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On-line Access: 2014-08-04

Received: 2014-04-30

Revision Accepted: 2014-07-10

Crosschecked: 2014-07-25

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Article info.
1.  Introduction
2.  Materials and methods
3.  Results and discussion
4.  Conclusions
5. Reference List
Open peer comments

Journal of Zhejiang University SCIENCE A 2014 Vol.15 No.8 P.662-670


Phytotoxicity of silver nanoparticles to cucumber (Cucumis sativus) and wheat (Triticum aestivum)*

Author(s):  Di Cui1,2, Peng Zhang1, Yu-hui Ma1, Xiao He1, Yuan-yuan Li1, Yue-chun Zhao2, Zhi-yong Zhang1

Affiliation(s):  1. Key Laboratory for Biological Effects of Nanomaterials and Nanosafety, Key Laboratory of Nuclear Radiation and Nuclear Energy Technology, Institute of High Energy Physics, Chinese Academy of Sciences, Beijing 100049, China; more

Corresponding email(s):   yczhao@scau.edu.cn

Key Words:  Silver nanoparticles, Ag+ , Cucumis sativus L., Triticum aestivum L., Phytotoxicity

Di Cui, Peng Zhang, Yu-hui Ma, Xiao He, Yuan-yuan Li, Yue-chun Zhao, Zhi-yong Zhang. Phytotoxicity of silver nanoparticles to cucumber (Cucumis sativus) and wheat (Triticum aestivum)[J]. Journal of Zhejiang University Science A, 2014, 15(8): 662-670.

@article{title="Phytotoxicity of silver nanoparticles to cucumber (Cucumis sativus) and wheat (Triticum aestivum)",
author="Di Cui, Peng Zhang, Yu-hui Ma, Xiao He, Yuan-yuan Li, Yue-chun Zhao, Zhi-yong Zhang",
journal="Journal of Zhejiang University Science A",
publisher="Zhejiang University Press & Springer",

%0 Journal Article
%T Phytotoxicity of silver nanoparticles to cucumber (Cucumis sativus) and wheat (Triticum aestivum)
%A Di Cui
%A Peng Zhang
%A Yu-hui Ma
%A Xiao He
%A Yuan-yuan Li
%A Yue-chun Zhao
%A Zhi-yong Zhang
%J Journal of Zhejiang University SCIENCE A
%V 15
%N 8
%P 662-670
%@ 1673-565X
%D 2014
%I Zhejiang University Press & Springer
%DOI 10.1631/jzus.A1400114

T1 - Phytotoxicity of silver nanoparticles to cucumber (Cucumis sativus) and wheat (Triticum aestivum)
A1 - Di Cui
A1 - Peng Zhang
A1 - Yu-hui Ma
A1 - Xiao He
A1 - Yuan-yuan Li
A1 - Yue-chun Zhao
A1 - Zhi-yong Zhang
J0 - Journal of Zhejiang University Science A
VL - 15
IS - 8
SP - 662
EP - 670
%@ 1673-565X
Y1 - 2014
PB - Zhejiang University Press & Springer
ER -
DOI - 10.1631/jzus.A1400114

The increasing release of silver (Ag) nanoparticles (NPs) into the environment highlights the importance of exploring the interactions between Ag NPs and plants, which are the basis of most ecosystems. In this study, two plant species, Cucumis sativus L. (cucumber) and Triticum aestivum L. (wheat) were exposed to Ag NPs and ag+ (added as AgNO3) at the germination and vegetative growth stages. Above certain concentrations, Ag NPs and ag+ were toxic to the two plants. However, stimulatory effects were observed on root elongation for the cucumbers that were exposed to Ag NPs at concentrations below 200 mg/L, and ag+ at concentrations below 5 mg/L. The two plants were more susceptible to the toxicity of Ag NPs at the vegetative growth stage than the germination stage. Ag was accumulated in the roots and was subsequently translocated to the shoots after the exposure to Ag NPs. To assess the role of released ag+, we measured the dissolution of Ag NPs in exposure solutions. About 0.03% and 0.01% of Ag NPs were dissolved into a hydroponic solution at the germination stage for cucumber and wheat, respectively; while 0.17% and 0.06% at the vegetative period for cucumber and wheat, respectively. Cysteine, a strong chelating ligand of ag+, could completely eliminate the effects of Ag NPs on cucumber and wheat, suggesting that the phytotoxicity of Ag NPs was possibly caused by the release of ag+.



Darkslateblue:Affiliate; Royal Blue:Author; Turquoise:Article

Article Content

1.  Introduction

 Silver (Ag) nanoparticles (NPs) are increasingly used for their antimicrobial properties in household antiseptic sprays, food packaging, and antimicrobial coatings of medical devices and clothes (Benn and Westerhoff, 2008; Blaser et al., 2008). Ag is considered to be one of the most toxic trace metals (Ratte 1999), and the widespread use of Ag NPs has increased the likelihood of releases into the environment, which underscores the need to assess the impacts of Ag NPs on the ecosystem’s health. Ag NPs are reported to be potentially toxic to bacteria (Morones et al., 2005), algae (Miao et al., 2010), human cells (Jiang et al., 2008; AshaRani et al., 2009), and animal cells (Hussain et al., 2005). Although much evidence has shown that both Ag NPs and Ag+ are toxic, it is unclear whether the toxicity is specifically related to NPs or dissolved forms of Ag from Ag NPs. Choi and Hu (2008) reported that Ag NPs less than 5 nm were more toxic to nitrifying bacteria than dissolved Ag or larger Ag NPs at similar mass concentrations. Yin et al. (2011) showed that the growth inhibition of gum arabic-coated Ag NPs on L. multiflorum was higher compared with the same concentration of Ag+ and Ag NPs which could exert direct toxic effects without dissolution. However, Ag+ released from Ag NPs was reported to inhibit respiratory enzymes and induce oxidative stress through the generation of reactive oxygen species (ROS) (Kim et al., 2009). Miao et al. (2009) found that Ag NPs could inhibit the cell growth, photosynthesis, and chlorophyll production of Thalassiosira weissflogii. These toxic effects were from the released Ag+, which suggested that toxicity was mainly due to the presence of dissolved Ag.

 Plants are the backbone of all life on earth and are an essential resource for human well-being. In the present study, we comparatively investigated the impacts of uncoated Ag NPs and AgNO3 on two agriculturally significant plants, Cucumis sativus L. (cucumber) and Triticum aestivum L. (wheat), at the germination and vegetative growth stages to reveal their phytotoxicities.

2.  Materials and methods

2.1.  Characterization of Ag NPs

 Uncoated Ag NPs were purchased from Sigma-Aldrich with the particle size <100 nm and purity of 99.5%. The size and morphology were determined by a transmission electron microscope (TEM; JEM-200CX, Japan). For TEM sample preparation, a drop of Ag NP suspension (diluted by ethanol) was dripped onto the copper grid after sonication for 30 min. After drying at room temperature, the sample was placed in a specimen holder. Hydrodynamic diameters and zeta potential of Ag NPs were measured by a dynamic light scattering equipment (ZetaSizer 90, Nano series, UK). For the sample preparation, Ag NPs were dispersed in deionized (DI) water and nutrient solution (1/4 strength Hoagland’s solution), sonicated for 30 min following by their immediate measurement in a plastic cuvette (path length 1 cm). The pH values of Ag NP suspensions dispersed in DI water and nutrient solution were 6.9 and 5.5, respectively.

2.2.  Root elongation assay

 Seeds of cucumber and wheat were purchased from the Chinese Academy of Agricultural Sciences and kept in a refrigerator (4 °C) until use. The seeds were pretreated in a 10% (v/v) sodium hypochlorite solution for 10 min and then rinsed for three times with DI water to ensure surface sterility. Different concentrations of Ag NPs were prepared and dispersed by ultrasonic treatment in DI water for 30 min before use. Then the seeds were soaked in Ag NP suspensions or AgNO3 solutions for 2 h. One piece of filter paper was put into each Petri dish (100 mm×15 mm), and 5 ml of the test solution or suspension was immediately added after ultrasonic treatments. Then 14 seeds were transferred onto each filter paper, and Petri dishes were sealed with parafilm, and placed in the dark under 25 °C in a climate incubator. After 5-d treatment, the germination was halted. Root lengths were measured with a meter ruler.

2.3.  Biomass assay

 Seeds of cucumber and wheat were germinated on filter papers moistened with DI water at 25 °C after sterilization and water soaking (Lin and Xing 2007). After 3 d, the uniform seedlings were transplanted into 250 ml beakers containing 100 ml of 1/4 strength Hoagland’s solution and each seedling was anchored by plastic foam with a hole in the center. The growth was conducted in a climate incubator for 10 d at a day/night humidity of 50%/70%, day/night temperature of 27 °C/18 °C, and a 16 h photoperiod (light intensity of 1.76×104 lux) before the phytotoxicity study. Ag NPs with or without cysteine were then added into the nutrient solution followed by ultrasonic pretreatment for 30 min. We tested the effects of Ag NPs alone (1, 5, 20, 50, and 100 mg/L), 100 mg/L Ag NPs+112 mg/L cysteine (molar ratio of cysteine:Ag=1:1), and cysteine alone (112 mg/L) on the growth of the cucumber and wheat seedlings. To maintain a constant volume (100 ml), the solution in each beaker was replenished with fresh nutrient solution every other day. There were six replicates for each treatment. The seedlings were allowed to further grow for three weeks. At the end of the growth period, the seedlings of cucumber and wheat were harvested and washed thoroughly with flowing tap water and DI water. Tissues were collected and biomasses were measured after drying to a constant weight at 70 °C for 48 h.

2.4.  Determination of Ag content

 After the above treatments, Ag+ concentrations in Ag NP suspensions were measured by an inductively coupled plasma-mass spectrometer (ICP-MS) (Thermo X7, USA) after centrifugation (14 000g for 10 min) and ultrafiltration (0.22 μm, polyethersulfone resins filter).

 The content of Ag in plant tissues was measured by ICP-MS after HNO3/H2O2 (v/v=4:1) digestion on a heating plate. Indium (100 ng/ml) was used as an internal standard to compensate for signal drifting and matrix suppression. The certified reference material GBW07602 (bush leaves and branches) was digested to examine the recovery. The recovery of Ag from GBW07602 was 98.9% and the spike recovery averaged 103%. The relative standard deviation (SD) was 2.3%, and the detection limit was 0.01 ng/ml.

2.5.  TEM examination

 Fresh roots of cucumber and wheat from the control and the treatments of 2000 mg/L of Ag NPs after 3-week exposure were observed by TEM to detect if Ag NPs could enter the plant cells. Roots were thoroughly washed with DI water. Samples for TEM were prepared following standard procedures (Bozzola and Russell, 1999). The root apexes (4 mm) were cut and prefixed in 2.5% glutaraldehyde, washed in a phosphate buffer (0.05 mol/L, pH 7.8), post-fixed in osmium tetroxide (10 g/L in 0.1 mol/L sodium phosphate buffer) for 1 h, dehydrated in graded acetone, and infiltrated and embedded in Spurr’s resin. The cross sections (90-nm thick) below root tips were cut for TEM using a UC6i ultramicrotome (Leica, Austria) with a diamond knife. TEM was operated at 80 kV on a JEM-1230. More than 10 sections cut from different roots were examined.

2.6.  Statistical analysis

 Data processing was performed on SPSS V17.0. One-way analysis of variance (ANOVA) followed by Tukey’s honestly significant difference (HSD) or Bonferroni test was performed to examine the statistical differences. Data were expressed as mean±SD, and P<0.05 was considered to be significantly different.

3.  Results and discussion

3.1.  Characterization of Ag NPs

 The average size of Ag NPs was (13.8±2.5) nm according to the TEM image (Fig. 1). The Ag NPs hydrodynamic diameters in the DI water and nutrient solution were (711.8±25.3) and (736.4±32.2) nm, respectively. Zeta potentials of the Ag NPs in the DI water and nutrient solution were (4.8±1.0) and (−9.6±0.5) mV, respectively.

TEM image of Ag NPs

3.2.  Effects of Ag on root elongation during the seed germination stage

 Both Ag NPs and Ag+ were toxic to cucumber and wheat plants at high exposure concentrations (Fig. 2). At the same concentrations, the plants were more sensitive to the effects of Ag+ than Ag NPs. Interestingly, Ag NPs and Ag+ showed stimulatory effects on root elongation of cucumber at low concentrations. Similar results have been reported previously. Wang et al. (2013) found that all forms of Ag (NPs and Ag+) were toxic to Arabidopsis and Populus above a specific concentration, but a stimulatory effect was observed on root elongation, fresh weight, and evapotranspiration of both plants at sub-lethal concentrations. They attributed this response to hormesis, a biphasic dose response in which the presence of low doses of toxicants can activate repair mechanisms to overcompensate for the exposure. However, in this study, it seems that the hormesis effects of Ag NPs and Ag+ were species-specific because no significant stimulatory effects on the root elongation of wheat were observed at all the exposure concentrations.

Effects of Ag NPs and Ag+ on the root elongation of cucumber and wheat after 5-d exposure at the germination stage
(a) Ag NPs on cucumber; (b) Ag+ on cucumber; (c) Ag NPs on wheat; (d) Ag+ on wheat. Data are given as mean±SD. * P<0.05 vs. control

3.3.  Effects of Ag NPs on biomass during the vegetative period

 The phytotoxicity of Ag NPs on cucumber and wheat during the vegetative period was evaluated at concentrations of 1, 5, 20, 50, and 100 mg/L. The dry biomasses of cucumber roots were remarkably reduced by Ag NPs at 50 and 100 mg/L after three weeks treatment compared with the control (P<0.05) (Fig. 3a). Cucumber shoots were less sensitive to Ag NPs than the roots, and no significant inhibitive effects were observed (P>0.05). As for wheat, Ag NPs significantly decreased the dry biomass of shoots at high concentrations (20–100 mg/L) but showed no significant effects on the dry biomass of roots (P>0.05) (Fig. 3b). Similar effects were observed for polar, with the leaf and stem biomass being restrained by Ag+ but having no effect on the root (Wang et al., 2013). The inhibition thresholds and degrees at this stage are both different from those at the germination stage, indicating that the susceptibility to toxic compounds of a plant is growth stage dependent. Longer time exposure to NP suspensions during the vegetative period than the germination stage might be another reason, which implied that NPs need a longer period to affect plant growth. Thus, the impact of NPs on plant growth may require a relatively long exposure time to determine sublethal effects (Gubbins et al., 2011).

Effects of Ag NPs, Ag NPs+cysteine, and cysteine on the dry biomasses of root and shoot of cucumber (a) and wheat (b) after three weeks exposure during the vegetative period
Treatment: 1, 5, 20, 50, and 100 are the Ag NPs in mg/L; 100+cys is the 100 mg/L Ag NPs+112 mg/L cysteine; cys is the 112 mg/L cysteine. Data are given as mean±SD.* P<0.05 vs. control

3.4.  Ag+ released in solution

 Rhizosphere mucilage and root exudates, such as organic acids and amino acids, could promote the adsorption of NPs on the root surface and bring about NPs dissolution, oxidation, or reduction (Cañas et al., 2008; Lin and Xing, 2008). Toxicity of the dissolved form might be a possible mechanism for the toxicity of metal-based NPs, including Ag, Ni, Cu, ZnO, and La2O3 (Limbach et al., 2007; Griffitt et al., 2008; Miao et al., 2009; Ma et al., 2011). Ag+ is known to alter the perception and/or responses to phytohormones and further to affect plant growth (Zhao et al., 2002; Binder et al., 2007; Strader et al., 2009). Recently, toxicity of Ag NPs has been frequently attributed, at least in part, to the release of Ag+ at the surface of NPs (Pal et al., 2007; Navarro et al., 2008; Miao et al., 2009). To assess the role of released Ag+, we first measured the dissolution of Ag NPs in exposure solutions, both at the end of the seed germination stage and vegetative period. After 5-d exposure of 1–1000 mg/L of Ag NPs at the germination stage for cucumber and wheat, the released Ag+ into the hydroponic solution was about 2–167 and 0.7–60 μg/L, respectively (Figs. 4a and 4b). That is about 0.03% of Ag NPs dissolved into the hydroponic solution of cucumber, two folds more than that of wheat. The difference in dissolution quantities of the two plant species may be attributed to the more developed root systems and the subsequent larger root surface areas of the cucumber than those of the wheat. It is worth noting that, Ag+ concentrations in the solutions for vegetative toxic tests were about two times more than the germination stage, 4–103 μg/L for cucumber and 2–41 μg/L for wheat (Figs. 4c and 4d), respectively. This is probably because of the larger root surface, larger quantity of root exudates, and longer interaction time between the Ag NPs and the root exudates during the vegetative period compared to the germination stage, so the more Ag+ released seemed to be inevitable.

Free ion concentrations in exposure solutions of Ag NPs at different stages
After 5-d treatment of Ag NPs at the germination stage of cucumber (a) and wheat (b); after 3-week treatment of Ag NPs during the vegetative period of cucumber (c) and wheat (d). Data are given as mean±SD

 The phytotoxicity induced by the released Ag+ after 5-d treatment during the germination stage was explored. Exposure to Ag NPs at 1000 mg/L (including 0.160 mg/L of released Ag+ in the hydroponic solution) significantly decreased the root elongation of cucumber (Fig. 2a). Yet exposure to Ag+ alone at 0.2 mg/L, which is similar to the concentration of Ag+ released by 1000 mg/L Ag NPs, had a stimulatory effect (Fig. 2b). Similarly, the root growth of wheat was dramatically inhibited by the presence of Ag NPs at 1000 mg/L (60 μg/L released Ag+) (Fig. 2c), but the measured Ag+ in these hydroponic solutions was too low to account for the observed inhibiting effects. Similar phenomenon was observed by Wang et al. (2013). Superficially, some NP-specific effects were likely to exert. However, an important fact herein seemed to be ignored that the Ag+ ion concentrations in the rhizosphere solutions might be higher than that in the exposure solutions. Ag NPs were adsorbed on the root surface with the aid of mucilage and there is an imbalance between oxidation and reduction in the microenvironment named rhizosphere. The concentration of released Ag+ we measured in the culture suspensions (with plants cultured) could be far less than that on the root surfaces. The nano-bio interface was the main location of the dissolution. Zhang et al. (2012) found that concentrations of Yb3+ in the rhizosphere solutions were indeed higher than that in the exposure solutions.

 The dissolution of Ag NPs in the culture medium, as well as the possible formation of NPs from Ag+ on root surfaces makes it difficult to differentiate ionic effects from NP-specific effects (Gardea-Torresdey et al., 2003; Geisler-Lee et al., 2013). As a strong Ag+ chelating ligand, cysteine has been proven to be useful in examining the contribution of Ag+ to the overall toxicity of Ag NPs (Navarro et al., 2008). Thus, the role of Ag+ in determining the phytotoxicity of Ag NP suspensions was assessed in the presence of cysteine. The complete abolishment of the impact on the root elongation at the germination stage by cysteine indicated that the protective effects of cysteine were due to its chelating with Ag+ in the exposure media, which resulted in a reduced Ag bioavailability (Fig. 5). Similar phenomenon appeared after three weeks of exposure at the vegetative period of the cucumber, when cysteine completely eliminated the inhibition of 100 mg/L of Ag NPs on the biomass (cysteine alone did not show any significant effect) (Fig. 3b). As for the cucumber, cysteine alone reduced the biomass possibly because of the high sensitivity to cysteine (Fig. 3a). However, cysteine still somewhat alleviated the toxicity of 100 mg/L of Ag NPs to the biomass of the cucumber. This strongly emphasized the fact that Ag NPs contributed to the toxicity by serving as a source of Ag+. He et al. (2012) discovered that cysteine completely removed the inhibitory effects of Ag NPs on the metabolic activity of Chattonella marina, which suggested that the toxicity of Ag NPs was due to the release of Ag+.

Effect of cysteine on the root elongation of cucumber (a) and wheat (b) after 5-d exposure of Ag NPs at the germination stage
C: control. Data are given as mean±SD. Pure cysteine (112 mg/L) did not show any effect on root elongation (P>0.05)

3.5.  Uptake and translocation of Ag NPs in cucumber and wheat

 TEM images of the cross sections of cucumber and wheat roots after 3-week exposure of 100 mg/L Ag NPs are shown in Fig. 6. In contrast to the control (Figs. 6a and 6c), high electron-dense deposits can be found in the cell wall and cytoplasm in sections of 100 mg/L Ag NPs treated groups (Figs. 6b and 6d).

TEM images of root cross sections from untreated (a) and Ag NP treated (b) cucumber, and untreated (c) and Ag NP treated (d) wheat after three weeks during the vegetative period
Ag NP was treated at 100 mg/L. Arrows indicated Ag-enriched areas

 Ag contents in cucumber and wheat tissues after three weeks treatments of Ag NPs are shown in Fig. 7. Total Ag contents increased with the increasing concentrations of Ag NPs in the exposure solutions. The majority of Ag was accumulated in the roots. Translocation factors (TFs) of Ag, defined as the Ag content ratio of the shoot to root, were very low (0.001–0.007) in cucumber and wheat with the treatments of Ag NPs. It seems that only a little Ag NPs or Ag+ were transported from the roots to shoots in this study. This might be because most of the Ag NPs were adsorbed on the root surface, and only a little Ag could move into the stele and was available for upward transport. It can be seen that the TF obtained in the cucumber were three times higher than those in wheat (Figs. 7c and 7d). The better transportation capability in cucumber probably resulted from the greater blade area and stronger evaporative power than in wheat.

Ag content in tissues of cucumber (a) and wheat (b) after three weeks of exposure of Ag NPs and the translocation factors (TFs) of Ag in cucumber (c) and wheat (d)
Data are given as mean±SD. The same letters above the bars in (c) and (d) were not significantly different (P>0.05)

4.  Conclusions

 Based on total Ag concentrations, it was observed that Ag+ displayed stronger effects on cucumber and wheat than Ag NPs at the germination stage. Meanwhile, the same concentration of Ag with different species (Ag NPs or Ag+) exerted different influences between the two stages. Thus, the developmental period of the plant should also be considered when assessing the risks posed by NPs in the environment.

 This study revealed the determinant role of dissolved Ag+ on the toxicity of Ag NPs for cucumber and wheat, and the protective effect of cysteine was attributed to its chelation with Ag+. Results of ICP-MS and TEM indicated that Ag (Ag NPs or other forms) could be absorbed by the roots and translocated to the shoots. The low translocation factors of Ag in the two plants suggested that the movement of Ag from the roots to shoots was difficult.

* Project supported by the National Key Basic Research Program of China (Nos. 2011CB933400 and 2013CB932703), the Special Fund for the Public Interest Research of China (No. 201209012), and the National Natural Science Foundation of China (Nos. 11275215, 11275218, and 11375009)


[1] AshaRani, P.V., Low Kah Mun, G., Hande, M.P., 2009. Cytotoxicity and genotoxicity of silver nanoparticles in human cells. ACS Nano, 3(2):279-290. 

[2] Benn, T.M., Westerhoff, P., 2008. Nanoparticle silver released into water from commercially available sock fabrics. Environmental Science and Technology, 42(11):4133-4139. 

[3] Binder, B.M., Rodriguez, F.I., Bleecker, A.B., 2007. The effects of Group 11 transition metals, including gold, on ethylene binding to the ETR1 receptor and growth of Arabidopsis thalianaFEBS Letters, 581(26):5105-5109. 

[4] Blaser, S.A., Scheringer, M., MacLeod, M., 2008. Estimation of cumulative aquatic exposure and risk due to silver: contribution of nano-functionalized plastics and textiles. Science of The Total Environment, 390(2-3):396-409. 

[5] Bozzola, J.J., Russell, L.D., 1999. Electron Microscopy: Principles and Techniques for Biologists, Jones & Bartlett Learning,:

[6] Cañas, J.E., Long, M., Nations, S., 2008. Effects of functionalized and nonfunctionalized single-walled carbon nanotubes on root elongation of select crop species. Environmental Toxicology and Chemistry, 27(9):1922-1931. 

[7] Choi, O., Hu, Z., 2008. Size dependent and reactive oxygen species related nanosilver toxicity to nitrifying bacteria. Environmental Science and Technology, 42(12):4583-4588. 

[8] Gardea-Torresdey, J.L., Gomez, E., Peralta-Videa, J.R., 2003. Alfalfa sprouts: a natural source for the synthesis of silver nanoparticles. Langmuir, 19(4):1357-1361. 

[9] Geisler-Lee, J., Wang, Q., Yao, Y., 2013. Phytotoxicity, accumulation and transport of silver nanoparticles by Arabidopsis thalianaNanotoxicology, 7(3):323-337. 

[10] Griffitt, R.J., Luo, J., Gao, J., 2008. Effects of particle composition and species on toxicity of metallic nanomaterials in aquatic organisms. Environmental Toxicology and Chemistry, 27(9):1972-1978. 

[11] Gubbins, E.J., Batty, L.C., Lead, J.R., 2011. Phytotoxicity of silver nanoparticles to Lemna minor L. Environmental Pollution, 159(6):1551-1559. 

[12] He, D., Dorantes-Aranda, J.J., Waite, T.D., 2012. Silver nanoparticle algae interactions: oxidative dissolution, reactive oxygen species generation and synergistic toxic effects. Environmental Science and Technology, 46(16):8731-8738. 

[13] Hussain, S., Hess, K., Gearhart, J., 2005.  In vitro toxicity of nanoparticles in BRL 3A rat liver cells. Toxicology in Vitro, 19(7):975-983. 

[14] Jiang, W., Kim, B.Y., Rutka, J.T., 2008. Nanoparticle-mediated cellular response is size-dependent. Nature Nanotechnology, 3(3):145-150. 

[15] Kim, S., Choi, J.E., Choi, J., 2009. Oxidative stress-dependent toxicity of silver nanoparticles in human hepatoma cells. Toxicology in Vitro, 23(6):1076-1084. 

[16] Limbach, L.K., Wick, P., Manser, P., 2007. Exposure of engineered nanoparticles to human lung epithelial cells: influence of chemical composition and catalytic activity on oxidative stress. Environmental Science and Technology, 41(11):4158-4163. 

[17] Lin, D.H., Xing, B.S., 2007. Phytotoxicity of nanoparticles: inhibition of seed germination and root growth. Environmental Pollution, 150(2):243-250. 

[18] Lin, D.H., Xing, B.S., 2008. Root uptake and phytotoxicity of ZnO nanoparticles. Environmental Science and Technology, 42(15):5580-5585. 

[19] Ma, Y.H., He, X., Zhang, P., 2011. Phytotoxicity and biotransformation of La2O3 nanoparticles in a terrestrial plant cucumber (Cucumis sativus). Nanotoxicology, 5(4):743-753. 

[20] Miao, A.J., Schwehr, K.A., Xu, C., 2009. The algal toxicity of silver engineered nanoparticles and detoxification by exopolymeric substances. Environmental Pollution, 157(11):3034-3041. 

[21] Miao, A.J., Luo, Z., Chen, C.S., 2010. Intracellular uptake: a possible mechanism for silver engineered nanoparticle toxicity to a freshwater alga Ochromonas danicaPLoS ONE, 5(12):e15196

[22] Morones, J.R., Elechiguerra, J.L., Camacho, A., 2005. The bactericidal effect of silver nanoparticles. Nanotechnology, 16(10):2346

[23] Navarro, E., Piccapietra, F., Wagner, B., 2008. Toxicity of silver nanoparticles to Chlamydomonas reinhardtiiEnvironmental Science and Technology, 42(23):8959-8964. 

[24] Pal, S., Tak, Y.K., Song, J.M., 2007. Does the antibacterial activity of silver nanoparticles depend on the shape of the nanoparticle? A study of the gram-negative bacterium Escherichia coliApplied and Environmental Microbiology, 73(6):1712-1720. 

[25] Ratte, H.T., 1999. Bioaccumulation and toxicity of silver compounds: a review. Environmental Toxicology and Chemistry, 18(1):89-108. 

[26] Strader, L.C., Beisner, E.R., Bartel, B., 2009. Silver ions increase auxin efflux independently of effects on ethylene response. The Plant Cell, 21(11):3585-3590. 

[27] Wang, J., Koo, Y., Alexander, A., 2013. Phytostimulation of poplars and Arabidopsis exposed to silver nanoparticles and Ag+ at sublethal concentrations. Environmental Science and Technology, 47(10):5442-5449. 

[28] Yin, L., Cheng, Y., Espinasse, B., 2011. More than the ions: the effects of silver nanoparticles on Lolium multiflorumEnvironmental Science and Technology, 45(6):2360-2367. 

[29] Zhang, P., Ma, Y.H., Zhang, Z.Y., 2012. Comparative toxicity of nanoparticulate/bulk Yb2O3 and YbCl3 to cucumber (Cucumis sativus). Environmental Science and Technology, 46(3):1834-1841. 

[30] Zhao, X.C., Qu, X., Mathews, D.E., 2002. Effect of ethylene pathway mutations upon expression of the ethylene receptor ETR1 from ArabidopsisPlant Physiology, 130(4):1983-1991. 

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