Investigations of the Toxic Effect of Silver Nanoparticles on Mammalian Cell Lines

Sambale, F.; Wagner, S.; Stahl, F.; Khaydarov, R. R.; Scheper, T.; Bahnemann, D.

doi:https://doi.org/10.1155/2015/136765

Journal of Nanomaterials

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Abstract Introduction Materials and Methods Results Discussion Conclusions Acknowledgments References Copyright Related Articles

Research Article | Open Access

Volume 2015 | Article ID 136765 | https://doi.org/10.1155/2015/136765

Investigations of the Toxic Effect of Silver Nanoparticles on Mammalian Cell Lines

F. Sambale,¹S. Wagner,¹F. Stahl,¹R. R. Khaydarov,²T. Scheper,¹and D. Bahnemann¹

Academic Editor: William W. Yu

Received10 Dec 2014

Revised09 Feb 2015

Accepted09 Feb 2015

Published24 Feb 2015

Abstract

Silver nanoparticles are widely used for many applications. In this study silver nanoparticles have been tested for their toxic effect on fibroblasts (NIH-3T3), on a human lung adenocarcinoma epithelial cell line (A-549), on PC-12-cells, a rat adrenal pheochromocytoma cell line, and on HEP-G2-cells, a human hepatocellular carcinoma cell line. The viability of the cells cultivated with different concentrations of silver was determined by the MTT assay, a photometric method to determine cell metabolism. Dose-response curves were extrapolated and IC₅₀, total lethal concentration (TLC), and no observable adverse effect concentration (NOAEC) values were calculated for each cell line. As another approach, ECIS (electric-cell-substrate-impedance-sensing) an automated method to monitor cellular behavior in real-time was applied to observe cells cultivated with silver nanoparticles. To identify the type of cell death the membrane integrity was analyzed by measurements of the lactate dehydrogenase releases and by determination of the caspase 3/7 activity. To ensure that the cytotoxic effect of silver nanoparticles is not traced back to the presence of Ag⁺ ions in the suspension, an Ag⁺ salt (AgNO₃) has been examined at the same concentration of Ag⁺ present in the silver nanoparticle suspension that is assuming that the Ag particles are completely available as Ag⁺ ions.

1. Introduction

Recently nanotechnology has revolutionized the technological progress and is predicted to be one of the key technologies of the 21st century [1]. Nanoparticles are defined with a particle size between 1 and 100 nm. Compared to their bulk counterparts, nanoparticles exhibit different physical and chemical properties. Many properties that are found to change in the nanoscale, for example, physical characteristics, surface area, magnetic, mechanical, optical as well as chemical properties such as reactivity, thermal properties, and so forth. Because of their new properties many of these newly developed nanomaterials are already used in different industries. Typical application fields are, for example, optics, photocatalysis, automotive industry, water and air treatment, fabrics, cosmetics, and health products [1].

Silver has been known for its antibacterial effect for a long time [2]. In ancient Greece, Rome, and Macedonia, silver was used to control infections. Nowadays, silver is used for many bactericidal applications, for example, wound healing [3], water treatment [4], and flower preservation [5]. Other application fields of silver nanoparticles include catalysis [6], optics [7, 8], electronics [9], and various other areas of science and technology. Currently the most effective application for silver nanoparticles appears to be their usage as antibacterial/antifungal agent [10, 11]. The manufacturing of bactericidal cotton fibers containing silver nanoparticles for textile industry [12, 13] is of great interest, because ordinary cotton fabrics provide an excellent environment for microorganisms [14]. Further applications for silver nanoparticles are paints; for example, nanosilver-based paint should prevent the growth of algae on outside walls [15].

However, at present concerns have been raised concerting the environmental impact of nanoparticles and the possible human exposure. Nanomaterial risk assessment is mainly influenced by the mobility of nanoparticles [1]. In addition, due to the large surface area of nanoparticles pollutants can be adsorbed to nanoparticles. During nanomaterials development accumulation of nanoparticles in the ground water or in the air can occur [1]. As nanoparticles such as silver nanoparticles can be absorbed by plants or other living organisms, the particles can reach the food chain [1]. There are a lot of publications reporting the results of investigations of the antibacterial effect of silver nanoparticles. Sotiriou and Pratsinis examined the antibactericidal activity of silver ions and nanosilver particles and reported that the bactericidal activity against gram negative Escherichia coli bacteria is dominated by Ag⁺ ions and not by the silver nanoparticles themselves [16]. Fabrega et al. investigated the effect of colloidal Ag nanoparticles at different pH values in the presence of Suwannee River humic acids (SRHA) against Pseudomonas fluorescens SBW25 and observed a toxic effect at a concentration of 2000 ppm without SRHA at pH 9 [17]. The effect of silver nanoparticles on aquatic organisms has also been investigated by different research groups [18, 19]. Until ten years ago it was assumed that silver is nontoxic to mammalian cells, except for argyria, a blue coloration of the skin, caused by colloidal silver [20].

The main nanoparticle uptake possibilities into the human body were via the skin, via the respiratory tract, or via the gastrointestinal tract [1]. Thereby, nanoparticle size, shape, and surface modification play an important role in the distribution in the organism. Nanoparticles absorbed via the respiratory tract can reach the lymph stream and the blood circulation [21]. Some studies showed that nanoparticles are able to pass through the blood-brain-barrier [22] and through cell membranes [23, 24] and can thus deposit in organs and interact with biological systems.

It has been shown that silver nanoparticles can induce a toxic response of different mammalian cell lines [25–29]. Hence silver nanoparticle exposure resulted in a decreased viability or the release of lactate dehydrogenase in rat liver cells [28], in mouse germline stem cells [27], in human fibroblasts [30], and in rat adrenal cells [31]. Chairuangkitti et al. investigated in vitro toxic effects of silver nanoparticles on human lung carcinoma (A-549) cells and reported a clear relationship to the generation of reactive oxygen species [25]. Kawata et al. investigated the toxic effect of silver nanoparticles in comparison to silver ions and polystyrene nanoparticles which are known as nontoxic nanomaterials to HEP-G2 cells. They contributed the toxic effect to both, the nanosize of these particles as well as the ionic form Ag⁺ [32]. AshaRani et al. investigated the cytotoxic and genotoxic effect of silver nanoparticles on human cells. Their results indicated mitochondrial dysfunction as well as induction of reactive oxygen species (ROS) by Ag-nanoparticles which result in DNA damage and chromosomal aberrations [33]. The induced toxic effects of silver nanoparticles can be divided into ROS-dependent and ROS-independent pathways [25].

Because silver nanoparticles are used in many application fields and previous studies showed the possible hazardous effects of these materials it is important to investigate the toxic action more intensely. Therefore, we have investigated the toxic effect of silver nanoparticles and silver ions on four commonly used cell lines, concentrating on the possible exposure options to the organism. The viability of the cells cultivated in the presence of different concentrations of Ag nanoparticles and Ag⁺ ions was measured employing the MTT assay, a well-established photometric method to determine the cell metabolism. Dose-response curves were extrapolated from these data and Total Lethal Concentration (TLC), No Adverse Effect Concentration (NOAEC), and IC₅₀-values were calculated. Electric-Cell-Substrate-Impedance-Sensing (ECIS), an automated method to monitor cell behavior in real-time, was also carried out. To investigate the cell death the caspase 3/7 activity assay was performed.

2. Materials and Methods

2.1. Silver Nanoparticles and Silver Ions

The silver nanoparticles used for the cytotoxic tests were synthesized by the Institute of Nuclear Physics, in Tashkent, Uzbekistan. They were liberated from pure silver electrodes via 12 V battery-operated constant current generators. The apparatus used for silver ion generation has been described previously [34]. The water-based colloidal silver solution was obtained by a recently reported three-stage process based on the electroreduction of silver ions in water [35]. The concentration of silver nanoparticles and ions in solution was determined by neutron activation analysis (NAA) [36]. Samples were irradiated in the nuclear reactor of the Institute of Nuclear Physics (Tashkent, Uzbekistan). The product of nuclear reaction ¹⁰⁹Ag(n,γ)^110mAg has the half-life days.

Through measurements of the intensity of gamma radiation with an energy of 0.657 MeV and 0.884 MeV emitted by ^110mAg. A Ge(Li) detector with a resolution of about 1.9 keV at 1.33 MeV the silver concentration was determined. A 6144-channel analyzer was used for recording gamma-ray quanta. The silver nanoparticles used in the study were characterized by Khaydarov et al. and obtained a primary particle size of nm (TEM) [35]. As reference for the cytotoxic testing a silver ion suspension was used (AgNO₃) at the same total Ag concentration.

2.2. Dynamic Light Scattering Measurements

To measure the hydrodynamic diameter and the distribution of the silver nanoparticles in water, dynamic light scattering (DLS) measurements were performed. Suspensions (1 mL) with a concentration of 10 ppm in water were prepared and then measured with a Malvern Zetasizer Nano-ZS (Malvern Instruments, UK). Each measurement was repeated three times to enable the calculation of a standard deviation.

2.3. Cell Culture

Four different cell lines were cultivated: HEP-G2 cells, NIH-3T3 cells, PC-12 cells, and A-549 cells. HEP-G2 cells are human hepatocellular carcinoma cells (DMSZ number: ACC 180), NIH-3T3 cells are mouse fibroblasts (DMSZ number: ACC 59), PC-12 cells are rat adrenal pheochromocytoma cells (DSMZ number: ACC 159), and A-549 cells are human lung carcinoma cells (DSMZ number: ACC 107). All cell lines were cultivated in Dulbecco’s Modified Eagle’s medium (DMEM) (D7777 Sigma-Aldrich, Steinheim, Germany) supplemented with the respective serum (Table 1) and 1% antibiotics (penicillin/100 U/mL and streptomycin/100 μg/mL) in a humidified environment at 37°C/5% CO₂. After three to four days the cells had grown to approximately 70% confluence. Afterwards, they were detached with trypsin and cultured in a new cell culture flask.

2.4. Cultivation with Nanoparticle Addition

Depending on the doubling times, the cells were seeded a defined number of cells (see Table 1) in a 96-well plate and were incubated for three days. At day four the medium of each well was removed and 200 μL of the different nanoparticle suspensions in varying concentrations in the cell culture medium was added to the wells. The cells were cultivated for three more days after which the viability of the cells was determined by the (3-(4,5-dimethylthiazol-2-yl)-2,5-diphenyl-tetrazolium-bromid)-assay. Moreover the caspase 3/7 activity was measured with the Apo-ONE Homogeneous Caspase-3/7 Assay (Promega, USA) or the lactate dehydrogenase release was determined with the CytoTox-ONETM Homogeneous Membrane Integrity Assay (Promega, USA).

2.5. Cytotoxicity Test Methods

2.5.1. MTT-Assay

The viability of the cells was analyzed by the MTT assay (Sigma-Aldrich, Steinheim, Germany). This assay is based on the reaction of the tetrazonium ring by mitochondrial dehydrogenase enzymes and leads to an insoluble blue reaction product [37]. Firstly, the medium was removed from each well. Secondly, 100 μL of fresh medium and 10 μL of MTT solution (5 mg/mL PBS, sterile) were added to each well and incubated for 4 h at 37°C/5% CO₂. After incubation of the dye 100 μL of 10% SDS in 0.01 M HCl were added and the plates were further incubated for 24 h. The determination of the transmission signals at 570/630 nm was performed using a microplate reader (Bio-Rad, Munich, Germany). Each measurement was repeated three times independently in quintuple to calculate the standard error. Statistical analysis was performed using the Student’s -test.

2.5.2. Electric-Cell-Substrate-Impedance-Sensing

ECIS is an automated method to monitor cellular behavior. Cells are grown on electrodes covered with a gold film and an alternating current (AC) signal is applied. As cells attach and spread upon these electrodes, their insulating membranes block and constrain the current flow resulting in measured variations in the electrode impedance. Any changes in the environment that result in morphological changes of the cells alter the current paths and can be readily detected by the ECIS model 1600R (Applied BioPhysics, USA). To implement this experiment, one 8W1E (8 wells, 1 electrode) ECIS slide was incubated for about 24 h with cell culture medium, with each well of the slide being filled with 400 μL of medium. Afterwards, the medium was removed and 125,000 A-549 cells in 400 μL were seeded per well and two electrodes remained cell-free as reference. When the impedance signal was stable, the cells had grown to confluence, the medium was removed, and 400 μL of the silver nanoparticle suspension in the culture medium at a concentration of 10 ppm was added to the wells. For each analysis, two wells were filled with the same suspension and three wells were filled with cell culture medium without nanoparticles as a reference. The impedance signal is monitored during the entire time of the measurement which is terminated when the signals do not change anymore.

2.6. Dose-Response-Curves

From the results obtained from the MTT assay, dose-response-curves were plotted for the determination of the “No Observable Adverse Effect Concentration” (NOAEC), the Inhibitory Concentration (IC₅₀), and the Total Lethal Concentration (TLC) values. For this the normalized cell viability (viability of cells in normal culture medium = 1) was plotted as a function of the logarithm of the particle or rather the ion concentration in ppm. The theoretical dose-response curves were extrapolated using the following equation: with = curve slope, = IC₅₀ value [ppm], and being the absorbance values expressed as percentage cell viability.

NOAEC values were determined with being 95% of the maximum response on the normalized cell viability employing the following equation: TLC values were determined with being 5% of the maximum response on the normalized cell viability with the following equation:

2.7. Caspase 3/7 Activity

The cells were cultivated in 96-well plates. The caspase 3/7 activity was measured with the Apo-ONE Homogeneous Caspase 3/7 Assay (Promega, USA). To perform this test 100 μL of the Apo-ONE Caspase 3/7 Reagent was added to each well of the 96-well plate. The plate was shaken for 1 minute at 400 rpm and was then incubated at 22°C. Every 10 minutes the fluorescence with an excitation wavelength of 485 nm and an emission wavelength of 538 nm was measured with the Fluoroskan Ascent (Thermo Electron Corporation). Three independent experiments were performed to calculate the standard error.

2.8. Lactate Dehydrogenase Assay (LDH)

The cells were cultivated in 96-well plates. The membrane integrity of the cells was analyzed by the CytoTox-ONETM Homogeneous Membrane Integrity Assay (Promega, USA). To perform the assay 100 μL medium from each well was transferred into a new well of a 96-well plate. This plate was incubated for 20 minutes at 22°C. Afterwards, 100 μL of the CytoTox-One reagent was added to each plate. Then the plate was shaken and the fluorescence with an excitation wavelength of 560 nm and an emission wavelength of 590 nm was measured with the Fluoroskan Ascent (Thermo Electron Corporation).

3. Results

3.1. DLS Measurements

To identify the diameter of the silver nanoparticles used for the cytotoxicity measurements DLS measurements of the particles at Ag concentrations of 10 ppm in water were carried out (Figure 1). In water Ag-NP obtained a hydrodynamic diameter of nm (mean ± standard derivation).

3.2. Dose-Response-Curves and Cytotoxicity Data

The first experiment was to measure the viability of the four different cell lines exposed to the silver nanoparticles and to the silver ions at different concentrations via the MTT assay. Figure 2 shows the dose-response curves of the four different cell lines: A-549, NIH-3T3, HEP-G2, and PC-12 cells cultivated in presence of silver nanoparticles and of silver ions, respectively, after 72 h exposure. The results of the MTT assay were extrapolated using formulas (1) to (3).

(a)

(b)

(c)

(d)

In Table 2 the thus calculated IC₅₀ (Inhibitory Concentration), TLC (Total Lethal Concentration), and NOAEC (No Observable Adverse Effect Concentration) values for the different cell lines cultivated with silver nanoparticles and with silver nitrate are shown.

For all cell lines the decrease of the viability is much higher by cultivation in the presence of silver nanoparticles than by cultivation with silver ions (Figure 2). For all cell lines the IC₅₀ values by cultivation in the presence of silver nanoparticles are similar ranging from 4 ppm for the NIH-3T3 and PC-12 cells to 10 ppm for the A-549 cells, whereas the slopes of the dose-response curves are varying considerably more, resulting in respective differences in the TLC and NOAEC values. The values calculated for the silver ions differ drastically from those obtained for the silver particles; here the range for the IC₅₀ values is between 25 ppm for the PC-12 cells and 97 ppm for the HEP-G2 cells. The slopes of the curves differ in the same way resulting in a rather narrow toxic dose range between 94 ppm and 99 ppm for the HEP-G2 cells, whereas the toxic dose range for the A-549 cells is quite wide, that is, between 19 ppm and 144 ppm.

A-549 cells were chosen for the impedance measurements of cells cultivated in the presence of particles. These experiments were performed to verify the cytotoxicity results obtained from the MTT assay and the dose-response curves.

Figure 3 shows the ECIS of A-549 cells cultivated with silver nanoparticles at the IC₅₀ concentration of 10 ppm in the cell culture medium and the cell growth in normal culture medium as well as the impedance signal of a cell-free-electrode as a reference. The ECIS measurements allow online-monitoring of the nanoparticle effects to the cells. The impedance signal of the electrodes seeded with cells and cultivated with nanoparticles in the culture medium decreases immediately after addition of the particles, indicating a morphology change of the cells on the electrodes or a detachment of cells from the electrode surface, respectively.

The micrographs of the A-549 cells cultivated on the electrodes in normal medium and with 10 ppm silver nanoparticles in the medium after the impedance measurements, respectively, are shown in Figure 4. The micrographs confirm the decrease of the impedance signal indicating a morphology change of the cells. Moreover, a lower number of cells are found on the ECIS electrode cultivated in the presence of silver nanoparticles in the culture medium as compared with the electrode cultivated in normal culture medium. The treated cells exhibit a more spherical shape in comparison with the untreated cells.

(a)

(b)

3.3. Determination of Cell Death

To determine cell death, that is, to distinguish between apoptosis and necrosis, LDH measurements and caspase 3/7 activity measurements were performed using A-549 cells. For these experiments concentrations were chosen exhibiting a toxic response in the dose-response curves of the A-549 cells. The IC₅₀ value of A-549 cells cultivated with silver nanoparticles was determined to be 10 ppm; hence this concentration was used for the determination of the cell death. For the silver ions a concentration of 50 ppm was employed for the determination of the caspase 3/7 activity.

In Figure 5 the caspase 3/7 activity of A-549 cells cultivated with addition of 10 ppm silver nanoparticles in the culture medium and with 50 ppm silver ions as well as the activity of untreated cells in normal culture medium is shown. Cells cultivated with silver nanoparticles show a much higher caspase 3/7 activity than untreated cells. The caspase 3/7 activity of cells cultivated with silver ions at a concentration of 50 ppm is slightly lower than that of untreated cells.

Figure 6 displays the LDH release of the cell culture supernatant of A-549 cells cultivated in normal cell culture medium (untreated cells), with addition of 10 ppm silver nanoparticles and with 10 ppm silver ions. There is no LDH release in the cell culture supernatant of A-549 cells cultivated with silver nanoparticles at a concentration of 10 ppm evincing that the cell membranes are not destroyed. By cultivation of A-549 cells with 10 ppm of silver ions in the medium there is a LDH release in the culture supernatant which is, however, higher than in the supernatant of untreated cells. This indicates that the membranes are destroyed and the cells die due to necrosis.

4. Discussion

DLS measurements of particle suspensions in water (Figure 1) revealed that the hydrodynamic particle diameter is nm. Presumably, the hydrodynamic diameter of Ag nanoparticles in the culture medium could be smaller. Other studies have previously reported and confirmed the nanoparticle stabilization by proteins and sera contained in the medium [38–40]. The results obtained from the viability data of the MTT assay could be good described with the extrapolated dose-response curves (Figure 2).

The calculated IC₅₀, TLC, and NOAEC values are different for each cell line ranging from 3 ppm to 144 ppm. The most sensitive cells expressing a toxic response caused by silver nanoparticles are PC-12 and NIH-3T3 cells; here, IC₅₀ values as low as 4 ppm have been determined, whereas the IC₅₀ value for the A-549 cells is about 10 ppm. However, in comparison with the sensitivity of the cell lines cultivated in presence of silver ions the variation in the toxic doses is not very high. When cultivating the cells with silver ions IC₅₀ values between 25 ppm for the PC-12 cells and 97 ppm for the HEP-G2 cells have been determined. For each cell line investigated here, the IC₅₀, TLC, and NOAEC values are in the same range. Adding 3 ppm silver nanoparticles to NIH-3T3 cells has no effect; however, upon the addition of 4 ppm almost 50% of the cells were not viable anymore and once 5 ppm of silver nanoparticles were present in the culture medium only 5% of the cells were viable, confirming that the range of the toxic doses is very small. The results obtained also show that the toxic effect is not mainly caused by the silver ions but rather by silver nanoparticles for all tested cell lines. This effect has previously been observed in sea urchin Paracentrotus lividus [41].

Braydich-Stolle et al. investigated the toxic effect of 15 nm sized silver particles and a soluble silver salt (silver carbonate) on C18-4 cells and did not observe any toxic effect for the silver ions in the investigated concentration range [27]. The EC₅₀ values for the particles calculated from the MTS assay are found to be 8.75 μg/mL (8.75 ppm) while for the silver ions they are as high as 408 μg/mL (408 ppm) [27]. In the present study higher toxicity of silver ions (IC₅₀ values between 25 ppm and 97 ppm) was observed; however, the EC₅₀ values for the silver particles are found to be in the same range for the cell lines studied here (IC₅₀ values between 4 ppm and 10 ppm).

Hussain et al. investigated the toxic effect of silver nanoparticles with different sizes on BRL3A rat liver cells [28]. The EC₅₀ value for the silver particles with a diameter of 100 nm was reported to be μg/mL ( ppm) while for particles with a size of 15 nm an EC₅₀ value of μg/mL ( ppm) has been determined [28]. These toxicity values are slightly lower than those found here, but in the same range. On the contrary, Haase et al. reported an IC₅₀ value of 110 μg/mL (110 ppm) for peptide coated silver nanoparticles with a diameter of 20 nm [38]. Kawata et al. investigated the toxic effect of silver nanoparticles with a size of 7–10 nm of silver carbonate and of polystyrene nanoparticles (as reference) to HEP-G2 cells [32]. They observed a decrease in cell viability by addition of 2 mg/L (2 ppm) of the silver nanoparticles to the cells. Both the cultivation with polystyrene as a nontoxic nanoparticle reference and that with silver ions in the concentration range between 0.1 mg/L and 3 mg/L showed no toxic effect [32]. Our results indicate that there is a toxic effect of silver nanoparticles on HEP-G2 cell when adding concentrations exceeding 4 ppm.

The ECIS of A-549 cells cultivated with silver nanoparticles at a concentration of 10 ppm and the reference cell growth in normal medium shown in Figure 3 confirm the toxicity of silver nanoparticles. It is obvious that the impedance signal decreases directly after addition of 10 ppm of silver nanoparticles. That indicates that the toxic effect occurs immediately after the addition of the nanoparticles. In the absence of cells the impedance signal is not influenced by the nanoparticles as shown in Figure 3. The signal of a cell-free electrode with nanoparticles showed the same impedance signal as the cell-free electrode incubated with only medium.

The micrographs of the electrodes taken after the ECIS experiment (Figure 4) confirm these results. The electrode seeded with cells in normal culture medium (Figure 4(a)) showed a confluent cell layer of A-549 cells which in the ECIS measurement was observed as a high impedance signal. The electrode with cells cultivated for 48 h with silver nanoparticles at a concentration of 10 ppm only showed a few cells on the electrode surface corresponding to a low impedance signal in the measurement. Apparently the dead cells detached from the electrode surface and because of that the impedance signal decreased. The cells which remained attached to the electrode surface exhibited changes in morphology and were found to be smaller than untreated cells which can be regarded as an indicator for apoptosis. Similar morphological changes of cells cultivated in the presence of silver nanoparticles at a concentration of 10 μg/mL were observed by Braydich-Stolle and coworkers [27]. The IC₅₀ value of A-549 cells cultivated with silver nanoparticles calculated from the dose-response curves is 10 ppm; thus ECIS showed a good correlation with these results.

To determine the kind of cell death LDH release and caspase 3/7 activity measurements were carried out with A-549 cells cultivated with silver nanoparticles and silver ions. As shown in Figure 6, there was no LDH release in the cell culture supernatant of the A-549 cells cultivated with silver nanoparticles at a concentration of 10 ppm, whereas the overlap of cells cultivated with silver ions showed much more LDH release which is similar to that observed for untreated cells. This indicates that cell death induced by cultivation with nanoparticles is not related to necrosis, since the cell membranes remain intact. Untreated cell culture also contains cells which due to mechanical interferences are necrotic. Braydich-Stolle et al. also found no significant LDH release in C18-4 cells cultivated with different concentrations of silver nanoparticles in the concentration range between 5 μg/mL and 100 μg/mL (5 and 100 ppm) [27]. Measurements of the caspase 3/7 activity of A-549 cells cultivated with silver nanoparticles at a concentration of 10 ppm and with silver ions at a concentration of 50 ppm (Figure 5) revealed a much higher activity of caspase 3/7 in cells cultivated with the particles as compared to cells cultivated in cell culture medium alone or with addition of 50 ppm silver ions. That indicates that the A-549 cells are undergoing apoptosis by cultivation with silver nanoparticles, whereas the cells cultivated with silver ions do not exhibit apoptosis but rather show necrosis.

The mechanism of cell death is clearly different when cultivation is performed in the presence of nanoparticles or ions, leading to the conclusion that the toxic effect of silver nanoparticles to A-549 cells is indeed not caused by the silver ions. Moreover, these results are supported by the dose-response curves as well as the calculated IC₅₀ values.

5. Conclusions

The toxic effect of silver nanoparticles on four different mammalian cell lines has been investigated studying the mitochondrial activity and employing the Electric-Cell-Substrate-Impedance-Sensing (ECIS) method. As reference, Ag⁺-ions were used at the same concentration as the Ag-atoms present in the particles.

Based upon the results of the MTT assay, dose-response curves were extrapolated and IC₅₀, TLC, and NOAEC values were calculated. The results showed that silver nanoparticles are considerably more toxic than silver ions. Depending on the cell line the respective values were found to be between 5 (PC-12 cells) and 18 (NIH-3T3 cells) times higher.

The results from ECIS measurements indicate that the toxic effect of the silver nanoparticles occurs immediately after addition of the silver nanoparticle suspension. Measurements of LDH release of the cell culture supernatant of cells cultivated with nanoparticles or ions, respectively, showed no release for cells cultivated with the particles but LDH release for the ions. Cells cultivated with toxic doses of nanoparticles or ions, respectively, showed caspase 3/7 activity for the nanoparticles but no activity for the ions. Clearly, the mechanism of cell death is different when cultivations are carried out with silver particles or with ions. Cells cultivated in the presence of particles apparently suffer apoptosis while cells cultivated with ions die due to necrosis.

Conflict of Interests

The authors declare that there is no conflict of interests regarding the publication of this paper.

Acknowledgments

This work was supported by the German Federal Ministry of Education and Research (BMBF Project “HelioClean,” Grant no. 03X0069F). For constructive discussions Professor Cornelia Kasper is gratefully acknowledged.

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Copyright © 2015 F. Sambale 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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