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Toxins 2014, 6(1), 229-253; doi:10.3390/toxins6010229
Published: 3 January 2014
Abstract: Benthic marine dioflagellate microalgae belonging to the genus Prorocentrum are a major source of okadaic acid (OA), OA analogues and polyketides. However, dinoflagellates produce these valuable toxins and bioactives in tiny quantities, and they grow slowly compared to other commercially used microalgae. This hinders evaluation in possible large-scale applications. The careful selection of producer species is therefore crucial for success in a hypothetical scale-up of culture, as are appropriate environmental conditions for optimal growth. A clone of the marine toxic dinoflagellate P. belizeanum was studied in vitro to evaluate its capacities to grow and produce OA as an indicator of general polyketide toxin production under the simultaneous influence of temperature (T) and irradiance (I0). Three temperatures and four irradiance levels were tested (18, 25 and 28 °C; 20, 40, 80 and 120 µE·m−2·s−1), and the response variables measured were concentration of cells, maximum photochemical yield of photosystem II (PSII), pigments and OA. Experiments were conducted in T-flasks, since their parallelepipedal geometry proved ideal to ensure optically thin cultures, which are essential for reliable modeling of growth-irradiance curves. The net maximum specific growth rate (µm) was 0.204 day−1 at 25 °C and 40 µE·m−2·s−1. Photo-inhibition was observed at I0 > 40 μEm−2s−1, leading to culture death at 120 µE·m−2·s−1 and 28 °C. Cells at I0 ≥ 80 µE·m−2·s−1 were photoinhibited irrespective of the temperature assayed. A mechanistic model for µm-I0 curves and another empirical model for relating µm-T satisfactorily interpreted the growth kinetics obtained. ANOVA for responses of PSII maximum photochemical yield and pigment profile has demonstrated that P. belizeanum is extremely light sensitive. The pool of photoprotective pigments (diadinoxanthin and dinoxanthin) and peridinin was not able to regulate the excessive light-absorption at high I0-T. OA synthesis in cells was decoupled from optimal growth conditions, as OA overproduction was observed at high temperatures and when both temperature and irradiance were low. T-flask culture observations were consistent with preliminary assays outdoors.
Microalgal dinoﬂagellates are a major source of structurally diverse bioactive natural products and toxins with potential uses in biomedical, toxicological and pharmacological research . Most of these molecules have not progressed beyond the discovery stage because of limited availability from the natural source and difﬁculty of synthesis due to structural complexity. Many source species have proved difﬁcult to culture in the laboratory or have failed to produce the desired compound under artiﬁcial culture conditions. In fact, of the marine bioactives and toxins under clinical evaluation , none has been sourced from dinoﬂagellates. Toxins from dinoﬂagellates are also attracting increasing attention because of their impact on the safety of seafood.
Only sparing quantities of dinoﬂagellate toxins are generally available, and this hinders bioactivity characterization and evaluation in potential applications. Approaches to production of increased quantities of dinoﬂagellate bioactives are needed , since the titer of the target toxin is often low. For example, the production of 150 g of a certain dinoflagellate toxin is estimated to require a culture broth volume of between 103 (Alexandrium minute) and 105 m3 (Gambierdiscus toxicus) . This is far larger than the volume of the fermentation broth needed to produce the same quantity of a typical antibiotic, for example. The handling of such a large volume of broth of a highly toxic material could be a major problem . Raising the concentration of the bioactive in the broth is a major issue to reduce both the volume to be handled and production costs. The concentration of a target compound can be enhanced by modifying and combining different levels of culture of abiotic factors.
Under nutrient excess, light and temperature are widely accepted as the driving factors acting on the overall biochemical composition of biomass and growth in microalgal cultures. Laboratory studies have also confirmed that temperature and light can significantly influence the growth rate and toxin production of dinoflagellates [5,6]. It is therefore essential to establish experimentally the individual and/or interacting effects of irradiance and temperature on cultures of dinoflagellates of interest in order to improve growth and toxin yields.
The marine dinoflagellate Prorocentrum belizeanum was selected because it is a recent source of okadaic acid analogues, polyketides and macrolides of interest (e.g., corozalic acid, belizeanolide, belizeanic acid) [7,8,9,10,11,12]. Marine dinoflagellates of the genus Prorocentrum are famous for the production of okadaic acid (OA) and its analogues, which are inhibitors of protein phosphatases types 1 (PP1) and 2A (PP2A), and causative toxins of diarrhetic shellfish poisoning (DSP) .
Since the physiology of P. belizeanum is yet to be investigated as a required stage of a potential bioprocess, the aim of this work was to evaluate the simultaneous influence of irradiance and temperature on growth kinetics, maximum photochemical yield of the photosystem II (PSII), pigment profile and OA production, by using several combinations of the two variables. This work also sought to establish relationships between response variables and the physiological state of the cells, in order to monitor more easily the current status of the culture.
2. Results and Discussion
2.1. Growth Kinetics and Modeling
The relative attenuation of irradiance in the T-Flask cultures over time was calculated as detailed in the Materials and Methods section. In general, the mutual shading increased with the age of the culture and the cell concentration (data not shown). The highest light attenuation values were observed in the stationary phase, reaching a maximum of around 10% in the experiment carried out at 25 °C and 40 µE·m−2·s−1. In the exponential phase, mutual shading in all the cultures was substantially below 10%. Consequently, our cultures can be considered optically thin, i.e., it is unlikely that self-shading affected the experimental results reported. This issue is critical in the modeling of the P-I curves (growth or photosynthesis rate versus irradiance). These curves derived from laboratory studies are commonly used to predict biomass productivity in photobioreactors or natural habitats (e.g., microalgal blooms), where the cell density is high, and hence also the effect of light attenuation. If the estimated kinetic parameters are markedly affected by mutual shading or acclimation phenomena, the predictions could be wrong, and the denser the culture systems, the greater the error. Novel aspects related with the modeling of P-I curves in microalgae have comprehensively been addressed in a recent study .
Figure 1 shows profiles of cell density with time for all experiments and T and I0 combinations. A maximum cell concentration of 134 × 103 cells∙mL−1 was attained at 25 °C and 40 μEs−1m−2. It can also be observed that the selected asymmetric logistic equations (ALEs; see Experimental Section 3) were able to fit the different experimental asymmetric growth curves. As shown in Figure 2, there is a good agreement (within ±25%) between measured data and values predicted from ALEs for all datasets. Clearly, Equation (2) fits experimental data obtained under different T and I0 quite well, supporting its use for estimating the typical physiological response in all phases of P. belizeanum batch cultures.
Maximum specific growth rates over time were calculated with Equation (3) by analytical differentiation of the ALE (Equation (2) of Experimental Section 3). The µm values of every T-Flask culture were used to evaluate the effect of T and I0 on cell growth. Inspection of Figure 3, where the dependence of µm on I0 and T is illustrated, reveals that the temperature of 25 °C also provided the highest µm value (0.204 day−1). Although no temperature effects on growth of P. belizeanum have been reported in the literature, optimal growth temperatures for other species of the genus Prorocentrum ranging from 10 to 29 °C are well-documented [15,16,17,18]. The optimal irradiance, Iopt, seemed to be around 50 µE·m−2·s−1 at 25 °C. While this value is very close to the irradiance levels used in many studies to grow the genus Prorocentrum for different purposes [19,20,21,22,23], it is far lower than those reported as optimum for other species of the same genus. For example, Iopt for Prorocentrum lima [24,25] was found to vary from 150 to 180 µE·m−2·s−1.
The curves µm-I0 in Figure 3a are similar to the typical P-I curves of microalgae where three main areas can be distinguished: (i) a light-limited region (≤40 μEm−2s−1) in which the light-absorption step controls the rate of the subsequent cell metabolic processes; (ii) zone of higher illumination (around 50 μEm−2s−1) in which sufficient energy is available for the cell metabolic processes to become saturated and the rate of photosynthesis is no longer a strong function of the irradiance (i.e., metabolic assimilation of energy becomes the rate-controlling step); and (iii) a photo-inhibition region (>40 μEm−2s−1), in which irradiance becomes detrimental, decreasing the growth rate and even leading to culture death as in the experiment carried out at I = 120 µE·m−2·s−1 and T = 28 °C. P. belizeanum cultures at I0 ≥ 80 µE·m−2·s−1 were photoinhibited irrespective of the temperature assayed. The extension and shape of the aforementioned µm-I0 curve zones depended on the culture temperature (see Figure 3a). Microalgae can acclimatize their photosynthetic system in response to shifts in temperature, modifying their irradiance requirements for optimal growth. As a result, microalgae can tolerate higher irradiances at temperatures closer to their optimum , i.e., saturation intensity increases with temperature. As stated above, and as Figure 3 illustrates, P. belizeanum presented an optimal growth temperature of around 25 °C, which corresponded to the highest µm values.
Lines in Figure 3 show the fit of the present models (Equations (4) and (5) of Experimental Section 3) to the experimental data of µm. The best-fit values of the kinetic parameters are displayed in Table 1 and Table 2. The values of the parameters of the µm-I model (see Table 1) were consistent with other simulations reported elsewhere . For instance, the values of α reasonably correspond to the boundary irradiance value (I0 = α) that separates the light-limitation region from the light-saturated photosynthesis zone (see Figure 3a). Thus, when I0 < α, the photosynthesis or growth rate depends strongly on irradiance. When I0 > α, cultures are light-saturated, and if I0 is sufficiently increased above α, cells may become photoinhibited. As expected, values of the cell maintenance rate (m) were clearly lower than the maximum specific growth rate (µmax). Values of µmax were similar. There is a degree of debate regarding the ideal value of exponent n, reaction order of the photoinhibition rate, which is 0.5 or 1 according to different authors . The n values obtained were close to 1, the main deviation corresponding to 28 °C.
|Table 1. Parameter estimation from fitting the µm-I model (Equation (4) of Experimental Section 3) to data gathered by temperature (see Figure 3a) using non-linear regression.|
|18 °C||25 °C||28 °C|
|α (µE m−2 s−1)||78.21||54.72||82.97|
|δ (µE−n m2n sn)||4.6 × 10−3||1.3 × 10−3||3.7 × 10−5|
|* R2 (-)||0.999||0.999||0.939|
Note: * Determination coefficient.
|Table 2. Parameter estimation from fitting the µm-T model (Equation (5) of Experimental Section 3) to data gathered by irradiance (see Figure 3b) using non-linear regression.|
|40 µE·m−2·s−1||80 µE·m−2·s−1|
|β (-)||6 × 10−7||1.3 × 10−6|
|* R2 (-)||0.999||0.999|
Note: * Determination coefficient.
The values of the parameters for the µm-T model in Table 2 were consistent with those reported by Huang et al. (2011) for microorganisms . Other models based on the Arrhenius equation  could also have been suitable for fitting the data with similar accuracy within the experimental range (data not shown). However, the Tmin values estimated by the Huang’s model (Equation (5) of Experimental Section 3) are closer to the biological minimum of both psychrotrophs and mesophyles as discussed elsewhere . Even so, all the commonly used µm-T models are formulated in such a way that µm has to be zero out of the interval [Tmin, Tmax]. It is an important hurdle because negative net growth rates cannot be predicted. In fact, experimental µm-T data at 28 °C could not be fitted to Equation (5), since the µm value at 120 µE·m−2·s−1 was negative (see Figure 3a). Therefore, negative specific growth rates due to cell mortality should be taken into consideration for T > Tmax. This is critical in the control of outdoor microalgal production processes, in which biomass destruction after a high temperature episode (T > Tmax) should be taken into account for an accurate prediction of the total biomass evolution .
Modeling of the simultaneous effect of T and I0 on µm was not presented here, although it was relatively straightforward from Equations (4) and (5) by coupling the effects of I0 and T. From a realistic point of view, uncoupled models can be seen as a functional artefact to replace coupled models that better represent the interdependent impact of T and I0 on photosynthesis, but are more difficult to obtain. This T-I0 interplay should be expressed by variation of the kinetic parameters of any P-I model with the temperature. Variation of the parameters in Table 1 with T are evidence of this, as are other cases reported in the literature, e.g., variation of saturation irradiance with T in cultures of harmful dinoflagellates of the genus Ceratium . However, coupled models have a large number of parameters, and therefore a high number of experiments are needed in order to fit without risk of overfitting . Future work should focus on this direction.
2.2. Maximum Photochemical Yield (Fv/Fm)
Fv/Fm, which is the ratio of variable fluorescence to maximal fluorescence (see Experimental Section 3), provides an estimate of the PSII maximum efficiency within dark-adapted material. Measurements of Fv/Fm with the time of culture were recorded for all the experiments. To analyze the effect of the factors involved (T, I0, and time) and their interactions on the variability of Fv/Fm, a multifactor ANOVA was carried out, and the results are shown in Table 3. All factors and interactions, except for I0-t, had a statistically significant effect on Fv/Fm at the 95.0% confidence level (p < 0.05). However, the contributions of the time of culture (4.44%) and of the sum of all interactions (14.87%) to the global variation of Fv/Fm were substantially lower than those of temperature (26.59%) and irradiance (54.09%). Figure 3 shows the mean µm values reached for each T and I0 and the intervals around each mean value. Fisher’s least significant difference (LSD) procedure was used for establishing discrimination among the means. Thus, for irradiances and temperatures above 40 µE·m−2·s−1 and 25 °C, respectively, there were statistically significant differences between factor levels. These values of I0 and T divided the plots in Figure 4 into two zones that allowed the separation of photoinhibited or thermally stressed cells from healthy cells in function of the recorded Fv/Fm. Photoinhibition of photosynthesis was clearly identified in Figure 4a by a light-induced depression in Fv/Fm. Photoinhibition at sub-optimal temperature (18 °C) was not observed in Figure 4b.
Figure 5 displays the impact of T-I0 interactions on Fv/Fm. Notice that the effect of photoinhibition and thermal stress is strengthened at high temperatures (>25 °C) and irradiances (>40 µE·m−2·s−1), respectively. These results are therefore in line with the aforementioned observations derived from the analysis of µm-I0 and µm-T curves.
|Table 3. Multifactor ANOVA testing the effect of temperature (T), irradiance (I0) and time of culture (t) on different cellular responses: maximum quantum yield (Fv/Fm), cell content of pigments (Chlorophyll a, Chl a; Chlorophyll c2, Chl c; Peridinin, Pe; Diadinoxanthin, Dd; Dinoxanthin, Dn) and production of okadaic acid (OA). Overall variability is divided into several components: a component attributable to the main effect of each factor and another one attributable to the interaction between different factors. Percentage of variation of the response (Variation, %), explained by the contribution of each factor and interaction, as the percentage of the F-ratio of each factor relative to the sum of all F-ratios.|
|Cha (pg cell−1)||Variation (%)||61.52||27.08||6.86||2.35||(-)||2.18|
|Chc (pg cell−1)||Variation (%)||64.33||24.68||6.34||0.84||(-)||0.67|
|Pe (pg cell−1)||Variation (%)||68.09||15.01||6.77||5.65||(-)||4.46|
|Dd (pg cell−1)||Variation (%)||65.36||18.06||11.09||4.67||(-)||0.79|
|Dn (pg cell−1)||Variation (%)||17.64||52.24||4.27||16.85||(-)||8.97|
|OA (pg·cell−1)||Variation (%)||79.02||16.94||(-)||4.04||(-)||(-)|
|OA (ng·mL−1)||Variation (%)||98.92||1.084||(-)||0.48||(-)||(-)|
Microalgal cultures with Fv/Fm values ranging from 0.6 for cyanobacteria to 0.8 for green algae are generally considered healthy by algologists. Although to date there is no established consensus about dinoflagellates, Fv/Fm values of around 0.6 also seem to be indicative of healthy cells (see Figure 4). Depending on the growth conditions, Fv/Fm can vary significantly during cultivation. Hence a decline in Fv/Fm from optimal values represents a reliable warning indicator for preventing or treating stressed microalgal culture as reported elsewhere . Dinoflagellates can also experience sharp declines in Fv/Fm under prolonged exposure to thermal and/or light stress [34,35,36]. P. belizeanum showed a similar behavior, as Figure 6 shows. In the severely photoinhibited and thermally stressed culture (28 °C and 120 µE·m−2·s−1), Fv/Fm markedly decreased from 0.65 for unstressed conditions at the beginning of the culture, to below 0.3 after 10 days of culture, indicating a strong photoinactivation of the PSII. Fv/Fm in the culture under optimal T and I0 (25 °C and 40 µE·m−2·s−1) showed consistent values from 0.6 to 0.7 by contrast. In the culture moderately photoinhibited (T = 28 °C and 80 µE·m−2·s−1), Fv/Fm only began to significantly decline from day 10.
The analysis of the results presented in this section showed that the Fv/Fm measurements are an appropriate indicator of the PSII photochemical yield and can be used to monitor the physiological state of adherent cell cultures of the benthic dinoflagellate P. belizeanum.
2.3. Synthesis of Pigments
Figure 7 shows a representative chromatogram of the pigment profile of P. belizeanum measured by high performance liquid chromatography (HPLC) in the culture used as inoculum. The following pigments were identified in P. belizeanum cells: chlorophyll a (Chl a) chlorophyll c (Chl c), β-carotene, diadinoxanthin (Dd), peridinin (Pe) and dinoxanthin (Dn). As the β-carotene concentration in the cells was always very low and was not detected in most of the chromatograms, it was excluded from the next analysis.
The abundance of carotenoid pigments (Dn, Dd and Pe) for different species of the genus Prorocentrum, expressed as molar ratios with respect to Chl a, are compared in Table 4. In general, intervals of variation of these ratios obtained in this study for P. belizeanum were consistent with the values reported for other species of the same genus, though some of the maximum and minimum values for P. belizeanum were slightly higher and lower, respectively. This was likely due to the different aforementioned stressful T-I0 combinations that could give rise to marked changes in pigment cellular content, as will be discussed below.
|Table 4. Intervals of variation of molar pigment ratios to Chl a in the genus Prorocentrum extracted from  for comparison with those observed in our study for P. belizeanum.|
|Ratios||Level||From ||Our study|
|Perid/chl c||Max||P. levis||38.92||P. belizeanum||43.80|
|Perid/chl a||Max||P. rostratum||1.69||2.08|
|Chl c/chl a||Max||P .nux||0.43||0.19|
|Diadino/chl a||Max||P. lima||1.09||1.36|
|Dino/chl a||Max||P. lima||0.3||3.70|
Table 3 presents results of a multifactor ANOVA carried out with all the pigment data measured during culture. Temperature was responsible for most of the variation observed in the pigment profile of P. belizeanum, while the influence of I0 was smaller. The interaction T-I0 only had a statistically significant effect (p < 0.05) on Dn, but its contribution to the overall variation of intracellular pigments was considerably inferior to the sum of T and I0 single factors. The remaining interactions were not significant.
Figure 8 shows the mean cellular content of each pigment, provided by the ANOVA, as a function of T and I0. Photolimited cells (<40 µE·m−2·s−1) strongly increased the content of light-harvesting pigments such as chlorophylls and peridinin (p < 0.05) in relation to photoinhibited cells (120 µE·m−2·s−1). The most visible change was the darkening of cells, which is observed in all photosynthetic microalgae grown under dim light . The same pigments decreased under high irradiance, resulting in cells being rather transparent. The opposite was observed with the photoprotective pigments of the xanthophyll cycle (i.e., diadinoxanthin and dinoxanthin). Although I0 had no statistically significant influence on Dd, the pool of Dn + Dd did increase when cells were exposed to high irradiance levels. This augmentation was concomitant with the drop in Fv/Fm at irradiances above 40 µE·m−2·s−1 (see Figure 4). This pattern is part of a vital mechanism of coping with excess irradiance by phototrophs that have been extensively described in microalgae over recent decades and is consistent with our results. Xanthophyll-cycle pigments are accumulated by the cells to increase thermal energy dissipation as photon harvesting rates exceed those required in photochemistry.
There are numerous studies, particularly with dinoflagellates, concerning the effect of temperature on the synthesis of pigments in microalgal cells [39,40,41,42,43,44]. In our study, P. belizeanum increased its content of chlorophylls and carotenoids with temperatures up to 25 °C (Figure 8c,d). Dn quota continued to grow up to 28 °C (p < 0.05), but peridinin and diadinoxanthin were exceptions under thermal stress at 28 °C. Their content decreased significantly (p < 0.05), though always maintaining a value above that registered at the lowest temperature assayed (18 °C). The tendency of chlorophylls is in accordance with results previously reported for several microalgal species [39,40,41,42,43], suggesting a common pattern of decrease in maximum rate of energy consumption with increasing temperature, as indicated by Carvalho et al., . The tendency of the carotenoids may be partially explained by reactive oxygen species (ROS)-mediated stimulation of carotenogenesis as reported with Haematococcus spp . However, the decrease in Dd at the highest temperature (28 °C) is a particular phenomenon, which is only observable, as far as we know, in a few species of symbiotic dinoflagellates . The fundamentals lies on that an excessive ROS production due to elevated temperature, with or without high irradiance, may trigger the selective destruction of photosynthetic pigments by photo/thermal oxidative processes in symbiotic dinoflagellates [46,47]. Thus, the dinoflagellate Symbiodinium is able to interconvert the pigments Dd and diatoxanthin (Dt) as part of a photoprotection process, which is vital to the prevention of ROS overproduction . More recently, it was observed in several symbiotic algae that elevated temperature/irradiance caused increased levels of Dt in relation to the Dd + Dt pool due to the preferential destruction of Dd, without a significant impact on chlorophyll a . In our results, the role of dinoxanthin (Dn) in P. belizeanum at 28 °C (see Figure 8c,d) seems to match that of the diatoxanthin in other dinoflagellates . Further research is, nevertheless, required in order to clarify this issue fully in non-symbiotic dinoflagellates.
2.4. Okadaic Acid Production
OA and analogues are secondary metabolites and therefore their synthesis is completely uncoupled from cell growth. They are mainly accumulated under long-term starvation. For this reason, determination of OA in cells was carried out in the stationary phase of growth. Cellular content of OA and its concentration in the broth were accordingly calculated and a multifactor ANOVA was performed (see Table 3). Temperature had a statistically significant effect on both OA cell content and concentration (p < 0.05), whereas the effect of irradiance on these responses was much less, proving irrelevant for OA concentration.
Figure 9 shows the mean OA cellular content and OA titer values reached for each T and I0 and the intervals around each mean value. Inspection of Figure 9a indicates minimal accumulation of OA in cells at the optimal growth temperature, and maximum accumulation at the lowest temperature. According to Figure 9b, only the lowest I0 had a statistically significant influence on OA content in cells. On the other hand, the OA titer in the broth dropped abruptly with the temperature (see Figure 9c). Thus, the maximum values of 6.85 ± 0.61 ng cell−1 and 419.0 ± 12.2 ng mL−1 for OA content per cell and OA titer, respectively, were obtained at 18 °C and 20 µE·m−2·s−1 (data not shown). OA production in P. belizeanum seems to be a response to stressful environmental conditions, as the OA content increased in two different circumstances: (i) with both low T and low I0, when growth is limited; and (ii) with high T, when growth is strongly inhibited. Presumably, synthesis of OA and other toxins in dinoflagellates may be an innate defence mechanism to suppress the growth of potential competitors , which is accentuated when growth is acutely stressed.
The above-described pattern partially resembles the observations reported for other species of the genus Prorocentrum . Apparently, P. belizeanum produced less OA than others of the same genus. OA cellular contents have been reported to range from 0.5 pg cell−1 to 192 pg cell−1, though large variability due to environmental factors is reported . However, the importance of this strain does not lie solely in the production of OA; OA analogues (lipophilic dinophysistoxins (DTX1–3) and the water-soluble derivatives (DTX4 and DTX5a–c)) and linear polycyclic compounds and macrolides (e.g., corozalic acid, belizeanolide, belizeanic acid) are also of great interest [7,8,9,10,11,12]. Unfortunately, the monitoring of the synthesis of these metabolites in culture is not possible, since the corresponding reference standards are not commercially available, and/or a routine laboratory-scale methodology for determining them has not been reported. Meanwhile, the determination of OA can serve as a reference for the other analogues and polyketides. The rationale for this lies in recent evidence, comprehensively reported by Hu (2010), on the biosynthetic origin and bioactivity of OA analogues . Although different Prorocentrum species can produce a great variety of different OA derivatives with different substituents or conformational change on their skeleton , these toxins seem to be biosynthesized via a polyketide pathway shared with OA. Therefore, the more than forty compounds identified to date from a reduced number of species of the genus Prorocentrum  may be indirectly monitored in culture through the determination of OA. This approach would have a clear benefit, since it would allow the planning of inexpensive experiments aimed to optimize culture conditions for enhancing the production of the toxins. Large-scale cultures could then be designed to obtain sufficient amounts of compound to carry out all the necessary studies. Nonetheless, a possible metabolic inter-conversion between toxins due to the effect of culture conditions should be taken into account in subsequent studies, because it can induce different ratios of OA and other analogues. This was the case of Prorocentrum lima with OA and methyl-okadaic acid .
2.5. Implications in Massive Culture
Dinoflagellates and their toxins are generally hazardous if inhaled or ingested. Safety issues merit special attention when producing dinoflagellates and toxins thereof, even more so as the scale of operation increases. A comprehensive safety management plan is necessary for any commercial facility producing or processing biotoxins . If producer species are photosynthetic, the costs of implementation of that plan can be greatly reduced because they may be grown in closed photobioreactors under outdoor conditions. However, excessive irradiance can be detrimental for cells.
At irradiances beyond the maximum regions represented in Figure 3a and Figure 4a, PSII can be strongly photoinhibited, so bioproductivity will decrease rapidly as I0 is further raised. Therefore the previous determination of the photoinhibition threshold of any photosynthetic microalgal species is crucial to the reliable design of an outdoor culture system. The tolerance to light flux of P. belizeanum was extremely low (around 50 µE·m−2·s−1), indicating that it is a light-sensitive species. Other microalgal species successfully grown in outdoor conditions could stand the local irradiance levels that occur in moderately sunny areas of the planet (e.g., up to 3000 µE·m−2·s−1 in Southeast Spain). Consequently, photobioreactors for growing them must be modified accordingly to prevent photoinhibition and to optimize the photosynthetic efficiency of the cells. Among the diverse strategies that may be devised to address this issue, the following may be mentioned aimed at attenuating the incident radiation on the surface of the photobioreactor: (i) covering the photobioreactor with meshes of different density depending on the degree of required illumination reduction; (ii) using dyed material for the construction of the photobioreactor (dyes should be carefully selected to avoid distortions in the spectrum of the photosynthetically active radiation (PAR)); or (iii) increasing the height of the column of water that circulates over the surface where the cells are attached. Not all dinoflagellates are equally sensitive to light; intra- and inter-specific differences exist [5,51]. Therefore, if a product can be sourced from multiple species, the selection of a more resistant species to outdoor culture conditions may have important advantages for large-scale production. Enhancements in the concentration of a target compound may also be made by improving the producer strain through genetic modification. Unfortunately, the molecular genetics of the biosynthesis of dinoflagellate toxins is poorly understood, though progress is being made and discussed .
According to the results presented here, synthesis of OA (and probably derivates thereof) in P. belizeanum seems to be stimulated under stressful temperature and/or illumination conditions. In a hypothetical outdoor culture, cells would be exposed to daily changes in irradiance and temperature. By properly controlling these two factors over time, we may culture P. belizeanum in a two-step process to increase the OA yield (i.e., cyclically alternating a period of optimal culture conditions with one of stressful conditions in which a part of the biomass is harvested to recover OA and the other is left in the photobiorreactor to begin a new cycle). Figure 10 shows photographs of a rudimentary bench-scale outdoor culture with P. belizeanum operated in batch mode. The culture system consisted of plastic bags covered by a mesh during the midday to reduce the irradiance at the surface of the culture to below 80 µE·m−2·s−1. Temperature was controlled around 18 °C. Outdoor culture reached 25,000 cells·mL−1 after 10 days. The results were consistent with the experiments performed in T-flask at the same temperature and similar irradiance (see Figure 1d). From that day, the culture was partially uncovered, reaching irradiance levels of up to 320 µE·m−2·s−1 on the bag surface. The cells were strongly photoinhibited and in the course of the next 10 days over 50% of the cells died.
3. Experimental Section
3.1. Species Selected
The strain used in this study was a clone of the photosynthetic toxic benthic dinoflagellate Prorocentrum belizeanum (VGO1029), kindly donated by the Culture Collection of Harmful Microalgae of IEO (Vigo, Spain) and already adapted to grow in L1 medium. P. belizeanum is commonly associated with floating detritus and sediments in tropical bays of the Caribbean Sea . P. belizeanum is a known producer of okadaic acid and derivatives thereof [8,11], dinophysistoxin-1  and cytotoxic macrolides .
3.2. Culture and Growth Kinetics
Basal inocula were grown under a 12:12-h light-dark cycle (100 μEm−2s−1) at 18 ± 1 °C. Filter sterilized (0.22 mm Millipore filter; Millipore Corporation, Billerica, MA, USA) L1 medium  prepared in natural Mediterranean Sea water (conductivity around 55,000 µS/cm) was used in all experiments. Preliminary experiments showed that reproducible and consistent growth occurred when cultures were maintained in vented polystyrene tissue culture T-flasks with vent/close cap (Nunclon® Δ surface treatment). As P. belizeanum is a benthic dinoflagellate microalga, cells grew forming numerous lumps consisting of dozens of cells that adhered to the T-flask bottom. In addition, cells secreted an extracellular mucus that covered the bottom forming a thin transparent layer. Cell confluence was not observed in any experiment. Culture T-flasks were horizontally located on an incubator tray and illuminated overhead by a bank of cool daylight fluorescent tubes (Philips TL40W). T-flasks of parallelepipedal geometry (see Figure 11a) were chosen because of the ease in the evaluation of the light field inside the cultures as reported elsewhere . The fixed culture volume (15 mL) provided a high surface to volume ratio, and thus a relatively low culture thickness. It is a relevant issue to be tackled prior to planning experiments for obtaining growth curves as a function of irradiance. Many factors, such as light scattering effects and/or mutual shading (when cells close to the illuminated surface intercept more light that they can use, and thereby shade algae deeper in the culture), may lead to a misevaluation of the effect of irradiance due to overestimation of the light available to cells. One way to avoid or mitigate this phenomenon is to work with optically thin cultures with minimum mutual shading. Our cultures fulfilled this condition because they had a high surface to volume ratio that provided a short light path (L) through the cultures. The rationale of this is based on the following analysis. Since the attenuation of any given light beam traveling through the medium can be calculated by the Lambert-Beer’s law , irradiance at any inner point separated by distance x from the culture surface (see Figure 2a) is obtained as:
Four irradiance levels (20, 40, 80, and 120 µE·m−2·s−1) at three temperatures (18, 25, and 28 °C) were assayed. Cultures were inoculated into 25 cm2 T-flasks containing 15 mL of L1 medium. The light:dark cycle and light source were the same as those described above for the inocula. To minimize undesirable effects on growth kinetics and toxin production due to possible photo- and thermo-acclimation phenomena in the inoculum, cultures were pre-acclimated to every experimental I0-T combination by repeatedly subculturing over a period of 4 weeks. All T-flasks were placed in an incubator as shown in Figure 11b. The walls were painted black to avoid reflections of the light that might modify the irradiance distribution on the surface of the cultures and thereby the illumination field in the cultures. The different irradiance levels were provided by varying the distance from the T-flask surface to the light source. Irradiance was measured with a 4π sensor (Biospherical instruments Inc., mod. QSL-100, San Diego, CA, USA). Experiments were carried out in duplicate.
Growth was measured by cell counts. For sampling, the cells were gently detached with cell scrapers to prevent cell breakage. The culture was then mildly agitated by hand to distribute uniformly cells in the culture. Afterwards, 1-mL samples were collected daily, fixed with lugol’s solution (L6146, Sigma-Aldrich, Co., Saint Louis, MO, USA), and the cells were counted on a Sedgewick-Rafter counting slide. This sampling technique was the least invasive of all tested. In fact, the cultures returned to the same original appearance hours later (data not shown).
The batch cultures of P. belizeanum exhibited asymmetric growth curves, i.e., a sharp decline in cell density was observed following the stationary phase. As this behavior cannot be described by the standard (symmetric) logistic equations, the following asymmetric logistic equation (ALE) was used to model cell concentration versus culture time data. In this way the corresponding specific growth rates were easily obtained by analytical differentiation of the ALE:
A previous discrimination analysis of equations using the F-test proved that the fits of Equations (2) and (3) were statistically superior to the ones with other equations at the 95% confidence level.
3.3. Modelling of Growth
The following mechanistic model of photosynthesis in microalgae (P-I curve) proposed by Camacho et al. (2003)  for nutrient-replete cells has been used to model the effect of the irradiance:
The effect of the temperature (T) on microalgal growth has been simulated with the following empirical equation, not based on the Arrhenius equation, recently proposed by Huang et al. (2011)  for descriptive microbiology:
3.4. Measurements of the Chlorophyll Fluorescence
Long-term kinetics of chlorophyll fluorescence in P. belizeanum were recorded with a pulse amplitude modulation (PAM) chlorophyll fluorometer (Mini-PAM-2500). All samples were kept in darkness for 30 min before measurements in order to determine photosynthetic parameters in a dark-adapted state. The initial fluorescence (F0) was measured by exposing cells to a red light weak pulse (<1 μEm−2s−1). Maximum fluorescence (Fm) was then quantified by applying a saturating light pulse (8000 μEm−2s−1; 800 ms pulse-width). The maximum variable fluorescence was calculated as Fv = Fm − F0. The Fv/Fm ratio, designated as the maximum photochemical yield of the photosystem II (PSII), is unanimously considered an indicator of cell stress since it represents the performance of photochemical processes in the PSII.
3.5. Outdoor Cultures
A bench-scale outdoor photobioreactor was custom built to a design based on previous experience with the T-flasks. The bioreactor was made with custom-made polyethylene bags (32 cm × 65 cm), which were introduced in parallelipepidal structure containing water. The culture temperature was controlled at 19 ± 1 °C by circulating thermostated water. The working volume was 18 L. The photosynthetically active irradiance on the surface of the photobioreactor and in the centre of the bag was measured using a QSL-100 quantum scalar irradiance sensor (Biospherical Instruments, San Diego, CA, USA). To reduce incident irradiance, the photobioreactor was covered with white fabric. Thus, irradiance on the bag surface ranged from 80 to 320 µE·m−2·s−1. Bags were partially sterilized using a microwave oven (2 min, 800 W). The reactor was then filled with the L1 medium made in filter sterilized Mediterranean Sea water. Inoculum was in the late exponential growth phase. The cell concentration in the freshly inoculated bioreactor was about 10,000 cells mL−1, and the photobioreactor was operated in batch mode.
3.6. Identification and Quantification of Pigments
Cell-free methanol extracts were obtained from culture samples as described elsewhere . Detection of pigments in methanol:H20 (9:1) extracts was performed by HPLC with a diode array detector as described in  using a Shimadzu SPD-M10AV high-performance liquid chromatograph (Shimadzu Corporation, Kyoto, Japan). Separation was performed on a Lichrosphere RP-18 5 μm column (4.6 × 150 mm). The eluents used were (A) water/methanol (2:8, v/v) and (B) acetone/methanol (1:1, v/v). The pigments were eluted at a rate of 1 mL/min and detected by measuring absorbance at 360–700 nm using a diode array detector. Standards of β-carotene and chloropyll a were provided by Sigma Chemical Co. (St. Louis, MO, USA), and peridinin, diadinoxanthin and dinoxanthin were from DHI Water & Environment (Horsholm, Denmark). Chlorophyll c content was determined by Hansmann’s spectrometric method  and using Parsons and Strickland’s equations for the quantification .
3.7. Determination of OA Concentration
Okadaic acid was measured separately in the biomass and in the culture supernatant following the method of Kelly et al., . OA was recovered from samples by chromatography on silica (Sep-pak Plus C18. Waters, Milford, MA, USA) for the biomass extracts (MeOH) and Diaion® HP-20 (glass columns packed with 500 mg of HP-20 from Supelco) for supernatants. Using 1-bromoacetylpyrene (BAP), as derivatization reagent, the OA was determined by HPLC with fluorimetric detection. An HPLC system (Shimadzu AV10; Shimadzu Corporation, Kyoto, Japan) with a fluorescence detector (Shimadzu RF-10AX), an auto-injector (Shimadzu SIL-10ADVP) and a SupelcosilTM LC-18 column (25 cm × 4.6 mm, 5 µm. Supelco) were used. The reference standard used was okadaic acid sodium salt (sodium okadate) provided by CIFGA (Cifga S.A., Lugo, Spain).
3.8. Statistical Analyses
Nonlinear regression to fit specific growth rate data to Equations (4) and (5), and multifactor ANOVA tests were conducted in STATGRAPHICS Centurion software package (StatPoint, Herndon, VA, USA).
This study has demonstrated that the benthic dinoflagellate P. belizeanum is a moderately mesophilic and extremely light-sensitive species. Cells showed a pronounced up-regulation of the pool of protective pigments of the xanthophyll cycle (diadinoxanthin and dinoxanthin) to dissipate excessive photonic energy as heat. Furthermore, P. belizeanum also reduced the content of peridinin, a light-harvesting pigment, at high irradiance/temperature; likely cells tried to minimize excessive light-absorption under stressful environmental conditions. However, these mechanisms of photoprotection were insufficient to prevent apparent photoinhibition above 40 µE·m−2·s−1 and thermal stress at 28 °C. A continuous sharp drop in Fv/Fm during culture was the prelude to this metabolic response, which finally led to death of the culture under the most stressful T-I0 combination (120 µE·m−2·s−1 and 28 °C). Chlorophyll a fluorescence thus represents a powerful technique, which allows rapid monitoring of physiological status in dinoflagellate culture, but always accompanied by other cellular responses (e.g., pigment profile).
T-flask culture observations were consistent with preliminary assays carried out in outdoor conditions, reinforcing the above-mentioned considerations to be taken into account before a hypothetical mass cultivation of this species. OA overproduction was a consequence of stressful environmental conditions owing to the combination of low temperature and irradiance, or due to high temperature alone.
This research was funded by the Spanish Ministry of Education and Science (SAF2011-28883-C03-02), the General Secretariat of Universities, Research and Technology of Andalusian Government (TEP-5375) and the European Regional Development Fund Program. Lorenzo López Rosales is grateful for personal funding through the PPI of the University of Almería (Spain). The strains used were kindly donated by Santiago Fraga (Culture Collection of Harmful Microalgae of IEO, Vigo, Spain).
Conflicts of Interest
The authors declare no conflict of interest.
- Camacho, F.G.; Rodríguez, J.G.; Mirón, A.S.; García, M.C.C.; Belarbi, E.H.; Chisti, Y.; Grima, E.M. Biotechnological significance of toxic marine dinoflagellates. Biotechnol. Adv. 2007, 25, 176–194, doi:10.1016/j.biotechadv.2006.11.008.
- Glaser, K.B.; Mayer, A.M.S. A renaissance in marine pharmacology: From preclinical curiosity to clinical reality. Biochem. Pharmacol. 2009, 78, 440–448, doi:10.1016/j.bcp.2009.04.015.
- Gallardo-Rodríguez, J.; Sánchez-Mirón, A.; García-Camacho, F.; López-Rosales, L.; Chisti, Y.; Molina-Grima, E. Bioactives from microalgal dinoflagellates. Biotechnol. Adv. 2012, 30, 1673–1684, doi:10.1016/j.biotechadv.2012.07.005.
- Shimizu, Y. Microalgal metabolites: A new perspective. Annu. Rev. Microbiol. 1996, 50, 431–465, doi:10.1146/annurev.micro.50.1.431.
- Xu, N.; Duan, S.; Li, A.; Zhang, C.; Cai, Z.; Hu, Z. Effects of temperature, salinity and irradiance on the growth of the harmful dinoflagellate Prorocentrum donghaiense lu. Harmful Algae 2010, 9, 13–17, doi:10.1016/j.hal.2009.06.002.
- Paz, B.; Vázquez, J.A.; Riobó, P.; Franco, J.M. Study of the effect of temperature, irradiance and salinity on growth and yessotoxin production by the dinoflagellate Protoceratium reticulatum in culture by using a kinetic and factorial approach. Mar. Environ. Res. 2006, 62, 286–300, doi:10.1016/j.marenvres.2006.04.066.
- Cruz, P.G.; Daranas, A.H.; Fernández, J.J.; Souto, M.L.; Norte, M. Dtx5c, a new oa sulphate ester derivative from cultures of Prorocentrum belizeanum. Toxicon 2006, 47, 920–924, doi:10.1016/j.toxicon.2006.03.005.
- Cruz, P.G.; Fernández, J.J.; Norte, M.; Daranas, A.H. Belizeanic acid: A potent protein phosphatase 1 inhibitor belonging to the okadaic acid class, with an unusual skeleton. Chem. Eur. J. 2008, 14, 6948–6956, doi:10.1002/chem.200800593.
- Napolitano, J.G.; Norte, M.; Fernández, J.J.; Daranas, A.H. Corozalic acid: A key okadaic acid biosynthetic precursor with phosphatase inhibition activity. Chem. Eur. J. 2010, 16, 11576–11579.
- Napolitano, J.G.; Norte, M.; Padrón, J.M.; Fernández, J.J.; Hernández Daranas, A. Belizeanolide, a cytotoxic macrolide from the dinoflagellate Prorocentrum belizeanum. Angew. Chem. Int. Ed. 2009, 48, 796–799.
- Paz, B.; Daranas, A.H.; Cruz, P.G.; Franco, J.M.; Napolitano, J.G.; Norte, M.; Fernández, J.J. Identification and characterization of dtx-5c and 7-hydroxymethyl-2-methylene-octa-4,7-dienyl okadaate from Prorocentrum belizeanum cultures by lc-ms. Toxicon 2007, 50, 470–478, doi:10.1016/j.toxicon.2007.04.011.
- Paz, B.; Daranas, A.H.; Cruz, P.G.; Franco, J.M.; Norte, M.; Fernández, J.J. Identification of 19-epi-okadaic acid, a new diarrhetic shellfish poisoning toxin, by liquid chromatography with mass spectrometry detection. Mar. Drugs 2008, 6, 489–495.
- Hu, W.; Xu, J.; Sinkkonen, J.; Wu, J. Polyketides from marine dinoflagellates of the genus Prorocentrum, biosynthetic origin and bioactivity of their okadaic acid analogues. Mini-Rev. Med. Chem. 2010, 10, 51–61, doi:10.2174/138955710791112541.
- García-Camacho, F.; Sánchez-Mirón, A.; Molina-Grima, E.; Camacho-Rubio, F.; Merchuck, J.C. A mechanistic model of photosynthesis in microalgae including photoacclimation dynamics. J. Theor. Biol. 2012, 304, 1–15, doi:10.1016/j.jtbi.2012.03.021.
- Aligizaki, K.; Nikolaidis, G.; Katikou, P.; Baxevanis, A.D.; Abatzopoulos, T.J. Potentially toxic epiphytic Prorocentrum (dinophyceae) species in greek coastal waters. Harmful Algae 2009, 8, 299–311, doi:10.1016/j.hal.2008.07.002.
- Pan, Y.; Cembella, A.D.; Quilliam, M.A. Cell cycle and toxin production in the benthic dinoflagellate Prorocentrum lima. Mar. Biol. 1999, 134, 541–549, doi:10.1007/s002270050569.
- Varkitzi, I.; Pagou, K.; Granéli, E.; Hatzianestis, I.; Pyrgaki, C.; Pavlidou, A.; Montesanto, B.; Economou-Amilli, A. Unbalanced N:P ratios and nutrient stress controlling growth and toxin production of the harmful dinoflagellate Prorocentrum lima (ehrenberg) dodge. Harmful Algae 2010, 9, 304–311, doi:10.1016/j.hal.2009.12.001.
- Morton, S.L.; Faust, M.A.; Fairey, E.A.; Moeller, P.D.R. Morphology and toxicology of Prorocentrum arabianum sp. Nov., (dinophyceae) a toxic planktonic dinoflagellate from the gulf of oman, arabian sea. Harmful Algae 2002, 1, 393–400, doi:10.1016/S1568-9883(02)00047-1.
- Lawrence, J.E.; Bauder, A.G.; Quilliam, M.A.; Cembella, A.D. Prorocentrum lima: A Putative Link to Diarrhetic Shellfish Poisoning in Nova Scotia, Canada. In Harmful Algae. In Proceedings of the VIII International Conference on Harmful Algae; Reguera, B., Blanco, J., Fernández, M., Wyatt, T., Eds.; Xunta de Galicia and IOC of UNESCO: Vigo, Spain, 1998; pp. 78–79.
- Nascimento, S.M.; Purdie, D.A.; Morris, S. Morphology, toxin composition and pigment content of Prorocentrum lima strains isolated from a coastal lagoon in southern UK. Toxicon 2005, 45, 633–649, doi:10.1016/j.toxicon.2004.12.023.
- Vale, P.; Veloso, V.; Amorim, A. Toxin composition of a Prorocentrum lima strain isolated from the portuguese coast. Toxicon 2009, 54, 145–152, doi:10.1016/j.toxicon.2009.03.026.
- Morlaix, M.; Lassus, P. Nitrogen and phosphorus effects upon division rate and toxicity of Prorocentrum lima (ehrenberg) dodge. Cryptogam. Algologie 1992, 13, 187–195.
- Aikman, K.E.; Tindall, D.R.; Morton, S.L. Physiology and Potency of the Dinoflagellate Prorocentrum hoffmannianum during One Complete Growth Cycle. In Toxic Phytoplankton Blooms in the Sea; Smayda, T.J., Shimizu, Y., Eds.; Elsevier: New York, NY, USA, 1993; pp. 463–468.
- Morton, S.L.; Norris, D.R. Role of Temperature, Salinity, and Light on the Seasonality of Prorocentrum lima (Ehrenberg) Dodge. In Toxic Marine Phytoplankton; Graneli, E., Sundstron, B., Edler, D., Anderson, D.M., Eds.; Elsevier: New York, NY, USA, 1990; pp. 201–205.
- Morton, S.L.; Norris, D.R.; Bomber, J.W. Effect of temperature, salinity and light intensity on the growth and seasonality of toxic dinoflagellates associated with ciguatera. J. Exp. Mar. Biol. Ecol. 1992, 157, 79–90, doi:10.1016/0022-0981(92)90076-M.
- Borowitzka, M. Wastewater Treatment with Algae. In Limits to Growth; Wong, Y., Tam, N., Eds.; Springer: Berlin, Germany, 1988; pp. 203–218.
- Rubio, F.C.; Camacho, F.G.; Sevilla, J.M.; Chisti, Y.; Grima, E.M. A mechanistic model of photosynthesis in microalgae. Biotechnol. Bioeng. 2003, 81, 459–473, doi:10.1002/bit.10492.
- Huang, L.; Hwang, C.A.; Phillips, J. Evaluating the effect of temperature on microbial growth rate-the ratkowsky and a bӗlehrádek-type models. J. Food Sci. 2011, 76, 547–557, doi:10.1111/j.1750-3841.2011.02345.x.
- Zwietering, M.H.; de Koos, J.T.; Hasenack, B.E.; de Wit, J.C.; van’t Riet, K. Modeling of bacterial growth as a function of temperature. App. Environ. Microbiol. 1991, 57, 1094–1101.
- Bernard, O.; Rémond, B. Validation of a simple model accounting for light and temperature effect on microalgal growth. Biores. Technol. 2012, 123, 520–527, doi:10.1016/j.biortech.2012.07.022.
- Baek, S.H.; Shimode, S.; Kikuchi, T. Growth of dinoflagellates, Ceratium furca and Ceratium fusus in Sagami Bay, Japan: The role of temperature, light intensity and photoperiod. Harmful Algae 2008, 7, 163–173, doi:10.1016/j.hal.2007.06.006.
- Béchet, Q.; Shilton, A.; Guieysse, B. Modeling the effects of light and temperature on algae growth: State of the art and critical assessment for productivity prediction during outdoor cultivation. Biotechnol. Adv. 2013, 31, 1648–1663, doi:10.1016/j.biotechadv.2013.08.014.
- Masojídek, J.; Vonshak, A.; Torzillo, G. Chlorophyll Fluorescence Applications in Microalgal Mass Cultures. In Chlorophyll a Fluorescence in Aquatic Sciences: Methods and Applications; Suggett, D.J., Prášil, O., Borowitzka, M.A., Eds.; Springer: Dordrecht, The Netherlanda, 2010; pp. 277–292.
- Fitt, W.K.; Warner, M.E. Bleaching patterns of four species of caribbean reef corals. Biol. Bull. 1995, 189, 298–307, doi:10.2307/1542147.
- Warner, M.E.; Fitt, W.K.; Schmidt, G.W. The effects of elevated temperature on the photosynthetic efficiency of zooxanthellae in hospite from four different species of reef coral: A novel approach. Plant Cell Environ. 1996, 19, 291–299, doi:10.1111/j.1365-3040.1996.tb00251.x.
- Franklin, D.J.; Hoegh-Guldberg, O.; Jones, R.J.; Berges, J.A. Cell death and degeneration in the symbiotic dinoflagellates of the coral stylophora pistillata during bleaching. Mar. Ecol. Prog. Ser. 2004, 272, 117–130, doi:10.3354/meps272117.
- Zapata, M.; Fraga, S.; Rodríguez, F.; Garrido, J.L. Pigment-based chloroplast types in dinoflagellates. Mar. Ecol. Prog. Ser. 2012, 465, 33–52, doi:10.3354/meps09879.
- Dubinsky, Z.; Stambler, N. Photoacclimation processes in phytoplankton: Mechanisms, consequences, and applications. Aquat. Microb. Ecol. 2009, 56, 163–176, doi:10.3354/ame01345.
- Thompson, P.A.; Guo, M.X.; Harrison, P.J. Effects of variation in temperature. I. On the biochemical composition of eight species of marine phytoplankton1. J. Phycol. 1992, 28, 481–488.
- Sukenik, A.; Zmora, O.; Carmeli, Y. Biochemical quality of marine unicellular algae with special emphasis on lipid composition. Ii. Nannochloropsis sp. Aquaculture 1993, 117, 313–326, doi:10.1016/0044-8486(93)90328-V.
- Del Campo, J.A.; Moreno, J.; Rodrı́guez, H.; Angeles Vargas, M.; Rivas, J.; Guerrero, M.G. Carotenoid content of chlorophycean microalgae: Factors determining lutein accumulation in Muriellopsis sp. (chlorophyta). J. Biotechnol. 2000, 76, 51–59, doi:10.1016/S0168-1656(99)00178-9.
- Borowitzka, M. Vitamins and Fine Chemicals from Micro-Algae. In Micro-Algal Biotechnology; Borowitzka, M., Borowitzka, L., Eds.; Cambridge University Press: Cambridge, UK, 1988; pp. 153–196.
- Carvalho, A.P.; Monteiro, C.M.; Malcata, F.X. Simultaneous effect of irradiance and temperature on biochemical composition of the microalga Pavlova lutheri. J. App. Phycol. 2009, 21, 543–552, doi:10.1007/s10811-009-9415-z.
- Venn, A.A.; Wilson, M.A.; Trapido-Rosenthal, H.G.; Keely, B.J.; Douglas, A.E. The impact of coral bleaching on the pigment profile of the symbiotic alga, Symbiodinium. Plant Cell Environ. 2006, 29, 2133–2142, doi:10.1111/j.1365-3040.2006.001587.x.
- Morton, S.L.; Moeller, P.D.R.; Young, K.A.; Lanoue, B. Okadaic acid production from the marine dinoflagellate Prorocentrum belizeanum faust isolated from the belizean coral reef ecosystem. Toxicon 1998, 36, 201–206, doi:10.1016/S0041-0101(97)00054-8.
- Tchernov, D.; Gorbunov, M.Y.; de Vargas, C.; Yadav, S.N.; Milligan, A.J.; Häggblom, M.; Falkowski, P.G. Membrane lipids of symbiotic algae are diagnostic of sensitivity to thermal bleaching in corals. Proc. Natl Acad. Sci. USA 2004, 101, 13531–13535, doi:10.1073/pnas.0402907101.
- Ledford, H.K.; Niyogi, K.K. Singlet oxygen and photo-oxidative stress management in plants and algae. Plant Cell Environ. 2005, 28, 1037–1045, doi:10.1111/j.1365-3040.2005.01374.x.
- Brown, B.; Downs, C.; Dunne, R.; Gibb, S. Preliminary evidence for tissue retraction as a factor in photoprotection of corals incapable of xanthophyll cycling. J. Exp. Mar. Biol. Ecol. 2002, 277, 129–144, doi:10.1016/S0022-0981(02)00305-2.
- Poulson, K.L.; Sieg, R.D.; Prince, E.K.; Kubanek, J. Allelopathic compounds of a red tide dinoflagellate have species-specific and context-dependent impacts on phytoplankton. Mar. Ecol. Prog. Ser. 2010, 416, 69–78, doi:10.3354/meps08788.
- Morton, S.L.; Bomber, J.W.; Tindall, P.M. Environmental effects on the production of okadaic acid from Prorocentrum hoffmannianum faust i. Temperature, light, and salinity. J. Exp. Mar. Biol. Ecol. 1994, 178, 67–77, doi:10.1016/0022-0981(94)90225-9.
- Grzebyk, D.; Berland, B. Influences of temperature, salinity and irradiance on growth of Prorocentrum minimum (dinophyceae) from the mediterranean sea. J. Plankton Res. 1996, 18, 1837–1849, doi:10.1093/plankt/18.10.1837.
- Guillard, R.R.L.; Hargraves, P.E. Stichochrysis immobilis is a diatom, not a chrysophyte. Phycologia 1993, 32, 234–236, doi:10.2216/i0031-8884-32-3-234.1.
- Grima, E.M.; Camacho, F.G.; Pérez, J.A.S.; Fernéndez, F.G.A.; Sevilla, J.M.F. Evaluation of photosynthetic efficiency in microalgal cultures using averaged irradiance. Enzyme Microb. Technol. 1997, 21, 375–381, doi:10.1016/S0141-0229(97)00012-4.
- Acosta, M.L.; Sánchez, A.; García, F.; Contreras, A.; Molina, E. Analysis of kinetic, stoichiometry and regulation of glucose and glutamine metabolism in hybridoma batch cultures using logistic equations. Cytotechnology 2007, 54, 189–200, doi:10.1007/s10616-007-9089-9.
- Rodríguez, J.J.G.; Mirón, A.S.; Camacho, F.G.; García, M.C.C.; Belarbi, E.H.; Chisti, Y.; Grima, E.M. Causes of shear sensitivity of the toxic dinoflagellate Protoceratium reticulatum. Biotechnol. Prog. 2009, 25, 792–800, doi:10.1002/btpr.161.
- Cerón, M.C.; Campos, I.; Sánchez, J.F.; Acién, F.G.; Molina, E.; Fernández-Sevilla, J.M. Recovery of lutein from microalgae biomass: Development of a process for Scenedesmus almeriensis biomass. J. Agric. Food Chem. 2008, 56, 11761–11766.
- Hansmann, E. Pigment Analysis. In Handbook of Phycological Methods: Culture Methods and Growth Measurements; Stein, J.R., Ed.; Cambridge University Press: London, UK, 1973.
- Strickland, J.D.H.; Parsons, T.R. A Practical Handbook of Seawater Analysis; Fisheries Research Board of Canada: Ottawa, Canada, 1972; p. 167.
- Kelly, S.S.; Bishop, A.G.; Carmody, E.P.; James, K.J. Isolation of dinophysistoxin-2 and the high-performance liquid chromatographic analysis of diarrhetic shellfish toxins using derivatisation with 1-bromoacetylpyrene. J. Chromatogr. A 1996, 749, 33–40, doi:10.1016/0021-9673(96)00448-7.
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