Open Access

The Effect of Copper and Selenium Nanocarboxylates on Biomass Accumulation and Photosynthetic Energy Transduction Efficiency of the Green Algae Chlorella Vulgaris

Nanoscale Research Letters201712:147

Received: 31 December 2016

Accepted: 10 February 2017

Published: 23 February 2017


Nanoaquachelates, the nanoparticles with the molecules of water and/or carboxylic acids as ligands, are used in many fields of biotechnology. Ultra-pure nanocarboxylates of microelements are the materials of spatial perspective. In the present work, the effects of copper and selenium nanoaquachelates carboxylated with citric acid on biomass accumulation of the green algae Chlorella vulgaris were examined. Besides, the efficiency of the reactions of the light stage of photosynthesis was estimated by measuring chlorophyll a fluorescence. The addition of 0.67–4 mg L−1 of Cu nanocarboxylates resulted in the increase in Chlorella biomass by ca. 20%; however, their concentrations ranging from 20 to 40 mg L−1 strongly inhibited algal growth after the 12th day of cultivation. Se nanocarboxylates at 0.4–4 mg L−1 concentrations also stimulated the growth of C. vulgaris, and the increase in biomass came up to 40–45%. The addition of Se nanocarboxylates at smaller concentrations (0.07 or 0.2 mg L−1) at first caused the retardation of culture growth, but that effect disappeared after 18–24 days of cultivation. The addition of 2–4 mg L−1 of Cu nanocarboxylates or 0.4–4 mg L−1 of Se nanocarboxylates caused the evident initial increase in such chlorophyll a fluorescence parameters as maximal quantum yield of photosystem II photochemistry (F v/F m) and the quantum yield of photosystem II photochemistry in the light-adapted state (F v'/F m'). Photochemical fluorescence quenching coefficients declined after 24 days of growth with Cu nanocarboxylates, but they increased after 6 days of the addition of 2 or 4 mg L−1 Se nanocarboxylates. Those alterations affected the overall quantum yield of the photosynthetic electron transport in photosystem II.


Copper Selenium Nanoparticles Nanocarboxylates Chlorella vulgaris Green algae Productivity Chlorophyll fluorescence


Nowadays, the range of nanomaterial utilization in biological applications broadens rapidly. Uptake, translocation and accumulation of nanoparticles in living organisms depend on the concentration, kind, size, surface area, chemical composition and stability of nanoparticles, species of organism etc. [13]. Interaction of nanoparticles with organisms may cause various physiological and biochemical changes, both positive and negative.

Promising nanomaterials are not only colloid solutions of nanoparticles but also so-called nanoaquachelates, the nanoparticles with the molecules of water and/or carboxylic acids as ligands. Primary nanomaterials for nanoaquachelate production are colloid nanoparticles obtained by means of blast erosion method, the type of electric impulse ablation technique based on the effect of energy self-concentration in the local microvolumes of conductor [4, 5]. Blast erosion nanotechnologies provide the opportunity to produce chelates with high coordination numbers [4]. The stability of such chelate complexes does not depend on the dimensions of nanoparticles because the surface electric charge and, correspondingly, the coordination number of the obtained spherical nanoparticle are proportional to its size. The obtained hydrated nanoparticles possess high chemical activity and hence can be further carboxylated by addition of the appropriate carbonic acid [6]. The structure of nanoaquachelates can be described by general formula [ηM 2n(H2O) m (HOOCR) p ]2n, where ηM 2n− is a core nanoparticle with surface electric charge 2n−; m and p are the numbers of H2O and RCOOH ligands, respectively [7]. The value of the negative electric charge at the surface of nanoparticle relates to the amount of ligands as 2n = 2m + p. The ability of hydrated and/or carboxylated nanoparticles to penetrate easily the cell membranes and release the ligands thereafter form the prerequisite for their high biological activity coupled with biocompatibility. Another characteristic feature of resultant products is their extremely low content of impurities, as compared with the nanomaterials obtained by chemical methods [4]. It was found that the toxicity of metal nanoaquachelates was much lesser than that of respective inorganic salts [4, 7]. Currently, the ultra-pure nanocarboxylates of principal biogenic and biocide elements are produced commercially and used widely in human and veterinary medicine, agriculture, food and cosmetic industry, municipal engineering, etc. [4]. Good prospects have nanocitrates, so far as the salts of citric acid are approved for use in the food industry [8].

Copper (Cu) and selenium (Se) are microelements essential for plant metabolism; however, their higher concentrations exert toxic effects. The ranges of physiological Cu and Se concentrations are rather narrow; they depend on the type of microelement-containing compound, oxidation state of microelement, species of the organism and many other factors. Copper is involved in many physiological processes because it can exist in multiple (Cu2+ and Cu+) oxidation states in vivo. Copper acts as a structural element in regulatory proteins and participates in photosynthetic electron transport, mitochondrial respiration, oxidative stress responses, cell wall metabolism and hormone signaling [9]. Copper ions act as cofactors in many enzymes such as Cu/Zn superoxide dismutase, cytochrome c oxidase, plastocyanin, amino oxidase, laccase and polyphenol oxidase [9]. At the cellular level, copper also plays an essential role in signaling of transcription and protein trafficking machinery, oxidative phosphorylation and iron mobilization [9].

Selenium is mostly involved in antioxidative processes [10]. This trace element is indispensable not only for heterotrophic organisms, such as mammals, fish and many bacteria, but also for certain green algae. However, its physiological significance for other photosynthesizing organisms, including higher plants, is not ascertained finally [11]. Predominant forms of bioavailable Se are its inorganic salts, selenite (SeO3 2−) and selenate (SeO4 2−). Living organisms contain selenium mostly in the form of selenoproteins, where Se atoms replace those of sulphur in some cysteine and methionine residues. In particular, Se is found in the active centres of such antioxidant enzymes as glutathione peroxidases and thioredoxin reductases [12]. At the same time, high concentrations of selenium (1–10 mg kg−1 for many plant species) are toxic, due to excessive incorporation of Se in place of S in amino acids, with subsequent alteration of protein three-dimensional structure and impairment of their enzymatic functions [11, 13].

The aim of the present research was to study the effects of copper and selenium nanoaquachelates carboxylated with citric acid on the growth rates and efficiency of photosynthetic photochemical reactions of the unicellular green algae Chlorella vulgaris that are widely used in biotechnology.


C. vulgaris Beijer. was grown under sterile conditions at a temperature of 25–26 °C in 1000-mL Erlenmeyer flasks containing 400 mL of liquid mineral medium [14], EDTA being omitted:

[mg L−1]



















The cultures were illuminated continuously with warm white fluorescent lamps providing the irradiance of 40–42 μmol m−2 s−1 photosynthetic photon flux density and stirred by shaking two times a day. At inoculation, the algal cultures were supplied with copper or selenium nanoparticles (average size about 100 nm) carboxylated with citric acid (nCu-Citr or nSe-Citr, respectively) [6, 7], obtained from the Ukrainian State Scientific Research Institute ‘Resource’ (Kyiv, Ukraine), to final concentrations ranging from 0.67 to 40 mg L−1 (nCu-Citr) and from 0.07 to 4 mg L−1 (nSe-Citr). Algal culture without nanoparticle addition was used as a control one. The samples for analyses were harvested at the beginning of the experiment and then every 6 days.

To determine the dry mass of algae, they were concentrated by centrifugation (10 min at 1500×g), washed two times with distilled water with the subsequent biomass concentration and dried to a constant weight at 105 °C.

The efficiency of photochemical reactions in the photosystem II was estimated by measuring modulated chlorophyll a fluorescence at room temperature [15] using the fluorometer XE-PAM (Heinz Walz GmbH, Effeltrich, Germany). Prior to measurements, all the samples were dark-adapted for 10 min in the stirring-enabled fluorometer cuvette. The measuring light flashes (2 Hz, 0.15 μmol m−2 s−1) were adjusted to be sufficiently weak for the prevention of photochemical charge separation in photosystem II reaction centres, as described previously [16]. The actinic light intensity was similar to that applied during the cultivation of algae. The saturating pulse duration and intensity (5500 μmol m−2 s−1, 1 s) were selected to ensure the complete closure of all photosystem II reaction centres.

Common chlorophyll fluorescence parameters were calculated [15, 17]:
  • F v/F m, maximal quantum yield of photosystem II photochemistry

  • F v'/F m', quantum yield of photosystem II photochemistry in the light-adapted state

  • q P, or F q'/F v', photochemical quenching coefficient

  • q L, or (F q'/F v')(F 0'/F'), photochemical quenching parameter estimating the fraction of open photosystem II centres

  • NPQ, non-photochemical quenching

  • Φ PSII, or F q'/F m', the effective quantum yield of photosystem II electron transport

All the measures were taken as the average of minimum three biological and analytical replicates from different test samples, and standard deviations were calculated.

Results and Discussion

The concentrations of copper nanoparticles chosen for the present experiment correspond to those of copper ions naturally occurring in the polluted aquatic environments [18]. The addition of copper nanoparticles carboxylated with citric acid (nCu-Citr) in all the range of concentrations examined evoked the initial increase in Chlorella dry matter (Fig. 1). If nCu-Citr concentration did not exceed 4 mg L−1, 20% growth stimulation was retained up to the end of experiment. Notably, the effect of the lowest applied concentration (0.67 g L−1) was the most sustainable. On the contrary, the addition of 20 to 40 mg L−1 nCu-Citr showed to be toxic to C. vulgaris because it stopped the algal growth starting from the 12th day of cultivation.
Fig. 1

Biomass of Chlorella vulgaris grown in the presence of nCu-Citr

The increase in inorganic copper concentration may cause the impairment of the biochemical and physiological processes in algal cells [19]. The redox transitions that make Cu an essential element also contribute to its inherent toxicity, catalyzing the production of reactive oxygen species with subsequent damage of biomolecules [9]. However, copper is one of the most toxic metals to unicellular algae [20]; C. vulgaris was earlier found to be rather insensitive to copper toxicity [18, 21]. On the one hand, it was shown that C. vulgaris growth in the presence of 100 mg L−1 of copper was not impaired [22] or that it can tolerate up to 0.5–1 mg L−1 [23] or even 100 mM [24] copper. However, other researchers found that the exposure to 0.5–100 μM Cu significantly decreased growth, chlorophyll and protein content, increased reactive oxygen species content and reduced the transcript abundance of photosynthesis-related genes psbA and rbcL [20, 25, 26].

CuO nanoparticles have been shown to induce growth inhibition and lead to cellular oxidative stress in green alga Chlamydomonas reinhardtii at concentrations higher than 100 mg L−1 [27]. The nanoparticle form of Cu was proved to have a unique advantage over Cu2+ in entering the bacterial cells, thus mediating specific effects (e.g. DNA oxidative damage) [2]. Additional testing should be conducted on the effects of various nano-Cu species in other organisms.

Selenium nanoparticles carboxylated with citric acid (nSe-Citr) at 2 or 4 mg L−1 concentrations induced 1.4-fold increase in C. vulgaris biomass accumulation after 6 days of cultivation (Fig. 2). Their positive effect on Chlorella growth retained throughout the whole period of experiment, although weakening with time. If nSe-Citr was added to 0.4 mg L−1 concentration, during 18 days, the growth of C. vulgaris increased only by 7–11%, but then it accelerated, and at the end of the experiment became the same as in the case of addition of five- to tenfold higher nSe-Citr concentrations. Being added at smaller concentrations (0.07 or 0.2 mg L−1), nSe-Citr caused the retardation of culture growth on the 12th day, but the amount of Chlorella dry mass gained the values of the control culture on the 18th day (0.2 mg L−1 nSe-Citr) or on the 24th day (0.07 mg L−1 nSe-Citr).
Fig. 2

Biomass of Chlorella vulgaris grown in the presence of nSe-Citr

Inorganic selenium salts in the concentration range close to that applied in the present study can either stimulate or inhibit the growth of various algal species [12, 2831]. For example, the growth of C. vulgaris in Erlenmeyer flasks under the temperature and illumination regime similar to that of our study was stimulated by 25–75 mg L−1 sodium selenite [30].

Chlorophyll a fluorescence kinetic analysis is commonly used as a tool to identify changes in photosynthetic light reactions because environmental stress can reduce the ability of plants to metabolize normally, resulting in imbalance between the light energy absorption by chlorophyll and the use of energy in photosynthesis [25]. Based on our data concerning Chlorella biomass accumulation, only the effects of 0.67–4 mg L−1 of nCu-Citr on modulated chlorophyll a fluorescence were determined, and for nSe-Citr, the effects of the whole concentration range were examined.

Copper (2–4 mg L−1) and selenium (0.4–4 mg L−1) nanocarboxylates caused the initial rise in F v/F m and F v'/F m' parameters (Figs. 3 and 4a, b) indicating, respectively, the capacity of dark-adapted and light-adapted algal cells to convert light energy into the energy of chemical bonds. Thereafter, in the case of nCu-Citr addition, the difference of both F v/F m and F v'/F m' with the respective control values diminished. On the 24th day of the experiment, their values exceeded the control ones only in the case of 4 mg L−1 nCu-Citr added. F v/F m and F v'/F m' in Chlorella cells grown in the presence of 0.67 mg L−1 nCu-Citr showed no appreciable distinctions with those of the control samples. On the other hand, the extent and duration of nSe-Citr positive effect on F v/F m and F v'/F m' values increased with the growth of their amount added.
Fig. 3

Chlorophyll fluorescence parameters of Chlorella vulgaris grown in the presence of various concentrations of nCu-Citr (af)

Fig. 4

Chlorophyll fluorescence parameters of Chlorella vulgaris grown in the presence of various concentrations of nSe-Citr (af)

Both photochemical quenching coefficients (q P and q L) estimate the fraction of open photosystem II reaction centres and thus represent the proportion of light excitation energy captured by photosystem II that is used for electron transport. Neither q P (Fig. 3c) nor q L (Fig. 3d) depended on the concentration of added nCu-Citr, and at the end of experiment, their values were lowered by 7–13% as against the control. On the contrary, 2 or 4 mg L−1 nSe-Citr stimulated the increase in q P on the sixth day of C. vulgaris cultivation (Fig. 4c), and q L was lowered after 12 days of Chlorella growth with 4 mg L−1 nSe-Citr (Fig. 4d). The assessment of q P parameter is widely accepted; the formula for q P calculation is based on the assumption that each photosystem II centre possesses its own independent antenna system. Otherwise, the q L parameter proposed by Kramer et al. [32] proceeds from the so-called lake model that photosystem reaction centres are connected by shared antennae and is recommended for more accurate assessment of the redox state of the primary quinone acceptor (Q A) pool instead of q P, especially at high light intensities [17]. In our experiment, even taking into account that photosynthetic photon flux density was rather low, q P values exceeded those of q L by 15–40% (Figs. 3 and 4c, d). Such results are not common, e.g. in the recent thorough investigation of another green alga, C. reinhardtii, undergoing nitrogen deprivation, the values of q L were shown to be approximately 1 to 2% lower than q P [33]. Taking into account that the calculation of q L is easy and does not demand any modifications of the generally accepted fluorescence measurement protocol, more attention may be paid to this parameter in order to gain further insight into the processes of light energy transfer between antennae in algae.

Φ PSII, or operational photosystem II quantum yield, evaluates the net efficiency of photosystem II photochemical processes and is considered to be the fluorescence index of the rate of linear photosynthetic electron transport. As this parameter is in fact the product of F v'/F m' and q P, therefore, its initial rise in the cells cultivated with 2 or 4 mg L−1 nCu-Citr is due to the increase in F v'/F m' (Fig. 3e). Similarly, q P decline contributes to the lowering of Φ PSII on the 24th day of growth in the presence of copper nanoparticles. In the case of nSe-Citr addition, the increase in Φ PSII was generally due to the rise of F v'/F m' values (Fig. 4e).

The nonphotochemical quenching (NPQ) value represents all quenching processes of the photosystem II chlorophyll fluorescence not directly related to photochemistry [34]. Treatment with copper nanocarboxylates did not affect that parameter significantly in C. vulgaris (Fig. 3f). However, the utilization of 4 mg L−1 nSe-Citr caused the reliable NPQ increase (Fig. 4f), so one can suggest that absorbed light energy exceeded the capacity of its utilization in photosynthetic processes.

As was found previously [16], millimolar concentrations of citrate do not exert significant effect on photochemical reactions in algae. Therefore, the study of any possible effects of nano- and micromolar citrate concentrations present in C. vulgaris cultures was beyond the scope of the present experiment.

Photosynthetic electron transport is known to be altered under both copper deficiency and excess conditions [9, 35, 36]. Photosystem II activity appears to be the most sensitive site of copper inhibition [35, 37, 38]. The important sites of copper inhibitory effect are associated with oxidizing and reducing sides of photosystem II electron transport [18, 37]. Copper ions suppress the activity of photosynthetic water splitting system [37, 39], interact with the QB [39, 40] and pheophytin [41] electron transport sites, eventually preventing the conversion of light energy absorbed by chlorophyll antenna complex into photosystem II electron transport. The effects of copper on the photosystem II photochemistry consequently decrease carbon dioxide uptake in algal cells [18, 42].

Previously, Juneau et al. [18] found that chlorophyll fluorescence parameters F v/F m, Φ PSII and q P obtained from C. vulgaris did not show susceptibility to CuSO4 at 100 μg Cu L−1 concentrations as compared with other green algae, C. reinhardtii and Selenastrum capricornutum. Besides, C. vulgaris was able to develop resistance to copper if the exposure was prolonged. Similarly, recent investigation by Chen et al. [25] showed that 1–2 μM CuCl2 somewhat improved photosystem II photochemical performance of C. vulgaris (judging by increase in F v/F m, q P and Φ PSII values). At the same time, 4 μM and higher CuCl2 provoked plasmolysis of C. vulgaris cells accompanied by complete loss of photosynthetic activity, thus emphasizing the extreme narrowness of physiological Cu2+ concentration range. In our study, much higher amount of copper in nanocarboxylate form was applied, but the inhibition of photosynthetic energy transduction, if any, was far from prominent.

Little is known to date about the effect of selenium at any form on photosynthetic processes. It was found that selenium (50 mg L−1) in the form of sodium selenate stimulated starch accumulation in the cells of the wild type of green alga Scenedesmus quadricauda; however, the process of starch hyperaccumulation followed the severe retardation of algal growth [12]. Sodium selenite in the concentrations up to 75 mg L−1 raised chlorophyll a and carotenoid content after 6 days of C. vulgaris cultivation [30]. Selenium was not shown to stimulate photosynthesis of Euglena gracilis [29]; however, in that study, selenite was used and its maximal concentration was tenfold lower than in our research. Therefore, the data obtained contribute to the understanding of the mechanisms of selenium effect on the photosynthetic productivity of algae. Further investigations require the thorough study of nanocarboxylate effects on photosynthesis, as compared with inorganic salts of respective microelements.


The utilization of copper (0.67–4 mg L−1) or selenium (0.4–4 mg L−1) nanoparticles, carboxylated with citric acid, has positive effect on C. vulgaris growth and transiently improves the efficiency of photosystem II photochemical reactions. Therefore, it may be recommended for further investigations aimed to stimulate the accumulation of algal biomass as the source of valuable nutrients, biofuels or soil fertilizers. Since growth and photosynthesis of Chlorella tolerate much higher concentrations of microelements in the form of nanocarboxylates than those in ionic forms, nanocarboxylates can be further applied in algal biotechnology.



The authors are thankful to Prof. V.H. Kaplunenko (Ukrainian State Scientific Research Institute ‘Resource’) for kindly granted preparations of nanoaquachelates.


This work, including the design of the study, collection, analysis and interpretation of data and writing the manuscript, was funded by the National Academy of sciences of Ukraine within research theme no. 0112U000059.

Authors’ Contributions

NM was responsible for data collection and analysis and for preparing the manuscript draft. EZ worked on the concept of the given study and on the final manuscript review. Both authors read and approved the final manuscript.

Competing Interests

The authors declare that they have no competing interests.

Open AccessThis article is distributed under the terms of the Creative Commons Attribution 4.0 International License (, which permits unrestricted use, distribution, and reproduction in any medium, provided you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made.

Authors’ Affiliations

M.G. Kholodny Institute of Botany of the National Academy of Sciences of Ukraine


  1. Bell IR, Ives JA, Jonas WB (2014) Nonlinear effects of nanoparticles: biological variability from hormetic doses, small particle sizes, and dynamic adaptive interactions. Dose Response 12:202–232View ArticleGoogle Scholar
  2. Kaweeteerawat C, Chang CH, Roy KR, Liu R, Li R, Toso D, Fischer H, Ivask A, Ji Z, Zink JI, Zhou ZH, Chanfreau GF, Telesca D, Cohen Y, Holden PA, Nel AE, Godwin HA (2015) Cu nanoparticles have different impacts in Escherichia coli and Lactobacillus brevis than their microsized and ionic analogues. ACS Nano 9:7215–7225View ArticleGoogle Scholar
  3. Singh A, Singh NB, Hussain I, Singh H, Singh SC (2015) Plant-nanoparticle interaction: an approach to improve agricultural practices and plant productivity. Int J Pharm Sci Invent 4:25–40Google Scholar
  4. Borisevich VB, Kaplunenko VG, Kosinov NV, Borisevich BV, Sukhonos VP, Khomin NM, Teliatnikov AV, Voloshina NA, Tkachenko SM, Doroshchuk VA, Korzh AV, Litvinenko DI, Kulida MA, Kulinich SL, Borisevich VB Jr, Borisevich IB, Dimchev VA (2012) Nanomaterials and nanotechnologies in the veterinary practice. VD «Avitsena», Kyiv [in Russian]Google Scholar
  5. Kosinov MV, Kaplunenko VG (2008) Method of producing colloidal metallic nanoparticles “blast erosion nanotechnology for producing colloid metallic particles”. UA Patent 29450. [in Ukrainian]
  6. Kosinov MV, Kaplunenko VG (2010) Kaplunenko-Kosinov process for the preparation of carboxylates using nanotechnology. UA Patent 49050. [in Ukrainian]
  7. Kosinov MV, Kaplunenko VG (2008) Method of obtaining the hydrated and carbonated nanoparticles “electroimpulse nanotechnology of obtaining hydrated and carbonated nanoparticles”. UA Patent 35582. [in Ukrainian]
  8. Al-Maali G, Bisko N, Mustafin K, Akhmetsadykov N, Maskeyeva Z, Rakhmetova Z, Suleimenova Z (2014) The influence of the manganese citrates, obtained using aquananotechnologies, on the biomass production of medicinal mushroom Trametes versicolor (L.) Lloyd. Int J Eng Res Appl 4(9):22–25Google Scholar
  9. Yruela I (2005) Copper in plants. Braz J Plant Physiol 17:145–156View ArticleGoogle Scholar
  10. Pilon-Smits EAH, Quinn CF (2010) Selenium metabolism in plants. In: Hell R, Mendel R-R (eds) Cell Biology of Metals and Nutrients, Plant Cell Monographs 17. Springer-Verlag, Berlin Heidelberg, pp 225–241View ArticleGoogle Scholar
  11. Germ M, Stibilj V, Kreft I (2007) Metabolic importance of selenium for plants. Eur J Plant Sci Biotechnol 1:91–97Google Scholar
  12. Vítová M, Bišová K, Hlavová M, Zachleder V, Rucki M, Čížková M (2011) Glutathione peroxidase activity in the selenium-treated alga Scenedesmus quadricauda. Aquat Toxicol 102:87–94View ArticleGoogle Scholar
  13. Hamilton SJ (2004) Review of selenium toxicity in the aquatic food chain. Sci Total Environ 326:1–31View ArticleGoogle Scholar
  14. Zolotariova OK, Shniukova EI, Syvash OO, Mykhailenko NF (2008) Prospects of microalgae utilization in biotechnology. Alterpres, Kyiv [in Ukrainian]Google Scholar
  15. Murchie EH, Lawson T (2013) Chlorophyll fluorescence analysis: a guide to good practice and understanding some new applications. J Exp Bot 64:3983–3998View ArticleGoogle Scholar
  16. Mykhaylenko NF (2005) The modes of glucose action on photosynthesis of Spirulina platensis (Nordst.) Geitl. (Cyanophyta) as revealed by chlorophyll fluorescence analysis. Int J Algae 7:213–227View ArticleGoogle Scholar
  17. Baker NR (2008) Chlorophyll fluorescence: a probe of photosynthesis in vivo. Annu Rev Plant Biol 59:89–113View ArticleGoogle Scholar
  18. Juneau P, El Berdey A, Popovic R (2002) PAM fluorometry in the determination of the sensitivity of Chlorella vulgaris, Selenastrum capricornutum, and Chlamydomonas reinhardtii to copper. Arch Environ Con Tox 42:155–164View ArticleGoogle Scholar
  19. Woolhouse HW (1983) Toxicity and tolerance in the responses of plants to metals. In: Lange OL, Nobel PS, Osmond CB, Ziegler H (eds) Physiological Plant Ecology III. Encyclopedia of Plant Physiology, New Series, Volume 12 C. Springer-Verlag, Berlin Heidelberg New York, pp 245–300View ArticleGoogle Scholar
  20. Bajguz A (2011) Suppression of Chlorella vulgaris growth by cadmium, lead, and copper stress and its restoration by endogenous brassinolide. Arch Environ Con Tox 60:406–416View ArticleGoogle Scholar
  21. Wong SL (1989) Algal assays to interpret toxicity guidelines for natural waters. J Environ Sci Health A24:1001–1010View ArticleGoogle Scholar
  22. Brady D, Letebele B, Duncan JR, Rose PD (1994) Bioaccumulation of metals by Selenastrum and Chlorella algae. Water SA 20:213–218Google Scholar
  23. Mallick N (2004) Copper-induced oxidative stress in the chlorophycean microalga Chlorella vulgaris: response of the antioxidant system. J Plant Physiol 161:591–597View ArticleGoogle Scholar
  24. Hassall KA (1962) A specific effect of copper on the respiration of Chlorella vulgaris. Nature 193:90View ArticleGoogle Scholar
  25. Chen C, Song S, Wen Y, Zou Y, Liu H (2016) Toxicity of Cu (II) to the green alga Chlorella vulgaris: a perspective of photosynthesis and oxidant stress. Environ Sci Pollut Res 23:17910–17918View ArticleGoogle Scholar
  26. Qian H, Li J, Sun L, Chen W, Sheng GD, Liu W, Fu Z (2009) Combined effect of copper and cadmium on Chlorella vulgaris growth and photosynthesis-related gene transcription. Aquat Toxicol 94:56–61View ArticleGoogle Scholar
  27. Melegari SP, Perreault F, Costa RHR, Popovic R, Matias WG (2013) Evaluation of toxicity and oxidative stress induced by copper oxide nanoparticles in the green alga Chlamydomonas reinhardtii. Aquat Toxicol 142–143:431–440View ArticleGoogle Scholar
  28. Abdel-Hamid MI, Skulberg OM (1995) Effect of selenium on the growth of some selected green and blue-green algae. Lakes Reserv Res Manag 1:205–211View ArticleGoogle Scholar
  29. Ekelund NGA, Danilov RA (2001) The influence of selenium on photosynthesis and “light-enhanced dark respiration” (LEDR) in the flagellate Euglena gracilis after exposure to ultraviolet radiation. Aquat Sci 63:457–465View ArticleGoogle Scholar
  30. Sun X, Zhong Y, Huang Z, Yang Y (2014) Selenium accumulation in unicellular green alga Chlorella vulgaris and its effects on antioxidant enzymes and content of photosynthetic pigments. PLoS One 9:e112270View ArticleGoogle Scholar
  31. Wheeler AE, Zingaro RA, Irgolic K, Bottino NR (1982) The effect of selenate, selenite, and sulfate on the growth of six unicellular marine algae. J Exp Mar Biol Ecol 57:181–194View ArticleGoogle Scholar
  32. Kramer DM, Johnson G, Kiirats O, Edwards GE (2004) New fluorescence parameters for the determination of QA redox state and excitation energy fluxes. Photosynth Res 79:209–218View ArticleGoogle Scholar
  33. Juergens MT, Deshpande RR, Lucker BF, Park J-J, Wang H, Gargouri M, Holguin FO, Disbrow B, Schaub T, Skepper JN, Kramer DM, Gang DR, Hicks LM, Shachar-Hill Y (2015) The regulation of photosynthetic structure and function during nitrogen deprivation in Chlamydomonas reinhardtii. Plant Physiol 167:558–573View ArticleGoogle Scholar
  34. Horton P, Ruban AV, Walters RG (1996) Regulation of light harvesting in green plants. Annu Rev Plant Physiol Plant Mol Biol 47:655–684View ArticleGoogle Scholar
  35. Barón M, Arellano JB, López Gorgé J (1995) Copper and photosystem II: a controversial relationship. Physiol Plantarum 94:174–180View ArticleGoogle Scholar
  36. Droppa M, Horváth G (1990) The role of copper in photosynthesis. Crit Rev Plant Sci 9:111–123View ArticleGoogle Scholar
  37. Burda K, Kruk J, Schmid GH, Strzalka K (2003) Inhibition of oxygen evolution in Photosystem II by Cu(II) ions is associated with oxidation of cytochrome b559. Biochem J 371:597–601View ArticleGoogle Scholar
  38. Dewez D, Geoffroy L, Vernet G, Popovic R (2005) Determination of photosynthetic and enzymatic biomarkers sensitivity used to evaluate toxic effects of copper and fludioxonil in alga Scenedesmus obliquus. Aquat Toxicol 74:150–159View ArticleGoogle Scholar
  39. Mohanty N, Vass I, Demeter S (1989) Copper toxicity affects Photosystem II electron transport at the secondary quinone acceptor, QB. Plant Physiol 90:175–179View ArticleGoogle Scholar
  40. Podorvanov VV, Polishchuk AV, Zolotareva EK (2007) Effect of copper ions on the light-induced proton transfer in spinach chloroplasts. Biofizika 52:1049–1053 [in Russian]Google Scholar
  41. Yruela I, Montoya G, Alonso PJ, Picorel R (1991) Identification of the pheophytin-QA-Fe domain of the reducing side of the photosystem II as the Cu(II)-inhibitory binding site. J Biol Chem 266:22847–22850Google Scholar
  42. Couture P, Visser SA, van Coillie R, Blaise C (1985) Algal bioassays: their significance in monitoring water quality with respect to nutrients and toxicants. Schweiz Z Hydrol 47:127–158View ArticleGoogle Scholar


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