Sequestration and Distribution Characteristics of Cd(II) by<i> Microcystis aeruginosa</i> and Its Role in Colony Formation

Bi, Xiangdong; Yan, Ran; Li, Fenxiang; Dai, Wei; Jiao, Kewei; Zhou, Qixing; Liu, Qi

doi:https://doi.org/10.1155/2016/9837598

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Volume 2016 | Article ID 9837598 | https://doi.org/10.1155/2016/9837598

Sequestration and Distribution Characteristics of Cd(II) by Microcystis aeruginosa and Its Role in Colony Formation

Xiangdong Bi,^1,2Ran Yan,²Fenxiang Li,¹Wei Dai,²Kewei Jiao,¹Qixing Zhou,¹and Qi Liu²

Academic Editor: Zhi-Hua Li

Received28 May 2016

Accepted05 Jul 2016

Published29 Sept 2016

Abstract

To investigate the sequestration and distribution characteristics of Cd(II) by Microcystis aeruginosa and its role in Microcystis colony formation, M. aeruginosa was exposed to six different Cd(II) concentrations for 10 days. Cd(II) exposure caused hormesis in the growth of M. aeruginosa. Low concentrations of Cd(II) significantly induced formation of small Microcystis colonies () and increased the intracellular polysaccharide (IPS) and bound extracellular polysaccharide (bEPS) contents of M. aeruginosa significantly (). There was a linear relationship between the amount of Cd(II) sequestrated by algal cells and the amount added to cultures in the rapid adsorption process that occurred during the first 5 min of exposure. After 10 d, M. aeruginosa sequestrated nearly 80% of 0.2 mg L⁻¹ added Cd(II), while >93% of Cd(II) was sequestrated in the groups with lower added concentrations of Cd(II). More than 80% of the sequestrated Cd(II) was bioadsorbed by bEPS. The Pearson correlation coefficients of exterior and interior factors related to colony formation of M. aeruginosa revealed that Cd(II) could stimulate the production of IPS and bEPS via increasing Cd(II) bioaccumulation and bioadsorption. Increased levels of cross-linking between Cd(II) and bEPS stimulated algal cell aggregation, which eventually promoted the formation of Microcystis colonies.

1. Introduction

Microcystis blooms frequently occur in eutrophic freshwaters and their outbreaks always lead to water deoxygenation, microcystin pollution, and fish kill. During Microcystis blooms, algal cells aggregate largely on the surface of water and can be visible. Colony formation plays a vital role in the occurrence of Microcystis blooms [1]. It protects Microcystis cells from zooplankton grazing [2], viral or bacterial attack, and other potential negative environmental factors [3] and also provides a competitive advantage over other phytoplankton species [4]. However, how unicellular Microcystis cells aggregate into colonies exactly is not yet known. Previous studies have found that both biotic and abiotic factors, such as zooplankton grazing, nutritive salt, and microcystins, could stimulate Microcystis colony formation [2, 4]. Both zooplankton grazing and microcystins were reported to increase the amount of extracellular polysaccharides (EPS) and eventually stimulate aggregation of Microcystis cells [2].

Cyanobacterial blooms frequently occur in eutrophic waters with serious metal pollution [5, 6]. Cadmium (Cd), as a nonessential metal for biology, has become an important pollutant in natural freshwaters due to increasing use in industry, agriculture, and anthropogenic activities [7]. The negative effects of Cd on the environment have been recognized and it readily accumulates in living organisms. It was documented that cyanobacteria (Synechocystis sp. BASO670 and Synechocystis sp. BASO672) had high tolerance to Cd(II)-induced toxic effects, and Cd(II) could significantly stimulate EPS production in these two Synechocystis isolates [8]. In our previous study, we found there were significant differences in cadmium accumulation in four sizes of Microcystis colony [9] and cadmium accumulation decreased with increasing Microcystis colony sizes. We speculated that cadmium ions might play an important role in the early stage of Microcystis colony formation in natural waters [9].

To better predict, prevent, and control Microcystis blooms in natural waters, it is important to understand all the factors involved in triggering colony formation of Microcystis species. In this study, both sequestration and distribution characteristics of Cd(II) by toxic M. aeruginosa and physiological responses related to colony formation were investigated in laboratory conditions.

2. Materials and Methods

2.1. Cyanobacterial Culture

M. aeruginosa FACHB-905, a very common microcystin-producing Microcystis strain, which was provided by the Institute of Hydrobiology of China, can form large visible colonies with non-microcystin-producing Microcystis strains in natural waters. M. aeruginosa FACHB-905 were cultured in conical flasks containing sterilized BG11 medium (without EDTA) under a 12 light:12 dark cycle with a light density of 60 μmol m⁻² s⁻¹ at 25°C. To reduce any effects related to minor differences in photon irradiance and to maintain homogeneity, the flasks were shaken slightly four times every day and rearranged randomly. Cultures were grown until the exponential growth phase.

2.2. Experimental Design

CdCl₂ (Merck, Germany) was dissolved in distilled water to prepare a stock solution (20000 mg L⁻¹). Based on the median effective concentration EC₅₀-96 h = 0.383 mg L⁻¹, determined by the method of Vanewijk and Hoekstra [10] of Cd(II) on M. aeruginosa obtained in preliminary experiments, Cd(II) was added to algal culture at an initial density of 5.473 × 10⁶ ind mL⁻¹ to final concentrations of 0 (control), 0.0125, 0.025, 0.05, 0.1, 0.2, and 0.4 mg L⁻¹, with three replicate flasks per concentration. Samples were removed from the cultures at 0, 5, 10, 20, 60, and 120 min and then daily until the 10th day of the experiment, to determine the algal cell density, colony numbers, bioadsorption and bioaccumulation characteristics of Cd(II), and bound extracellular polysaccharide (bEPS) and intracellular polysaccharide (IPS) contents of M. aeruginosa.

2.3. Effects of Cd(II) on Growth and Colony Formation of M. aeruginosa

Algal cell density and M. aeruginosa colonies were measured using a hemocytometer under a light microscope (×40). To reduce erroneous results, samples were taken 1 cm below the water surface with movement by a wide-mouth pipette, and the flasks were shaken up slightly 30 min before taking samples. The inhibition rate (IR), the decrease of intact algae in suspension, was calculated using the following formula: IR (%) = , where is algal cell density in the control (ind L⁻¹) and N_S is algal cell density in the Cd(II)-added treatment (ind L⁻¹) [11]. M. aeruginosa were classified as unicellular, two-cell aggregation or colony (aggregation of ≥3 cells).

2.4. Determination of Bioadsorption and Bioaccumulation of Cd(II) by M. aeruginosa

Algal culture (500 mL) was centrifuged at 10,000 ×g for 10 min at 4°C, and the supernatant was dried to constant weight at 180°C to determine the content of Cd(II) in the medium (μg L⁻¹). The algal cell deposit was resuspended in 1.0 × 10⁻³ mol L⁻¹ EDTA solution and then stirred with glass beads for 30 min to detach bEPS associated with the algal cells. After centrifugation at 10,000 ×g for 30 min at 4°C, the algal cell deposit was used to determine Cd(II) content accumulated inside algal cells (pg cell⁻¹). The resulting supernatant was dried to constant weight at 180°C to determine Cd(II) content bioadsorbed on the algal cell walls. The resulting solid was precisely weighed (0.5 g) and transferred into a polytetrafluoroethylene, where 7 mL of HNO₃ and 1 mL of H₂O₂ were added. The digester was sealed tightly and placed in a microwave digestion system (ETHOS One, Milestone, Italy). The procedure for microwave digestion is summarized as follows: the digester was heated from 25°C to 180°C over 10 min and then held for 25 min to digest the samples. After complete digestion, the digestion solution was evaporated to 2.5 mL, transferred to a 50 mL volumetric flask, and diluted with deionized water. A reagent blank was prepared using the same chemicals and digestion procedure as a comparison. Content of Cd(II) in collected samples was measured using Inductively Coupled Plasma-Atomic Emission Spectrometry (ICP-AES) using an ICP-9000 (N + M) (Thermo Jarrell Ash, USA), for which the detection limit of Cd is 0.01 mg kg⁻¹.

2.5. Effects of Cd(II) on bEPS and IPS Production by M. aeruginosa

Algal culture (50 mL) was centrifuged at 5,000 ×g for 10 min at 4°C, and the cell pellet was washed with 1.0 × 10⁻³ mol L⁻¹ EDTA solution using a glass rod. The resulting suspension was stirred with glass beads to detach bEPS associated with the algal cells. After centrifugation at 10,000 ×g for 30 min at 4°C, the algal cell pellet and supernatant were collected to determine IPS and bEPS contents (pg cell⁻¹), respectively. To precipitate proteins from the supernatant, trichloroacetic acid (TCA) was added to a final concentration of 10% and the precipitated proteins were removed by centrifugation at 10,000 ×g for 20 min at 4°C. The clear supernatant was precipitated overnight at 4°C with six volumes of 95% ethanol. TCA precipitation and ethanol precipitation were repeated once. After centrifugation (12,000 ×g for 30 min at 4°C), the deposit obtained was dissolved in distilled water, dialyzed (3,600 mol wt cutoff tubing) against distilled water at 4°C for 24 h with 2 times, and then concentrated to 2 mL by rotary evaporation. The content of bEPS (pg cell⁻¹) was estimated using the phenol-sulfuric acid method [12]. Algal cells were disrupted by freezing and thawing repeatedly to obtain IPS and then treated as for bEPS measurement.

2.6. Statistical Analysis

Results are expressed as means ± SD and were subjected to Fisher’s least significant difference test (SPSS version 17.0) to determine significant differences () among groups [13]. The Pearson correlation coefficient was examined by paired t-test (SPSS version 17.0) [14].

3. Results and Discussion

3.1. Effects of Cd(II) on Growth of M. aeruginosa

The growth of M. aeruginosa FACHB-905 was affected in a Cd(II) concentration-dependent manner. With increasing exposure time, M. aeruginosa cell densities increased in low concentration Cd(II)-added groups (0.0125 and 0.025 mg L⁻¹) and decreased in high-concentration Cd(II)-added groups (0.05, 0.1, 0.2, and 0.4 mg L⁻¹) as compared with the control groups (Figure 1). These results indicated that Cd(II) had a dual effect (promotion and inhibition) on the growth of M. aeruginosa. Such an effect is described as hormesis, a dose-response relationship characterized by low-dose stimulation and high-dose inhibition [15]. Gong et al. found that inorganic arsenic could also cause hormesis in M. aeruginosa FACHB 905 [16]. In our experiment, high Cd(II) of concentrations inhibited the growth, possibly because the Cd(II) concentration exceeded the tolerance limit of M. aeruginosa cells, causing cell structure damage and disintegration. Among the tested concentrations, 0.4 mg L⁻¹ Cd(II) exhibited the strongest inhibitory effects, with a 4-day IR of 74.752% and a 10-day IR of 99.992% (Figure 2). It is documented that M. aeruginosa PCC 7806 was susceptible to trace metal toxicity [17], while a M. aeruginosa strain isolated in the Czech Republic had high tolerance to 5.0–10.0 mg L⁻¹ Cd(II) [18]. Therefore, it is possible that different strains of M. aeruginosa have different sensitivities to Cd(II)-induced toxicity.

3.2. Effects of Cd(II) on Colony Formation by M. aeruginosa

Compared with colonial forms that predominate in natural conditions, Microcystis exists mainly as noncolonial (single and a few paired) cells in culture [19]. Colony formation of M. aeruginosa is a phenotypic response of single cells to environmental stress [3]. Colonial Microcystis had higher endurance to heavy metal-induced stress than noncolonial Microcystis [20]. Our results show that three concentrations of Cd(II) (0.05, 0.1, and 0.2 mg L⁻¹) significantly induced Microcystis colony formation (), and 0.2 mg L⁻¹ Cd(II) had the highest inductive effect (Figure 3). The proportion of Microcystis colonies was significantly decreased in the 0.4 mg L⁻¹ Cd(II)-added group after 4 d, and no Microcystis colonies could be observed under the microscope after 6 d, which might result from the strong inhibitory effects of 0.4 mg L⁻¹ Cd(II) on the growth of M. aeruginosa (Figures 1, 2, and 3). No colonies with five or more cells were observed during the whole experimental period. Unlike Fe, Al, Mn, Pb, and Cr, Cd was the only heavy metal element accumulated much higher in small Microcystis colony than in middle, large, and super-large colonies in natural waters [9]. These observations indicate that Cd(II) may play an important role in the early stage of Microcystis colony formation in natural waters [9].

3.3. Sequestration and Distribution Characteristics of Cd(II) by Microcystis Cells

When Microcystis cells were exposed to Cd(II), a rapid adsorption process occurred in the first 5 min. There was a linear relationship between Cd(II) sequestrated by algal cells (including Cd(II) bioadsorbed on bEPS and bioaccumulated inside cells) and the added Cd(II) concentrations during this time period (y = 8.5326x − 8.664; = 0.9864). More chances for metal ions to combine with cation-chelating binding sites in bEPS were provided with the increasing Cd(II) concentrations [21, 22]. Once Cd(II) was bioadsorbed onto the external cell wall, an internal bioaccumulation process would begin immediately [23]. Use of different strains of M. aeruginosa might lead to a longer adsorption process (10 min) [24]. In our experiment, there was also a slow adsorption process following the initial 5 min rapid adsorption, suggesting that Cd(II) was removed via interactions with functional groups on the cell surface [8, 17].

On longer Cd(II) exposure the proportion of Cd(II) sequestrated in Microcystis cells increased, reaching >93% at the end of the 10th day in the groups exposed to ≤0.1 mg L⁻¹ Cd(II) (Figure 4). M. aeruginosa sequestrated >80% of the 0.2 mg L⁻¹ added Cd(II). We suggest that when 0.2 mg L⁻¹ Cd(II) was added, Cd(II) sequestration by M. aeruginosa cells reached its saturation level. Considering the sequestration Cd(II) in M. aeruginosa, >80% was bioadsorbed by bEPS and <20% was bioaccumulated inside algal cell (Figures 5 and 6), which is consistent with the results of Parker et al. [25] and Ozturk et al. [8].

3.4. Effects of Cd(II) on bEPS and IPS Production by M. aeruginosa

Under normal physiological conditions, polysaccharide produced in cells can be partially secreted to form EPS. The cyanobacterial EPS can be divided into two main groups: polysaccharides bound to the cell surface (bEPS) and soluble polysaccharides released into the surrounding environment (soluble extracellular polysaccharide, sEPS) [26]. Bound extracellular polysaccharide, referred to as sheath, capsule, or slime, plays an important role in the attachment of M. aeruginosa cells into colonies and in protecting cells from unfavorable environmental conditions [26]. Compared to the control, no significant changes in IPS content were observed in M. aeruginosa exposed to 0.0125 and 0.025 mg L⁻¹ Cd(II) throughout the experiment, and a similar result was obtained for bEPS for the first 6 days (Figures 7 and 8), because M. aeruginosa in long-term laboratory culture responded only slowly to slight environmental disturbance [27]. Higher concentrations of Cd(II) (0.05, 0.1, and 0.2 mg L⁻¹) significantly and simultaneously increased IPS and bEPS levels throughout the experimental period () (Figures 7 and 8). IPS and bEPS contents changed in the same way as each other after Cd(II) exposure and had a high Pearson correlation coefficient throughout the experiment (Table 1), suggesting Microcystis cells could respond positively to Cd(II) stress by secreting organic substances (mainly polysaccharides) via active transport [28] (Figures 7 and 8). It is also worth noting that Cd(II) could significantly stimulate bEPS production of M. aeruginosa at relatively low concentrations, while the stimulatory activities of Pb(II) were observed at much higher concentrations [29]. Therefore, we speculate that Cd(II) at low concentration could promote the early formation of Microcystis colonies by stimulating bEPS production in natural waters.

3.5. Role of Cd(II) in Colony Formation of M. aeruginosa

The Pearson correlation coefficients of exterior and interior factors related to colony formation by M. aeruginosa are shown in Table 1. With increasing concentrations of Cd(II) added to the culture medium, Cd(II) bioadsorption onto bEPS and Cd(II) bioaccumulation inside algal cells significantly increased. Increased Cd(II) bioaccumulation inside algal cells stimulated more IPS production. We suggest that, through active transport [28], more IPS was secreted outside the cells, leading to an increased chance of cross-linking between Cd(II) and bEPS [30]. Algal cell aggregation was stimulated by this increased cross-linking, which eventually promoted the formation of Microcystis colonies.

4. Conclusions

M. aeruginosa was very sensitive to Cd(II) compared to other heavy metal ions and adsorbed >93% of the Cd(II) in the culture medium when exposed to ≤0.1 mg L⁻¹ Cd(II). Among the sequestrated Cd(II) in M. aeruginosa, >80% was bioadsorbed by bEPS, and <20% was bioaccumulated inside algal cells. Under the stress of Cd(II), M. aeruginosa increased the production of IPS and bEPS, which could significantly promote the formation of small colonies. Notably, this phenomenon occurred at low Cd(II) concentrations, close to those found in natural waters. Moreover, we have found that Pb(II) in the tolerance range of M. aeruginosa could stimulate bEPS production, which promoted colony formation [29]. Therefore, heavy metals with different stimulatory effects on different stages of the formation of Microcystis colonies might be one factor that contributes to the occurrence of M. aeruginosa blooms in natural conditions.

Abbreviations

IPS:	Intracellular polysaccharide
bEPS:	Bound extracellular polysaccharide
sEPS:	Soluble extracellular polysaccharide
EPS:	Extracellular polysaccharide
IR:	Inhibition rate
ICP-AES:	Inductively Coupled Plasma-Atomic Emission Spectrometry.

Competing Interests

The authors declare that they have no competing interests.

Acknowledgments

This work was supported by grants from China National Critical Project for Science and Technology on Water Pollution Prevention and Control (2012ZX07501002-001), the National Natural Science Foundation of China (Grant no. 31300393), China Postdoctoral Science Foundation (Grant nos. 2015T80212 and 2014M551013), Project of Tianjin Science and Technology (Grant nos. 16JCYBJC29900 and 15ZCZDNC00230), and Project of Tianjin Municipal Science and Technology Support Program (Grant no. 12ZCDZNC05300).

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Copyright © 2016 Xiangdong Bi et al. This is an open access article distributed under the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.

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