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A Less Saline Baltic Sea Promotes Cyanobacterial Growth, Hampers Intracellular Microcystin Production, and Leads to Strain-Specific Differences in Allelopathy

  • Andreas Brutemark ,

    Current address: Calluna AB, Stockholm, Sweden

    Affiliations ARONIA Coastal Zone Research Team, Novia University of Applied Sciences & Åbo Akademi University, Ekenäs, Finland, Tvärminne Zoological Station, University of Helsinki, Hanko, Finland

  • Angélique Vandelannoote,

    Current address: Ghent University, Kortrijk, Belgium

    Affiliation Marine Research Centre, Finnish Environment Institute SYKE, Helsinki, Finland

  • Jonna Engström-Öst,

    Affiliations ARONIA Coastal Zone Research Team, Novia University of Applied Sciences & Åbo Akademi University, Ekenäs, Finland, Tvärminne Zoological Station, University of Helsinki, Hanko, Finland

  • Sanna Suikkanen

    Affiliation Marine Research Centre, Finnish Environment Institute SYKE, Helsinki, Finland


Salinity is one of the main factors that explain the distribution of species in the Baltic Sea. Increased precipitation and consequent increase in freshwater inflow is predicted to decrease salinity in some areas of the Baltic Sea. Clearly such changes may have profound effects on the organisms living there. Here we investigate the response of the commonly occurring cyanobacterium Dolichospermum spp. to three salinities, 0, 3 and 6. For the three strains tested we recorded growth, intracellular toxicity (microcystin) and allelopathic properties. We show that Dolichospermum can grow in all the three salinities tested with highest growth rates in the lowest salinity. All strains showed allelopathic potential and it differed significantly between strains and salinities, but was highest in the intermediate salinity and lowest in freshwater. Intracellular toxin concentration was highest in salinity 6. In addition, based on monitoring data from the northern Baltic Proper and the Gulf of Finland, we show that salinity has decreased, while Dolichospermum spp. biomass has increased between 1979 and 2013. Thus, based on our experimental findings it is evident that salinity plays a large role in Dolichospermum growth, allelopathic properties and toxicity. In combination with our long-term data analyses, we conclude that decreasing salinity is likely to result in a more favourable environment for Dolichospermum spp. in some areas of the Baltic Sea.


The Baltic Sea is one of the largest brackish water basins on earth and has a wide range in salinity. Surface salinity decreases from south to north and varies from ~23 in the Kattegat, 9 in southern Baltic Proper to <1 in the eastern parts of the Gulf of Finland and the northern parts of the Bothnian Bay. It is expected that river runoff and precipitation will increase with climate change in the drainage area, and thereby increase the freshwater inflow to the Baltic Sea [1,2]. Further, there is a substantial annual variation in the amount of saline water entering the Baltic Sea [3]. As a result of the combined effects of decreasing inflow of saline water into the Baltic Sea via the Danish Straits, and increasing freshwater inputs, a decreasing salinity trend has been observed for some Baltic Sea basins [4,5,6,7].

The summer in the Baltic Sea is characterized by cyanobacterial mass occurrences, consisting mainly of three filamentous diazotrophic taxa: Aphanizomenon sp., Nodularia spumigena and Dolichospermum spp. (ex. Anabaena spp. [8]). N. spumigena produces the hepatotoxin nodularin that affects aquatic organisms, causes poisonings of domestic animals as well as wildlife, and can pose a hazard for human health [9,10]. Aphanizomenon sp. and Dolichospermum spp. are known to produce toxins in freshwaters [11] and more recently, Dolichospermum has occasionally proven to be hepatotoxic in the Baltic Sea, producing microcystins [12,13].

The role of toxins is debated, but the production of chemical compounds to kill or limit growth of competitors may be of competitive advantage to phytoplankton under certain environmental conditions [14]. Allelopathy, defined by the International Allelopathy Society (as in [15]) as”any process involving secondary metabolites produced by plants, microorganisms, viruses and fungi that influence the growth and development of agricultural and biological systems”, seems to be common for many groups of phytoplankton, including chlorophytes, diatoms, dinoflagellates, haptophytes, raphidophytes, and cyanobacteria (see reviews by [14,15]). Both biotic and abiotic factors, including the species involved and their density, growth phase, nutrient concentrations, pH, light intensity, and temperature have been suggested to affect the allelopathic potency (reviewed by [15]).

The role of salinity in the production of cyanobacterial toxins and/or allelopathic compounds is largely unknown. The levels of nodularin increased with increasing salinity for the Baltic N. spumigena [16], whereas Blackburn et al. [17] found an opposite effect; toxin content decreased in Australian N. spumigena with rising salinity. In the experiment by Lehtimäki et al. [18], N. spumigena toxin levels were highest in the salinity range 5–20 compared with higher and lower salinities. Further, Halinen et al. [12] suggested that salinity was the best explanatory factor for the presence of microcystin-producing Dolichospermum sp. in the Gulf of Finland. Toxic Dolichospermum sp. was only found in environments with low salinity [12], indicating that microcystin production was favoured in low salinities (cf. [19]). As some basins of the Baltic Sea are becoming less saline [4,5,6,7,20], we can consequently expect a change in toxicity of the phytoplankton present. Since Dolichospermum spp. are common freshwater species, a reduced salinity can promote a competitive advantage. Thus salinity can play a large role in growth and toxin production and overall fitness of Dolichospermum spp. Indeed, the northern Baltic Proper has over the last 34 years become less saline, while the biomass of cyanobacteria has increased [7]. However, little information is available concerning the allelopathic capabilities in this changing environment. The aim of this study is therefore to determine the effect of salinity on Dolichospermum spp. growth, intracellular microcystin concentrations and allelopathic properties towards a co-occurring non-toxic cryptophyte Rhinomonas nottbecki. We used salinities relevant for the Gulf of Finland—northern Baltic Proper, i.e., stretching from a freshwater environment (salinity 0), via an intermediate salinity (3), to brackish waters (6). In addition, by using long-term monitoring data for western Gulf of Finland and northern Baltic Proper, we addressed salinity and Dolichospermum spp. biomass trends from 1979 to 2013.

Materials and Methods

Ethics statement

No permits were required for the described study, and the study did not involve endangered or protected species.

Strains and cultivation

For the experiment, three different strains of Dolichospermum sp. were used: BIR250A, BIR256 and BIR257, isolated by Katrianna Halinen from the Gulf of Finland, Baltic Sea in 2004, and provided by Prof. Kaarina Sivonen (University of Helsinki). Prior to the experiment the strains were cultured for more than one year under the targeted salinity conditions (salinity 0, 3 and 6) as batch cultures at 18°C, in a 16:8 h light:dark cycle with a ~8 μmol photons m-2 s-1 light intensity using Z8 medium [21] with nitrogen omitted and NaCl added to reach the desired salinities. Salinity was continuously measured using a refractometer as well as a conductivity meter (EC300 VWR).

The cryptophyte R. nottbecki strain 07B6 (isolated from the Baltic Sea in 2007 by Dr. Anke Kremp) was grown in F/2 medium with silicate omitted [22] at 16°C and salinity 6.

Experimental design

For the growth experiment, each Dolichospermum sp. strain was cultivated in triplicate 300 mL tissue culture flasks (total culture volume 200 mL) at 18°C, in 35 μmol photons m-2 s-1 in a 14:10 h light:dark cycle. The batch culture experiment was started from a cell concentration of 70 000 cells mL-1 and growth and toxicity of the cultures were monitored for 29 days.

In mid-exponential phase (day 18–20) as well as late stationary phase (day 43), a separate experiment was conducted to study allelopathic effects of cell-free filtrates of the strains on the growth of the cryptophyte R. nottbecki. Allelopathic effects were expressed as EC50, i.e., the Dolichospermum cell concentration yielding a 50% decline in R. nottbecki fluorescence (modified from [23]). Filtrates of each of the Dolichospermum sp. strains in the different salinities were prepared using 2.0 μm polycarbonate filters (Whatman, Nuclepore). The filtrate salinity was adjusted to 6 using NaCl, as R. nottbecki was grown in this salinity. F/2-Si medium nutrients were added to both the control Z8 medium and the filtrates in order to provide excess nutrients for R. nottbecki. In addition, pH of the filtrates was measured (using a Metrohm 780 pH meter, calibrated with Merck CertiPUR 4.01 and 7.00 buffers) and a 1.5 mL sample of each filtrate was collected and frozen until toxin analysis.

A total of seven Dolichospermum sp. filtrate dilutions and a control were prepared ranging from 0 to 366 700 cells mL-1 in exponential phase, and 0 to 1 000 000 cells mL-1 in stationary phase (maximum number of cells was determined by the least dense culture). To dilute the filtrate, Z8 medium with nitrogen omitted (salinity 6) was used. The EC50 experiments were conducted in 12-well culture plates. Control medium and each Dolichospermum filtrate dilution were added in triplicate to a fixed initial R. nottbecki cell density (10 000 cells mL-1). The total experimental volume in one well was 4 mL (3.9 mL Dolichospermum sp. filtrate dilution or control Z8 medium, 0.1 mL R. nottbecki cell suspension). The plates were incubated for 4 days at 18°C in 80 μmol photons m-2 s-1 light before fluorescence was measured as described below.

Analytical procedures

To identify an optimal Dolichospermum sp. growth phase for the allelopathy experiments, the growth of the strains was followed on an almost daily basis (1–2 day intervals) by measuring chlorophyll a fluorescence (data not shown). The fluorescence was read from 400 μL samples in a 96-well plate with Varian Cary Eclipse Fluorescence Spectrophotometer, using excitation wavelength 625 nm and emission wavelength 683 nm [24]. In the EC50 experiment, fluorescence of R. nottbecki was measured after 4 days (Ex. 440 nm, Em. 680 nm).

Cell count samples (1.2 mL) for Dolichospermum sp. were collected and preserved with a drop of acid Lugol’s solution and stored in Eppendorf tubes in a refrigerator. The cell counts were performed using a 1 mL Gridded Sedgewick Rafter (Wildlife Supply Company) counting chamber and a microscope (Leica DMI3000 B) with a 200 × magnification. From each Dolichospermum sp. sample, the cells of at least 50 filaments were counted. Cell width and length were measured for each strain and salinity (N = 20), and biovolume was determined [25]. Growth rates, k, defined as doublings d-1, were calculated based on the longest period of exponential growth, using the equation k = log2(Nt/N0)/Δt, where N = biomass and t = time [26]. The interval of exponential growth was determined from growth curves established for each experimental culture replicate.

Both intracellular and extracellular toxins (for the allelopathy experiment) were measured using ELISA (Enzyme-linked immunosorbent assay) QuantiPlate Kit for Microcystin (Envirologix) following the kit instructions. Ten mL samples were taken from the cultures on three sampling days (day 1, 15 and 29) and filtered using 2.0 μm TTTP membrane filters (Isopore, Millipore). Both the filter (containing Dolichospermum sp. cells, i.e., intracellular toxins) and the 1.5 mL filtrate samples from the allelopathy experiment (i.e., extracellular toxins) were stored in -20°C. Before analysis, the filters were freeze-dried for at least 48 h. The intracellular samples were dissolved in 5 mL methanol, sonicated for 5 min and extracted overnight. The samples were dried using compressed air and dissolved again by adding 100 μL 50% methanol, followed by adding 900 μL of MilliQ over 4 days (225 μL MilliQ d-1). On the final day of MilliQ addition (final concentration of 5% methanol [27]), the samples were measured. The intracellular toxin samples were diluted (1:20–1:1000) and filtered on Whatman GF/C filters before performing ELISA. The extracellular samples were completely melted and shaken properly before measurement. The microcystin concentration was determined using a micro-plate reader (Tecan, Infinite M200) and was based on a standard curve (standards: 0.16, 0.6 and 2.5 ppb).

Statistical analyses

To analyse differences in biovolume, growth rate and allelopathic effect between strains, salinities and growth phases, a general linear model (GLM) was fitted separately to each response variable. The explanatory variables for biovolume and growth rate included strain and salinity and their interaction. A separate GLM was fitted to check the influence of strain, salinity and growth rate and their interactions on exponential phase (day 15) intracellular toxicity. For allelopathic effect as response variable, a GLM with main effects for strain, salinity and growth phase, and interactions between strain and growth phase, and salinity and growth phase was selected based on the model’s Akaike information criterion (AIC) value. Percentage reduction of R. nottbecki fluorescence by filtrates from both growth phases prepared from a concentration of ca. 4–5×105 cells mL-1 was used as a measure of allelopathic potency.

Due to temporal dependence of toxin measurements conducted at 3 time points during the experiment, a linear mixed-effects (LME) model (R package ‘nlme’ [28]) was used to analyse differences in intracellular toxin concentrations between salinities, days and strains, with salinity and day as fixed effects and strain as a random effect. Statistical significance of the random effect for strain was assessed by comparing a generalized least squares (GLS) model without random effect, but with salinity and day as main effects, with the final LME model. The comparison was executed by using a likelihood ratio test (LRT). Distributional assumptions of linear models (normality and homoscedasticity of residuals) were checked for each response variable, and biovolume and toxin data were log-transformed before analysis to meet the assumptions. Tukey’s pairwise post-hoc comparisons (R package ‘lsmeans’ [29]) were used to determine which of the effects of explanatory factors and their interactions differed significantly from each other.

The EC50 (effective dose) value was calculated from the best fitting dose-response model (judged by the smallest AIC value), using the R package ‘drc’ [30].

The non-parametric Spearman’s rank correlation was used to assess the degree of correlation between toxin concentration and allelopathic effects of the filtrates.

To check for decadal trends in salinity and Dolichospermum spp. biomass, monitoring data from 7 sampling stations in the western Gulf of Finland—northern Baltic Proper (sampling area with spatial limits N 59°03–59°85, E 21°08–24°83) between 1979 and 2013 were analysed. The data originated from national monitoring cruises, where sampling is conducted according to the Helsinki Commission (HELCOM) COMBINE programme, and they were downloaded from the databases Sumppu (Finnish Environment Institute and Finnish Meteorological Institute; and Hertta (Finnish Environment Institute; A non-parametric Mann-Kendall test was used to detect significant monotonic trends in the annual mean summer-early autumn (June-September) salinity and Dolichospermum spp. biomass at 0–10 m depth. Curves estimated with a locally weighted scatterplot smoother (LOESS; span = 0.75) with 95% confidence interval were fitted to describe the long-term variation.

All analyses were conducted using R 2.15.2 software [31].


Biovolume and growth

In the batch-culture experiments, Dolichospermum spp. cell size differed significantly between strains and salinities, varying between 58.97 ± 14.68 μm3 cell-1 (mean ± SD, n = 20) in BIR257 at salinity 6 and 159.58 ± 45.13 μm3 cell-1 in BIR256 at salinity 3 (GLM, p < 0.01, Tables 1 and 2). On average, BIR257 had a smaller biovolume than the other two strains (Tukey, p < 0.04), and the cells of all strains were largest at salinity 3 and smallest at 6 (Tukey, p < 0.001).

Table 1. Mean cellular biovolume (V; n = 20), and filtrate pH, toxin concentration and EC50 value (n = 3) of the Dolichospermum spp. strains in different salinities and growth phases.

Table 2. Results of general linear models (GLM) and linear mixed-effects (LME) models for each response variable.

Growth rates of the strains were also significantly dependent on the strain and salinity, ranging from 0.12 ± 0.01 doublings per day (mean ± SD, n = 3) in BIR250A at salinity 6 to 0.28 ± 0.03 doublings day-1 in BIR256 in freshwater (GLM, p < 0.04, Table 2, Figs 1 and 2). Although BIR250A reached the highest observed final biomass in freshwater (Fig 1), the strain had, on average the lowest maximum growth rates (Tukey, p < 0.004, Fig 2). Growth rates of all strains were highest at salinity 0 (p < 0.001).

Fig 1. Biomass development of the Dolichospermum spp. strains in the experimental salinities (mean ± SD, n = 3).

Fig 2. Biomass based growth rates (k, doublings day-1) of strains in the different salinities (mean ± SD, n = 3).

Microcystin concentrations

The intracellular microcystin concentrations of the Dolichospermum sp. cultures differed significantly between salinities and days (LME, p < 0.001; Table 2, Fig 3), but not between strains (p = 0.277). The mean intracellular microcystin concentration ranged from 1.70 ± 1.34 mg g BM-1 (mean ± SD, n = 3) in BIR256, salinity 3 on day 1, to 24.66 ± 14.54 mg g BM-1 in BIR257, salinity 6 on day 15, and was for all strains on average highest at salinity 6 and lowest on day 1 (Tukey p < 0.03, Fig 3). In addition, we tested for a potential effect of growth rate, strain and salinity on intracellular toxin concentrations during exponential growth. In addition to a significant effect of salinity (GLM, p < 0.001), but no direct effects by strain or growth rate (p > 0.40), there was a significant interaction effect between growth rate and salinity (p = 0.031; Table 2), indicating that the growth rate may have affected toxicity differently in the different salinities.

Fig 3. Dolichospermum spp. intracellular microcystin concentrations (mean ± SD, n = 3) in different salinities at the start, middle and end of the experiment.

Allelopathic effects

The pH of the Dolichospermum sp. filtrates, used for testing their allelopathic properties, varied from 7.15 to 7.93 (Table 1), whereas the average pH of the R. nottbecki culture was 9.74 and that of the control medium (Z8, salinity 6) 7.55.

All strains showed allelopathic potential by reducing the fluorescence of R. nottbecki during 4 days (Table 1, Fig 4), although during some conditions, the effects were undetected or even positive. With an EC50 value of ca. 6.2×104 cells mL-1, the exponential phase filtrate of BIR256 at salinity 3 was the most effective one against R. nottbecki (Table 1). Percentage reduction of R. nottbecki fluorescence by filtrates prepared from a comparable cell concentration (Fig 4) generally reflected the EC50 values, but the most effective strain, based on this approach, was the stationary phase BIR257 strain at salinity 6, causing a 35.4 ± 8.2% (mean ± SD, n = 3) reduction in R. nottbecki fluorescence compared with the control.

Fig 4. Allelopathic effect of Dolichospermum spp. on R. nottbecki.

Expressed as percentage fluorescence of R. nottbecki, cultured for 4 days in filtrates of exponential and stationary phase Dolichospermum spp. cultures (cell concentrations 4–5×106 mL-1), in relation to control (100%) (mean ± SD, n = 3).

Allelopathic potency differed significantly between strains and salinities (GLM, p < 0.007; Fig 4), but not between growth phases (p = 0.880; Table 2). However, interactions between strain and growth phase, as well as salinity and growth phase were significant (p < 0.001, Table 2), indicating that strain and salinity affected the allelopathic properties differently in each growth phase (see Fig 4). A significantly stronger allelopathic effect of Dolichospermum was observed when grown in salinity 3 and 6, for exponential and stationary phase respectively, than in freshwater (Tukey, p < 0.006). On average, BIR256 was more allelopathic than the other strains (p < 0.05), and the allelopathic effects were most pronounced at salinity 3 (p < 0.04).

The extracellular toxin concentrations in the exponential phase filtrates (expressed as toxin cell-1 in the original culture) ranged from 0.50 fg cell-1 in BIR257 in salinity 3 to 180.65 fg cell-1 in BIR257 in freshwater (Table 1). Allelopathic effects (percentage R. nottbecki fluorescence reduction or EC50 value) of the exponential phase filtrates did not correlate with their extracellular toxin concentration (Spearman’s rank correlation, rs < 0.19).

Long-term trends

There was a significant decreasing trend in surface water salinity of the western Gulf of Finland—northern Baltic Proper between 1979 and 2013 (Mann-Kendall test, S = -165, N = 33, p = 0.015). During the same time span, biomass of Dolichospermum spp. increased significantly (S = 170, N = 33, p = 0.009). Both trends were strongest until around 2005, after which the decline in salinity and rise in Dolichospermum spp. biomass levelled out (Fig 5).

Fig 5. Annual mean summer-early autumn (A) salinity and (B) Dolichospermum spp. biomass in the western Gulf of Finland—northern Baltic proper at 0–10 m depth in 1979–2013.

A Loess curve (span = 0.75; solid line) is fitted, with a 95% confidence interval (dashed line).


In short, this study shows that the Baltic cyanobacteria Dolichospermum spp. can grow in all studied salinities (0, 3 and 6), with the highest growth rate in freshwater. Highest intracellular microcystin concentration was measured in the highest salinity (6). Allelopathic properties were evident in all strains tested, and they were most pronounced at salinity 3. However, interactions between strain and growth phase, as well as salinity and growth phase were significant, indicating that strain and salinity affected the allelopathic properties differently in each growth phase. Monitoring data show that summertime surface water salinity has decreased between the years 1979 and 2013 while Dolichospermum spp. biomass has increased. Overall, our laboratory experiment, combined with long-term monitoring data, suggests that a decrease in salinity results in a more favourable environment for Dolichospermum spp.

The growth rates of the different Dolichospermum strains were clearly affected by salinity. Although some strain-specific variation occurred, they showed best growth in freshwater. BIR256 biomass was highest in salinity 3 during the last ten days of the experiment. The Dolichospermum taxa originate from freshwater and grow usually better in freshwater or low saline water, whereas some strains are adapted to brackish water (cf. [32]). Dolichospermum spp. are generally considered sensitive to salt, and growth decreases strongly above 10 g NaCl L-1 [33]. When exposed to salt stress, cyanobacteria increase the N-fixation leading to a further energy demand, and consequently a reduction in their growth rates can be detected [33]. Indeed, in the southern Baltic Sea, where salinity is higher (~10) the abundance of Dolichospermum is negligible [34]. Thus, it seems that Baltic Dolichospermum spp. can grow in salinities up to ~10 but, as we show here, they proliferate in freshwater.

Interestingly, cells of all strains were largest at salinity 3 and smallest at 6. Also Tonk et al. [35] showed that cell size of freshwater cyanobacteria decreases in increasing salinity. The authors claim that this occurs when osmoregulation capacity is exceeded, and cells no longer are able to uphold turgor, which can cause cell leakage and shrinking, when salinity rises even further. The phenomenon is called plasmolysis and is shown also in picocyanobacteria Synechocystis [36] and bacteria Escherichia coli [37].

A positive relationship between growth rate and microcystin production has been shown [38,39]. In the current study, however, the relationship between intracellular microcystin content and growth was not that clear (Table 2). It seems that growth rate affected toxin levels differently in different salinities and, thus, no direct relationship between growth and toxin levels is evident. The role of microcystins has not yet been determined but several hypotheses for toxin production among cyanobacteria have been suggested including grazer avoidance, allelopathy, infochemicals and stress reduction (cf. [40,41,42]). For example, higher microcystin production of Microcystis during stress has been reported in elevated temperature and during low light [43,44]. Zilliges et al. [43] found a clear fitness advantage for microcystin-producing strains, in comparison to non-producers. It is therefore possible that microcystins serve as a defence mechanism against oxidative stress. Salinity may cause oxidative stress in cyanobacteria as shown for Anabaena doliolum, Fremyella diplosiphon and Nostoc muscorum [45,46,47]. In the current study, one may speculate that enhanced toxin production is a result of elevated oxidative stress in high salinity environment, for some strains of this cyanobacterium having a freshwater origin. In the field, however, toxic Dolichospermum sp. has so far only been found in the Baltic Sea areas with salinity <6 [12]. More recently, using a microcystin-producing wild-type strain of Microcystis aeruginosa and a microcystin deficient-mutant, Makower et al. [48] found differences in gene expression between the two strains. The authors suggested that changes to the photosystem as well as a more pronounced carbon limitation for the microcystin deficient-mutant occurs when grown under similar conditions [48]. Salinity has been showed to induce stress responses in cyanobacteria including inhibition of photosynthesis associated genes and upregulation of genes associated with photorespiration [49]. Thus, it is possible that microcystin plays a role in salinity-induced changes of photosystems as well as photorespiration. However, to understand the underlying mechanisms of cyanobacteria responses to different salinities, further investigations are needed.

All three Dolichospermum strains showed allelopathic potential, which did not differ between exponential and stationary growth phase, implying that allelochemicals are continuously excreted from the cells. Dolichospermum has frequently been identified as allelopathic (reviewed by [50,51]). From a general perspective, allelopathy was strongest in salinity 3 and the highest allelopathic ability upon Rhinomonas was shown by strain BIR256. However, interactions between strain and growth phase, as well as salinity and growth phase suggest that the allelopathic capacity of Dolichospermum does not respond solely to changes in salinity, and that there seem to be strain-specific differences that are challenging to predict. Interestingly, a significantly stronger allelopathic effect of Dolichospermum is observed for exponential and stationary phase when grown in salinity 3 and 6, respectively, than when grown in freshwater. Thus, it seems as if the allelopathic potency is relatively lower in freshwater than in the two salinity (3 and 6) treatments. This suggests that salinity or salinity induced stress stimulates allelopathy in Dolichospermum in order to weaken competitors or otherwise harm them. Also during other stressful conditions, such as nutrient and light limitation, Anabaena sp. out-competed the competitor via allelopathy, and another taxon, Oscillatoria increased the production of allelopathic compounds [52,53]. Higher allelopathic potency allows the species to outcompete other bacterial and micro-algal competitors, such as the cryptophyte Rhinomonas. Dolichospermum is known to have strong allelopathic potency against cryptophytes both in mono-cultures and the natural community, decreasing their cell numbers by 50–80% [54,55]. Allelopathy can contribute to cyanobacterial bloom maintenance as the growth of competitors will be inhibited or competing species even exterminated. According to long-term data analyses, cryptophytes have rapidly decreased in the Baltic Sea [6,7], but the phenomenon is assumed to be associated with warming [56]. Biotic interactions, such as allelopathy are difficult or impossible to detect using annual monitoring data.

Microcystins are usually considered as not having a role in the allelopathic processes [50], as the microcystin-producing cyanobacteria yield a number of other bioactive compounds. Nevertheless, microcystin produced by Anabaena flos-aquae caused mortality and lowered growth in chlorophyte Chlamydonomas reinhardtii [57], whereas in other studies the compound responsible for allelopathy in Anabaena has remained unknown [52,54,55]. In the present study, allelopathic effects of the filtrates did not correlate with their extracellular toxin concentration; thus it is unlikely that microcystin caused the observed reduction in R. nottbecki fluorescence. Further, it has been suggested that rather high pH is responsible for the observed allelopathic effect by cyanobacteria [58]. However, in the present study, pH of all filtrates used in the EC50 experiment was lower than that of a dense R. nottbecki culture (>9.7), indicating that elevation of culture pH to a level intolerable for R. nottbecki by the Dolichospermum filtrates did not cause the observed allelopathic effects.

Summertime surface water salinity showed a negative trend in the western Gulf of Finland and northern Baltic Proper, based on long-term monitoring data collected between 1979 and 2013. The result was expected as salinity started to decline already in the beginning of the 1980s [5,6,7]. The salinity decrease is largely due to larger inflow of freshwater following increasing climate-related precipitation [1]. In addition, saline water inflows to the Baltic Sea via the Danish Straits from the North Sea are not as common today as before; the inflows are expected to drop also in the future [59], as a consequence of mild winters and positive NAO indices [60]. At the same time, Dolichospermum biomass showed an increasing trend. This trend has not been reported before as phytoplankton trends in the Baltic Sea have usually been analysed at the class-level. Previous trend analyses [6,7] have shown increasing late-summer biomasses for cyanobacteria in the northern Baltic Proper and the Gulf of Finland, but not in the southern Baltic Sea [34]. The main factors affecting the increase of filamentous, diazotrophic cyanobacteria, including Dolichospermum, are warmer surface waters, rising phosphate levels, and decreasing salinity [7]. In the current study we demonstrate that on a salinity scale 0–6, the growth rate of Dolichospermum spp. is highest in freshwater. Further, the allelopathic properties of Dolichospermum spp. seem to be enhanced in intermediate salinities, to be lowest in freshwater, and cellular microcystin concentration is reduced in the lower salinity range. With decreasing salinities the habitat for Dolichospermum is getting more favourable especially in the northern and eastern parts of the Baltic Sea. Thus, the species complex will probably get more common in the future, perhaps at the extent of brackish water species, such as N. spumigena.


We thank Prof. Kaarina Sivonen (University of Helsinki) for the Dolichospermum spp. strains and Dr. Anke Kremp (Finnish Environment Institute) for the Rhinomonas nottbecki culture. The reviewer is greatly acknowledged for the valuable input helping us to improve the manuscript.

Author Contributions

Conceived and designed the experiments: AB JEÖ SS. Performed the experiments: AB AV JEÖ SS. Analyzed the data: SS. Contributed reagents/materials/analysis tools: AB JEÖ SS. Wrote the paper: AB AV JEÖ SS.


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