of total dissolved inorganic nitrogen (DIN, panel a), NH4 + (b) and Nitrite + Nitrate (c) in 6 enclosures which were perturbed by bubbling with ambient air (400 ppmv CO2, Low CO2 level) or ...
Figure 4
Temporal variations of concentrations of soluble reactive phosphorus (SRP, panel a), dissolved silicate, SiO3 2− (b), and ratios of dissolved inorganic nitrogen to soluble reactive phosphorus (c, DIN/SRP) and to SiO3 2− (d, DIN/SiO3 2− ...

The downward trends of SRP (soluble reactive phosphate) and SiO3 2− concentrations were consistent with that of ammonium, and the SRP concentrations were consumed completely first in LC treatments by day 6 (Fig. 4). Despite the eutrophic status of the collected experimental water, it was also potentially P-limited, as the SRP was first exhausted by day 6 and the initial DIN/SRP ratio was 24.5. This ratio exhibited a sustained increase along with the decline of inorganic nutrient concentrations in the seawater (Fig. 4c). Since more NOx was used in the HC enclosures, the DIN/SRP ratios in HC treatments after day 6 were significantly lower than those of the LC enclosures. Similar results were observed for variations in the DIN/SiO3 2− ratios (Fig. 4d). Ratios of net nutrient uptake (the difference with initial concentrations) also indicated treatment-dependent differences with significantly higher ratios of ΔDIN/ΔSRP and ΔDIN/ΔSiO3 2− in HC enclosures during the nutrient replete period (Fig. 5, day 4–7, n = 4, paired t-Test, p < 0.01). This suggests more consumption of DIN in the HC enclosures relative to SRP and SiO3 2−.

Figure 5
Temporal variations in nutrient consumption ratios of dissolved inorganic nitrogen to soluble reactive phosphorus (a, ΔDIN/ΔSRP) and to SiO3 2− (b, ΔDIN/Δ SiO3 2−) during the nutrients replete period (day ...

Variations on phytoplankton communities and carbon metabolism

During the experiment, algal blooms were induced artificially in the enclosures (Fig. 6a). As there were no zooplankton grazers present, phytoplankton responses to the high CO2 treatments were strictly driven by “bottom-up” influences. Although the initial total chlorophyll a (Chl-a) concentrations of the four phytoplankton species were the same and the initial cell number of the prymnesiophytes was higher than that of the diatoms, the diatoms had an obvious advantage in the highly eutrophic water (Fig. 6). This is evident from the observation that the consumption of SiO3 2− was coupled to that of the other nutrients (Figs 3 and and4),4), as well as the increase in the diagnostic diatom pigment (Fucoxanthin, Fuco) (Fig. 6b).

Figure 6
Temporal variations in concentrations of chlorophyll a (a) and diagnostic pigments of diatoms (b, Fucoxanthin) and prymnesiophytes (c, 19′hexanoyl-oxy-fucoxanthin, 19-Hex) in 6 seawater enclosures which were perturbed by bubbling with ambient ...

Phytoplankton Chl-a biomass reached a significantly higher concentration in the HC treatment on day 9 (185 ± 59 µg L−1), although its response seemed to show a short time lag (Fig. 6a). Prymnesiophytes rapidly responded in the HC enclosures as indicated by their diagnostic pigment 19′hexanoyl-oxy-fucoxanthin (19-Hex), reaching a peak on day 6 (1.4 ± 0.5 µg L−1, Fig. 6c). The temporal variations in the ratio of 19-Hex to Chl-a confirm that the contribution of prymnesiophytes to total Chl-a biomass was higher in the HC enclosures in the early phase (day 2–7), and the opposite was observed during days 8–14 (Fig. 7b). The ratios of Fuco to Chl-a exhibited no clear differences between the different treatments, both with a rising trend following a decline during the first few days (Fig. 7a). Based on the pigment ratios obtained in the mono-culture, the maximum Chl-a concentrations of diatom and prymnesiophytes in the HC enclosures were 166 ± 62 and 21 ± 33 µg L−1, while they were 76 ± 6 and 5.5 ± 3.5 µg L−1 in the LC treatments.

Figure 7
Temporal variations in ratios of fucoxanthin (a, Fuco) and 19′hexanoyl-oxy-fucoxanthin (b, Hex-Fuco) to chlorophyll a in 6 seawater enclosures which were perturbed by bubbling with ambient air (400 ppmv CO2, Low CO2 level) or an air/CO ...

The production of CaCO3 (calcification) by prymnesiophytes in the HC enclosures (1.27 ± 0.07 µmol kg−1 d−1) was significantly lower than in the LC treatment (1.58 ± 0.12 µmol kg−1 d−1), while the production of particulate and dissolved organic carbon (POC and DOC) showed opposite trends (Table 1). These values in the HC enclosures (20.2 ± 7.6 and 29.7 ± 3.4 µM d−1, respectively) were significantly higher than those in the LC condition (8.8 ± 4.0 and 14.2 ± 4.8 µM d−1), respectively (p < 0.01). Thus, the ratios of particulate inorganic carbon (PIC) to POC in the HC enclosures were lower than those in the LC enclosures (Table 1).

Table 1
The overall particulate inorganic carbon (PIC), particulate organic carbon (POC) and dissolved organic carbon (DOC) production rates and PIC:POC ratios during the mesocosm incubations for 15 days under present and elevated partial pressure of CO2 (pCO ...


Enhanced biomass and production under HC treatment

As we mentioned above, acidification in eutrophic waters is not only accompanied by but also coupled to the development of eutrophication3. In natural sea water, typically the DOC concentration is less than 100 µM, and a least half of which is resistant to biological degradation17. In coastal eutrophic seawater, the concentration of labile DOC is high. In our system, the initial concentration was more than 200 µM. It is obvious that the decomposition of DOC led to the high pCO2 in the initial water (805 µatm). Although the initial pCO2 in the water in our study was much higher than the atmospheric CO2, the continued aeration in HC enclosures further exacerbated the pre-existing ocean acidification and reduced the pH (800–1000 ppm, Figs 1 and and2).2). The continued aeration of 400 ppm air reflects the initially high pCO2 water gradually returning to the air sea equilibrium state (400–800 ppm) by the exchange with ambient pCO2 air. Our results confirm the two states. The mean pCO2 levels in the HC and LC treatments were 879.15 ± 145.76 and 658.05 ± 113.98 ppmv, with the significant differences of 221.10 ppmv in the first 4 days (Fig. 2b). Therefore, the results of this study may inform us about phytoplankton responses during a similar natural bloom in current low-pH coastal eutrophic environments under higher atmospheric CO2 concentrations in the future.

Many previous mesocosm studies were conducted in high latitude waters (Table S1), where low temperatures lead to high solubility of CO2, and potentially larger biological effects of acidification6, 7. Our work is the first mesocosm CO2 perturbation study in a eutrophic subtropical ecosystem (24.5°N, 118.2°E) and thus could be comparable to the previous mesocosm experiment in the coastal waters of Korea (34.6°N and 128.5°E)14, 18. However, the Korean experiments were performed in winter. More importantly, these previous studies were done by adding inorganic nutrients to trigger algae blooms. While, we used natural sea water after filtering out particles (< 0.01 µm). The high nutrient concentration is its own characteristics (eutrophication in Chinese coastal water). Nutrients concentrations, nutrients compositions (N/P/Si, NH4 +/NOx, DIN/DON) and other factors (such as metals) were the same as the in-situ seawater with a salinity of 27.3.

In the HC treatment, clear enhancement of phytoplankton total Chl-a biomass and diagnostic pigment concentrations of both diatom and prymnesiophytes were observed (Fig. 6). These results are consistent with the production of particulate and dissolved organic carbon in the HC enclosures (Table 1). The increases in pH and DIN/DIC/pCO2 drawdown due to phytoplankton growth during the experiment were also larger in the HC scenario than those of the LC treatment (Figs 13). Similar to our results, increasing inorganic carbon concentrations have been shown to enhance primary production19 and carbon assimilation in various photoautotrophs. Of course, studies have reported similar results for diatoms20 and coccolithophores21 in mono-culture. Growth of a natural phytoplankton community was also stimulated by elevated CO2 in an Arctic mesocosm experiment, leading to enhanced nutrient uptake and higher biomass build-up right after dissolved inorganic nutrient addition16. The enhanced production and exudation of organic matter in particular stimulated microbial loop activities and altered food web structure7.

It has been suggested that CO2 could limit carbon fixation by marine phytoplankton and by large diatoms in particular, as the free CO2 concentration is usually below that required for half saturation of Ribulose-1, 5-bisphosphate Carboxylase Oxygenase (RUBISCO), the core carbon-fixing enzyme in photosynthesis. There is experimental support for this idea20, 22, even though most phytoplankton can utilize cellular C-concentrating mechanisms (CCM) based on the active uptake of CO2 and/or HCO3 from the environment23. The quite high pH values (8.90) and low pCO2 in water (31 µatm) on day 10 in our HC treatments also indicate that there might be insufficient CO2 for phytoplankton (Figs 1 and and2).2). For diatoms (Phaeodactylum tricornutum), previous studies showed that growth and photosynthetic carbon fixation rates were enhanced by the enrichment of CO2 under low or moderate levels of light24, though photosynthetic inorganic carbon affinity was down regulated by 20% under the high CO2 condition22. Therefore, it is reasonable to infer that the growth of phytoplankton in eutrophic water, in particular that of large diatoms25, can be enhanced by high CO2 (Fig. 6 and Table 1).

However, there are also reports of neutral responses and even negative effects26. Species-specific CO2 responses could result from taxonomic differences among phytoplankton in the physiological mechanisms of CO2 uptake27. In addition to increased pCO2 in seawater under HC, lowered pH can lead to acidic stress. The lower calcification rates (Table 1) reflect a more rapid dissolution of CaCO3 or reduced rates of calcification in the low pH enclosures28. The difference on the ratios of PIC:POC between treatments suggest two opposing effects on the production of organic and inorganic carbon, respectively (Table 1). The lowered pH may also reduce the ability of some species to tolerate high light stress, resulting in increases in respiratory carbon loss29. Thus, whether or not phytoplankton will benefit from increased CO2 remains controversial26, since species-specific behavior and different physiological processes in different waters or experimental conditions are involved29, 30. In eutrophic coastal waters where diatoms dominated in the phytoplankton community, our results support the general proposition that increasing CO2 may promote phytoplankton photosynthesis and growth7, 15.

Species composition under high CO2

Changes in dissolved aqueous CO2 may affect phytoplankton community structure31. A meta-analysis of published experimental data emphasized that the differing responses to elevated pCO2 caused sufficient changes between phytoplankton types in competitive fitness to significantly alter community structure32. Our results indicate a rapid response of prymnesiophytes in the HC treatment, while a short time-lag was observed in the stimulation of diatom growth (Figs 6 and and7).7). This response was the opposite of the expected trend, by which large phytoplankton should grow faster than small phytoplankton in nutrient replete conditions while the latter have the advantage in oligotrophic environments. This unexpected result could be due to the greater contribution of NH4 + to total DIN compared to NO3 , as prymnesiophytes began to decline in day 6 when NH4 + was depleted (Figs 3 and and6).6). Results of an Arctic mesocosm experiment also indicated a positive effect of HC on pico- and nano-eukaryotes during the nutrient replete phase16. The authors of this study suggested that if cells are small enough that their dissolved inorganic carbon supply needs can be met at least partly by diffusion, higher seawater CO2 concentrations could stimulate photosynthetic carbon fixation and growth in these species16.

Our study indicates that diatoms have an overall advantage in eutrophic HC waters compared to prymnesiophytes, although the initial Chl-a concentrations of both groups were the same and the initial cell numbers of prymnesiophytes were even higher than those of diatoms (Fig. 6). As mentioned above, the decreased affinity for HCO3 or/and CO2 and down-regulated CCM in diatom can save CCM-operational energy22, 33, so that increased CO2 availability can be beneficial in terms of energetics. In contrast, prymnesiophytes could have a competitive advantage over diatoms in low CO2 environments34. Similarly, it was observed a clear succession from prymnesiophytes to diatoms when CO2 concentrations increased from 150 to 750 ppmv31. Another experimental study in the North Atlantic Ocean, however, showed a shift away from diatoms and towards coccolithophores under HC, warmer conditions35. It has been suggested that paleooceanographic data showing lower Si:N utilization ratios by phytoplankton during the last glacial maximum could be due to community shifts towards non-siliceous species such as prymnesiophytes caused by decreased CO2 in the glacial atmosphere (180 ppmv)31, although other studies have attributed lower Si:N utilization ratios and export of biogenic Si to relaxed iron limitation of diatoms during glacial periods36. In addition, other factors are likely to be also important, such as light. Prymnesiophytes can grow fast and make dense blooms, but they also like high light conditions37. In a mesocosm where Chl-a reaches such high concentrations, light must be much reduced through self-shading, possibly not favoring prymnesiophyte growth.

Effects on stoichiometry

Overconsumption of carbon relative to nutrient uptake has been reported in several studies of the planktonic response to increased CO2 9, 20, 38. For the same uptake of inorganic nutrients, net community carbon consumption under increased CO2 exceeded present rate by 27 and 39% in 700 and 1050 μatm respectively1. However, many other studies have found contrary trends or no effect of high CO2 on C:N ratios 10, 13, 14, 18, 39. Differing effects of HC on stoichiometric uptake ratios (Table S1) may be attributed to the different biogeochemical demands of the dominant plankton functional types, and life stage-specific biogeochemical requirements13.

Our results indicate a clear increase in N:P and N:Si consumption ratios under HC treatments throughout the experiment, supporting higher Chl-a and production (Figs 36 and Table 1). In other words, assimilations of SRP and SiO3 2− may be reduced relative to that of nitrogen in eutrophic coastal environments under high CO2. A previous study reported that C:P, in contrast to the C:N response, increased significantly in the post-bloom phase18. An Arctic mesocosm project with higher CO2 had higher POC/POP and PON/POP during the nutrient rich phase16. Based on our results, the differences in N:P and N:Si consumption ratios between the two treatments (Figs 4 and and5)5) were completely due to changes in nitrate drawdown (Fig. 3C). Previous study revealed that elevated pCO2 strikingly reduced NO3 uptake and assimilation in the diatom Thalassiosira pseudonana at both high and low light, as indicated by both short-term and steady-state net NO3 uptake rates, which was further supported by the reduced gene transcription, protein expression and enzymatic activity of nitrate reductase at high CO2 33. In parallel, diminished NO3 uptake at elevated pCO2 resulted in lower PON and total protein content40. This could be more important for larger diatoms as they require a greater fraction (by 3.5-fold compared with small ones) of their total cellular nitrogen to RUBISCO for maintaining carbon fixation, hence a higher nitrogen cost in larger diatoms for RUBISCO leads to higher nitrogen requirements25. In addition, accumulating evidence suggests that the nitrogen cycle may respond strongly to higher pCO2 through increases in global N2 fixation41 and possibly denitrification42, as well as decreases in nitrification43.

In contrast, to date, most studies have found negligible or minor effects of projected future changes in pCO2 on most phytoplankton phosphorus requirements10. If indeed N:P and N:Si consumption ratios are elevated under HC environment, the P and Si limitation often observed in fresh and coastal waters will be possibly eased by lower consumption of SRP and Si under HC conditions, relative to the same uptake of DIN (Figs 3 and and4).4). This is also likely to be the cause of higher Chl-a biomass in HC environments with the same initial nutrient concentrations (Fig. 6).

Moreover, the ongoing increase in wind-driven upwelling44 and anthropogenic nutrient inputs in coastal systems45 may increase nutrient inputs and blooms in coastal waters46. The sustained increase in nitrate loading from the Mississippi River47, the Pearl River48 and the Changjiang River49 has resulted in rapidly rising nutrient ratios (N:P and N:Si) since the 1950s, due to increased use of agricultural fertilizers. Associated with the higher Chl-a biomass, species succession and eased P and/or Si limitation discussed above, our study further suggests that future climate and land use changes may result in even more serious and complicated interactive effects of eutrophication, ocean acidification and hypoxia in coastal waters3, 50.


Shallow coastal areas are vulnerable to the effects of human development, and can receive massive loads of fresh water, nutrients, and organic and inorganic carbon. In this study, a mesocosm CO2 perturbation study was conducted to investigate the effect of rising CO2 on a model plankton community in a eutrophic subtropical bay in China. Although the initial DIC and further decomposition of organic matter led to the pCO2 in the coastal water being much higher than that in the air, further enrichment of CO2 appeared to be conducive to the production and biomass of both diatoms and prymnesiophytes. Diatoms had a clear advantage in this highly eutrophic water under the elevated CO2 concentration. However, prymnesiophytes seemingly responded rapidly in the HC enclosures, whereas a time lag was observed in diatom growth. Compared with the low CO2 treatments, the N/P and N/Si consumption ratios significantly increased during the growth of phytoplankton at higher CO2 partial pressure. These results indicate complex effects induced by ocean acidification in phytoplankton stoichiometry, production and community structure in eutrophic coastal waters which may have serious consequences for these biologically and economically important ecosystems.

Material and Methods

Experimental setup and sampling

The Xiamen University mesocosm facility for ocean acidification impacts study (FOANIC-XMU, was deployed in Wuyuan Bay, Xiamen, China (24.5°N, 118.2°E)51. The dimensions of the floating platform are 28 × 10 m, and the facility includes 9 mesocosm enclosures immersed in the seawater along the south side of the platform to avoid shading (Supplementary Material, Fig. S1). The enclosures are 3 m deep and 1.5 m wide, with 50 cm projecting above the sea surface. The volume of the enclosures was 4 m3, and they were composed of a 0.9 mm thick cylindrical transparent thermoplastic polyurethane plastic membrane that is partially transparent to UV. The mesocosms are covered with plastic domes to reduce the contamination risk and prevent rainfall from diluting the experiments.

In order to minimize the influences of other groups of organisms such as grazers, and remove non-living suspended particles that would potentially affect the later measurements of biogenic elements, in situ seawater was filtered through a water purifier (MU801-4T, Midea) which was equipped with 0.01 μm pore size cartridges, and simultaneously injected into the enclosures. Then 0.2 g L−1 of NaCl solution was added into each mesocosm to determine the exact volume by comparison of the salinity before and after salt addition. Ocean acidification conditions were induced gradually with aeration using CO2 enrichlors (CE-100, Wuhan Ruihua Instrument & Equipment, China). The pCO2 of seawater in 6 of the enclosures was perturbed by bubbling with free air (ambient CO2, ~400 ppmv, denoted LC) or using an air/CO2 mixture at the concentration of 1000 ppmv (denoted HC). The air with different CO2 concentrations was delivered into the seawater at a flow rate of ~5 L min−1 with 6 mm diameter plastic tubing, and dispersed by an air stone disk placed in the center of each mesocosm’s bottom. The bubbling was continued for the duration of the whole experiment.

The species interactions of natural populations are typically extremely complicated, depending on the abundance and intrinsic properties of various species as well as other abiotic and biotic factors. Therefore, four well-studied phytoplankton species were used in this study, including the diatoms Phaeodactylum tricornutum (CCMA 106, from Center for Collections of Marine Algae, Xiamen University) and Thalassiosira weissflogii (CCMP 102, from The National Center for Marine Algae and Micobiota, USA), and the coccolithophores Emiliania huxleyi (CS-369, from Commonwealth Scientific and Industrial Research Organization, Australia) and Gephyrocapsa oceanica (NIES-1318, National Institute for Environmental Studies, Japan), were first mono-cultured indoors at 400 and 1000 ppmv CO2. They were acclimated for 10 days (about 10–15 generations) at 20 °C and 150 μmol m−2 s−1 (cool white fluorescence) irradiance using the same eutrophic bay seawater later used for the experiments, collected and filtered in situ without nutrient additions. After the acclimation period, these species were inoculated into each enclosure with equivalent chlorophyll a (Chl-a), respectively, at a total final abundance of 5.07*104 cells L−1. The initial abundances of Phaeodactylum tricornutum, Thalassiosira weissflogii, Emiliania huxleyi and Gephyrocapsa oceanica were about 10000, 700, 20000 and 20000 cells L−1, respectively. The initial cell concentrations were set up based on their differences in size and Chl-a per cell to yield similar initial biomass levels. The growth of these phytoplankton groups was studied for 15 days (15 to 30 June, 2013) under present and elevated partial pressure of CO2 (pCO2 = 400 and 1000 ppmv, respectively) in triplicate 4 m3 enclosures.

Environmental factors

The salinity, temperature and pH profiles in the mesocosm were measured daily at 10:00 AM with a CTD (RBR) or a SeaFET (Satalantic). Due to aeration, these profiles indicated the water in each enclosure was homogenized (Supplementary Material, Fig. S2). The subsamples for chemical and biological determinations were taken at the middle of the mesocosms with a water sampler. The total amount of water for sampling from the enclosures was less than 5% of the initial volume. The pH values were determined using the pH indicator meta-cresol purple with a spectrophotometer (Agilent 8453), with a measurement accuracy of ± 0.0005. The CO2 partial pressure in the seawater (pCO2) was calculated by the program CO2SYS52 from dissolved inorganic carbon (DIC) and total alkalinity (TA)53, 54.

Nutrient samples for NO3  + NO2 (NOx), NH4 + and soluble reactive phosphate (SRP) were filtered immediately after collection through 47 mm GF/F filters and were then frozen at −20 °C. Samples for SiO3 2− were filtered through acid-cleaned 0.45 µm pore size acetate cellulose filters and were kept refrigerated at 4 °C. Filtrates for NH4 + and SiO3 2− were preserved with 100 μL CCl4. All the nutrient samples were measured in our land-based laboratory at Xiamen University within 15 days after the mesocosm experiment. Nutrient samples for NOX, SRP and SiO3 2− were analysed using a four-channel continuous-flow Technicon AA3 Auto-Analyzer (Bran-Lube GmbH)55. NOx was analyzed using the copper-cadmium column reduction method5. SRP and SiO3 2− were measured using typical spectrophotometric methods56. NH4 + was run with a 722 type spectrophotometer (Xiamen Analytical Instrument Co., China) according to the indophenol blue spectrophotometric method5, 57. The precision for nutrient analyses in this study was ≤3%, and the detection limits for NOx, SRP, SiO3 2− and NH4 + analyses were 0.03, 0.03, 0.05 and 0.16 μM, respectively.

Phytoplankton biomass and community structure

Photosynthetic pigment concentrations were measured by high-performance liquid chromatography (HPLC) using a Shimadzu 20 A HPLC system fitted with a 3.5 μm Eclipse XDB C8 column (4.6 × 150 mm, Agilent Technologies, Waldbronn, Germany), as in our previous studies8, 58. Briefly, seawater samples for phytoplankton pigment analysis (0.2–2 L, according to biomass) were filtered through 25 mm GF/F glass fiber filters (under a vacuum pressure < 10 kPa under dim light), and then they were immediately frozen (−80 °C) until analysis in the laboratory within 30 days. Phytoplankton pigments were extracted in N, N-dimethylformamide and analyzed. The concentrations of chlorophyll a (Chl-a), diagnostic pigments of diatoms, (fucoxanthin, Fuco) and prymnesiophytes (19′hexanoyl-oxy-fucoxanthin, 19-Hex) were detected, and quantified using standards that were purchased from DHI Water & Environment, Hørsholm, Denmark.

Pigment samples of the four phytoplankton species were collected in exponential growth phase during mono-culture under indoor conditions to obtain the ratios of diagnostic pigments to Chl-a for CHEMTAX analyses8, 58. These initial pigments ratios might be quite different from those of the same species grown under sunlight in the mesocosms. To confirm the phytoplankton community structure based on pigments information, a 0.5 L water sample was collected and preserved with Lugol’s iodine solution for microscopic observation. The Chl-a concentrations were also compared to the cell number, and these two values were significantly correlated (Supplementary Material, Fig. S3, R2 = 0.76, n = 27, p < 0.01).

Carbon metabolism

Net calcification rate was estimated by the TA anomaly method59. TA was measured by potentiometric titration using the Gran procedure60. In addition, TA has to be corrected for the effect of primary production, i.e., since an uptake of 1 mol NO3 or PO4 3− increases TA by 1 mole59, and an uptake of 1 mol NH4 + decreases TA by 1 mole61. Thus, the net calcification rate can be estimated as equation (1).

Net calcification rate = − 0.5 × (ΔTAmeasured − ΔNO3 − ΔPO43− + ΔNH4+)/Δt

For particulate organic carbon (POC) sampling, seawater was filtered through a pre-combusted 47 mm GF/F filter (Whatman). Prior to analysis, the filters were frozen at −20 °C and POC (via acid fuming) was determined with a PE-2400 SERIES IICHNS/O analyzer according to the JGOFS protocols56. Dissolved organic carbon (DOC) samples were filtering onto pre-combusted 25 mm GF/F filters and stored in pre-combusted EPA vials at −20 °C until analysis using a Shimadzu TOC-V Analyzer62. The overall POC and DOC production rates for 15 days (day 0–day 14) were calculated according to the following equations:

POC production rate = ΔPOCt

DOC production rate = ΔDOCt

Since particulate inorganic carbon (PIC) samples were limited, we assumed that all PIC is in the form of CaCO3. Accordingly, the PIC value in this study was calculated with the following formula63:

ΔPICcalculatedCaCO3 accumulation = − 0.5 × (ΔTAmeasured − ΔNO3 − ΔPO43− + ΔNH4+)

In all the formulas above, ΔTA, ΔNO3 , ΔPO4 3−, ΔNH4 +, ΔDOC, ΔPOC, ΔPICcalculated denote the changes of these parameters, and Δt denotes the elapsed time. A one-way ANOVA was used for statistical analysis following a test for homogeneity of the variances. The significance level was set at p < 0.05. ANOVA results were compared using the Tukey HSD method.

Electronic supplementary material


This work was supported by grants from the National Key R&D Program of China (No. 2016YFA0601203), and the China NSF (Nos. 41406143, 41430967, 41120164007, 41330961, and 41206091), State Oceanic Administration (National Program on Global Change and Air-Sea Interaction, GASI-03-01-02-04), and the U.S. National Science Foundation Biological Oceanography (OCE 1538525). Visit of DH and FF was supported by “111” project. We would like to thank Tao Huang and Shuimiao Lu for help with the data collection. We also thank Yahe Li, Nana Liu, Liguo Guo, Jianzhong Su, Zhouling Zhang, Peng Jin, Wei Li, Jiancheng Ding, Futian Li, Tifeng Wang, Shanying Tong, Tao Xing, Jie Zhou, and Juntian Xu, who all took part in the mesocosm experiments; we also grateful to the technical supporting staff, Xianglan Zeng, Wenyan Zhao and Litong Peng.

Author Contributions

Author Contributions

X. Liu, Y. Li and Y. Wu contributed equally to this paper for their leading roles in field sampling and writing of the manuscript. D. Hutchins and F. Fu contributed to writing and editing the manuscript. K. Gao, M. Dai and B. Huang initially designed the study and supervised the projects. This study was conceived in discussions between all authors.


Competing Interests

The authors declare that they have no competing interests.


Xin Liu, Yan Li and Yaping Wu contributed equally to this work.

Electronic supplementary material

Supplementary information accompanies this paper at doi:10.1038/s41598-017-07195-8

Publisher's note: Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.

Contributor Information

Bangqin Huang, nc.ude.umx@gnauhqb.

Minhan Dai, nc.ude.umx@iadm.

Kunshan Gao, nc.ude.umx@oagsk.


1. Riebesell U, et al. Enhanced biological carbon consumption in a high CO2 ocean. Nature. 2007;450:545–548. doi: 10.1038/nature06267. [PubMed] [Cross Ref]
2. Busch DS, et al. Understanding, characterizing, and communicating responses to ocean acidification: challenges and uncertainties. Oceanography. 2015;25:30–39. doi: 10.5670/oceanog.2015.29. [Cross Ref]
3. Cai WJ, et al. Acidification of subsurface coastal waters enhanced by eutrophication. Nat. Geosci. 2011;4:766–770. doi: 10.1038/ngeo1297. [Cross Ref]
4. Zhai W, Dai M, Cai WJ, Wang Y, Wang Z. High partial pressure of CO2 and its maintaining mechanism in a subtropical estuary: the Pearl River estuary, China. Mar. Chem. 2005;93:21–32. doi: 10.1016/j.marchem.2004.07.003. [Cross Ref]
5. Dai M, et al. Nitrification and inorganic nitrogen distribution in a large perturbed river/estuarine system: the Pearl River estuary, China. Biogeosciences. 2008;5:1227–1244. doi: 10.5194/bg-5-1227-2008. [Cross Ref]
6. Riebesell U, Bellerby RGJ, Grossart HP, Thingstad F. Mesocosm CO2 perturbation studies: from organism to community level. Biogeosciences. 2008;5:1157–1164. doi: 10.5194/bg-5-1157-2008. [Cross Ref]
7. Riebesell U, Gattuso JP, Thingstad TF, Middelburg JJ. “Arctic ocean acidification: pelagic ecosystem and biogeochemical responses during a mesocosm study” Biogeosciences. 2013;10:5619–5626. doi: 10.5194/bg-10-5619-2013. [Cross Ref]
8. Liu X, et al. Responses of phytoplankton communities to environmental variability in the East China Sea. Ecosystems. 2016;19:832–849. doi: 10.1007/s10021-016-9970-5. [Cross Ref]
9. Bellerby RGJ, et al. Marine ecosystem community carbon and nutrient uptake stoichiometry under varying ocean acidification during the PeECE III experiment. Biogeosciences. 2008;5:1517–1527. doi: 10.5194/bg-5-1517-2008. [Cross Ref]
10. Hutchins DA, Mulholland MR, Fu F. Nutrient Cycles and Marine Microbes in a CO2-Enriched Ocean. Oceanography. 2009;22:128–145. doi: 10.5670/oceanog.2009.103. [Cross Ref]
11. Riebesell U, Gattuso JP. Lessons learned from ocean acidification research. Nat. Clim. Change. 2015;5:12–14. doi: 10.1038/nclimate2456. [Cross Ref]
12. Tatters AO, et al. Short- and long-term conditioning of a temperate marine diatom community to acidification and warming. Philos. Trans. R. Soc. Lond. B. Biol. Sci. 2013;368:20120437. doi: 10.1098/rstb.2012.0437. [PMC free article] [PubMed] [Cross Ref]
13. Silyakova A, et al. Pelagic community production and carbon-nutrient stoichiometry under variable ocean acidification in an Arctic fjord. Biogeosciences. 2013;10:4847–4859. doi: 10.5194/bg-10-4847-2013. [Cross Ref]
14. Kim JM, et al. Shifts in biogenic carbon flow from particulate to dissolved forms under high carbon dioxide and warm ocean conditions. Geophys. Res. Lett. 2011;38:L08612.
15. Kim JH, et al. Enhancement of photosynthetic carbon assimilation efficiency by phytoplankton in the future coastal ocean. Biogeosciences. 2013;10:7525–7535. doi: 10.5194/bg-10-7525-2013. [Cross Ref]
16. Schulz KG, et al. Temporal biomass dynamics of an Arctic plankton bloom in response to increasing levels of atmospheric carbon dioxide. Biogeosciences. 2013;10:161–180. doi: 10.5194/bg-10-161-2013. [Cross Ref]
17. Wu K, et al. Dissolved organic carbon in the South China Sea and its exchange with the Western Pacific Ocean. Deep Sea Res. II. 2015;122:41–51. doi: 10.1016/j.dsr2.2015.06.013. [Cross Ref]
18. Kim JM, et al. The effect of seawater CO2 concentration on growth of a natural phytoplankton assemblage in a controlled mesocosm experiment. Limnol. Oceanogr. 2006;51:1629–1636. doi: 10.4319/lo.2006.51.4.1629. [Cross Ref]
19. Hein M, Sand-Jensen K. CO2 increases oceanic primary production. Nature. 1997;388:526–527. doi: 10.1038/41457. [Cross Ref]
20. Riebesell U, Wolf-Gladrow DA, Smetacek V. Carbon dioxide limitation of marine phytoplankton growth rates. Nature. 1993;361:249–251. doi: 10.1038/361249a0. [Cross Ref]
21. Feng Y, et al. Interactive effects of increased pCO2, temperature and irradiance on the marine coccolithophore Emiliania huxleyi (Prymnesiophyceae) Eur. J. Phycol. 2008;43:87–98. doi: 10.1080/09670260701664674. [Cross Ref]
22. Wu Y, Gao K, Riebesell U. CO2-induced seawater acidification affects physiological performance of the marine diatom Phaeodactylum tricornutum. Biogeosciences. 2010;7:2915–2923. doi: 10.5194/bg-7-2915-2010. [Cross Ref]
23. Raven JA, Giordano M, Beardall J, Maberly SC. Algal and aquatic plant carbon concentrating mechanisms in relation to environmental change. Photosynthesis Res. 2011;109:281–296. doi: 10.1007/s11120-011-9632-6. [PubMed] [Cross Ref]
24. Gao KS, Campbell DA. Photophysiological responses of marine diatoms to elevated CO2 and decreased pH: a review. Funct. Plant Biol. 2014;41:449–459. doi: 10.1071/FP13247. [Cross Ref]
25. Wu Y, Jeans J, Suggett DJ, Finkel ZV, Campbell DA. Large centric diatoms allocate more cellular nitrogen to photosynthesis to counter slower RUBISCO turnover rates. Front. Mar. Sci. 2014;1:1–11.
26. Mackey K, Morris JJ, Morel F, Kranz S. Response of photosynthesis to ocean acidification. Oceanography. 2015;25:74–91. doi: 10.5670/oceanog.2015.33. [Cross Ref]
27. Raven JA, Johnston AM. Mechanisms of inorganic-carbon acquisition in marine phytoplankton and their implications for the use of other resources. Limnol. Oceanogr. 1991;36:1701–1714. doi: 10.4319/lo.1991.36.8.1701. [Cross Ref]
28. Riebesell U, et al. Reduced calcification of marine plankton in response to increased atmospheric CO2. Nature. 2000;407:364–367. doi: 10.1038/35030078. [PubMed] [Cross Ref]
29. Gao K, Helbling EW, Häder DP, Hutchins DA. Responses of marine primary producers to interactions between ocean acidification, solar radiation, and warming. Mar. Ecol. Prog. Ser. 2012;470:167–189. doi: 10.3354/meps10043. [Cross Ref]
30. Wu HY, Zou DH, Gao KS. Impacts of increased atmospheric CO2 concentration on photosynthesis and growth of micro- and macro-algae. Sci. China Ser. C. 2008;51:1144–1150. doi: 10.1007/s11427-008-0142-5. [PubMed] [Cross Ref]
31. Tortell PD, DiTullio GR, Sigman DM, Morel FMM. CO2 effects on taxonomic composition and nutrient utilization in an Equatorial Pacific phytoplankton assemblage. Mar. Ecol. Prog. Ser. 2002;236:37–43. doi: 10.3354/meps236037. [Cross Ref]
32. Dutkiewicz S, et al. Impact of ocean acidification on the structure of future phytoplankton communities. Nat. Clim. Change. 2015;5:1002–1006. doi: 10.1038/nclimate2722. [Cross Ref]
33. Shi D, et al. Interactive effects of light, nitrogen source, and carbon dioxide on energy metabolism in the diatom Thalassiosira pseudonana. Limnol. Oceanogr. 2015;60:1805–1822. doi: 10.1002/lno.10134. [Cross Ref]
34. Hinga KR. Co-occurrence of dinoflagellate blooms and high pH in marine enclosures. Mar. Ecol. Prog. Ser. 1992;86:181–181. doi: 10.3354/meps086181. [Cross Ref]
35. Feng Y, et al. Effects of increased pCO2 and temperature on the North Atlantic spring bloom. I. The phytoplankton community and biogeochemical response. Mar. Ecol. Prog. Ser. 2009;388:13–25. doi: 10.3354/meps08133. [Cross Ref]
36. Hutchins DA, Bruland KW. Iron-limited diatom growth and Si: N uptake ratios in a coastal upwelling regime. Nature. 1998;393:561–564. doi: 10.1038/31203. [Cross Ref]
37. Ziveri P, Broerse ATC, van Hinte JE, Westbroek P, Honjo S. The fate of coccoliths at 48°N 21°W, northeastern Atlantic . Deep Sea Res. II. 2000;47:1853–1875. doi: 10.1016/S0967-0645(00)00009-6. [Cross Ref]
38. Zark M, Riebesell U, Dittmar T. Effects of ocean acidification on marine dissolved organic matter are not detectable over the succession of phytoplankton blooms. Science Advances. 2015;1:e1500531. doi: 10.1126/sciadv.1500531. [PMC free article] [PubMed] [Cross Ref]
39. Engel A, et al. Testing the direct effect of CO2 concentration on a bloom of the coccolithophorid Emiliania huxleyi in mesocosm experiments. Limnol. Oceanogr. 2005;50:493–507. doi: 10.4319/lo.2005.50.2.0493. [Cross Ref]
40. Hennon GMM, Quay P, Morales RL, Swanson LM, Armbrust EV. Acclimation conditions modify physiological response of the diatom Thalassiosira pseudonana to elevated CO2 concentrations in a nitrate-limited chemostat. J. Phycol. 2014;50:243–253. doi: 10.1111/jpy.12156. [PubMed] [Cross Ref]
41. Hutchins D, et al. CO2 control of Trichodesmium N2 fixation, photosynthesis, growth rates, and elemental ratios: Implications for past, present, and future ocean biogeochemistry. Limnol. Oceanogr. 2007;52:1293. doi: 10.4319/lo.2007.52.4.1293. [Cross Ref]
42. Fennel, K., Wilkin, J., Previdi, M. & Najjar, R. Denitrification effects on air-sea CO2 flux in the coastal ocean: Simulations for the northwest North Atlantic. Geophys. Res. Lett. 35 (2008).
43. Beman JM, et al. Global declines in oceanic nitrification rates as a consequence of ocean acidification. Proc. Natl. Acad. Sci. USA. 2011;108:208–213. doi: 10.1073/pnas.1011053108. [PubMed] [Cross Ref]
44. Bakun A. Global climate change and intensification of coastal ocean upwelling. Science. 1990;247:198–201. doi: 10.1126/science.247.4939.198. [PubMed] [Cross Ref]
45. Kim IN, et al. Increasing anthropogenic nitrogen in the North Pacific. Ocean. Science. 2014;346:1102–1106. [PubMed]
46. Glibert PM, et al. Vulnerability of coastal ecosystems to changes in harmful algal bloom distribution in response to climate change: projections based on model analysis. Global. Change. Biol. 2014;20:3845–3858. doi: 10.1111/gcb.12662. [PubMed] [Cross Ref]
47. Rabalais NN, et al. Hypoxia in the northern Gulf of Mexico: Does the science support the plan to reduce, mitigate, and control hypoxia? Estuar. Coast. 2007;30:753–772. doi: 10.1007/BF02841332. [Cross Ref]
48. Harrison P, Yin K, Lee J, Gan J, Liu H. Physical–biological coupling in the Pearl River estuary. Cont. Shelf. Res. 2008;28:1405–1415. doi: 10.1016/j.csr.2007.02.011. [Cross Ref]
49. Zhou MJ, Shen ZL, Yu RC. Responses of a coastal phytoplankton community to increased nutrient input from the Changjiang (Yangtze) River. Cont. Shelf. Res. 2008;28:1483–1489. doi: 10.1016/j.csr.2007.02.009. [Cross Ref]
50. Greene RM, Lehrter JC, Hagy JD. Multiple regression models for hindcasting and forecasting midsummer hypoxia in the Gulf of Mexico. Ecol. Appl. 2009;19:1161–1175. doi: 10.1890/08-0035.1. [PubMed] [Cross Ref]
51. Xing T, Wu YP, Ding JC, Gao KS. Diurnal light utilization efficiency of phytoplankton is decreased by elevated CO2 concentration: a mesocosm experiment. Fundam. Appl. Limnol. 2016;188:83–92. doi: 10.1127/fal/2016/0885. [Cross Ref]
52. Lewis, E., Wallace, D. & Allison, L. J. Program developed for CO2system calculations. (Carbon Dioxide Information Analysis Center, managed by Lockheed Martin Energy Research Corporation for the US Department of Energy Tennessee, 1998).
53. Langdon, C. & Atkinson, M. J. Effect of elevated pCO2 on photosynthesis and calcification of corals and interactions with seasonal change in temperature/irradiance and nutrient enrichment. J. Geophys. Res. (Oceans)110, doi:10.1029/2004jc002576 (2005).
54. Millero, F. J. In Chemical Oceanography (ed Frank J Millero) 259–329 (CRC press, 2013).
55. Han A, et al. Nutrient dynamics and biological consumption in a large continental shelf system under the influence of both a river plume and coastal upwelling. Limnol. Oceanogr. 2012;57:486–502. doi: 10.4319/lo.2012.57.2.0486. [Cross Ref]
56. Knap, A. H., Michaels, A., Close, A. R., Ducklow, H. & Dickson, A. G. Protocols for the joint global ocean flux study (JGOFS) core measurements. JGOFS, Reprint of the IOC Manuals and Guides No. 29, UNESCO 199419 (1996).
57. Pai SC, Tsau YJ, Yang TI. pH and buffering capacity problems involved in the determination of ammonia in saline water using the indophenol blue spectrophotometric method. Anal. Chim. Acta. 2001;434:209–216. doi: 10.1016/S0003-2670(01)00851-0. [Cross Ref]
58. Liu X, et al. High-resolution phytoplankton diel variations in the summer stratified central Yellow Sea. J. Oceanogr. 2012;68:913–927. doi: 10.1007/s10872-012-0144-6. [Cross Ref]
59. Delille B, et al. Response of primary production and calcification to changes of pCO2 during experimental blooms of the coccolithophorid Emiliania huxleyi. Global Biogeochem. Cycles. 2005;19:GB2023. doi: 10.1029/2004GB002318. [Cross Ref]
60. Wang ZA, Cai WJ. Carbon dioxide degassing and inorganic carbon export from a marsh-dominated estuary (the Duplin River): A marsh CO2 pump. Limnol. Oceanogr. 2004;49:341–354. doi: 10.4319/lo.2004.49.2.0341. [Cross Ref]
61. Wolf-Gladrow DA, Zeebe RE, Klaas C, Körtzinger A, Dickson AG. Total alkalinity: The explicit conservative expression and its application to biogeochemical processes. Mar. Chem. 2007;106:287–300. doi: 10.1016/j.marchem.2007.01.006. [Cross Ref]
62. Dai M, et al. Excess total organic carbon in the intermediate water of the South China Sea and its export to the North Pacific. Geochem Geophy Geosy. 2009;10:Q12002. doi: 10.1029/2009GC002752. [Cross Ref]
63. De Bodt C, Harlay J, Chou L. Biocalcification by Emiliania huxleyi in batch culture experiments. Mineral. Mag. 2008;72:251–256. doi: 10.1180/minmag.2008.072.1.251. [Cross Ref]

Articles from Scientific Reports are provided here courtesy of Nature Publishing Group