|Home | About | Journals | Submit | Contact Us | Français|
The use of silver in the past demonstrated the certain antimicrobial activity, though this has been replaced by other treatments. However, nanotechnology has provided a way of producing pure silver nanoparticles, and it shows cytoprotective activities and possible pro-healing properties. But, the mechanism of silver nanoparticles remains unknown. This study was aimed to investigate the effects of silver nanoparticles on bronchial inflammation and hyperresponsiveness. We used ovalbumin (OVA)-inhaled female C57BL/6 mice to evaluate the roles of silver nanoparticles and the related molecular mechanisms in allergic airway disease. In this study with an OVA-induced murine model of allergic airway disease, we found that the increased inflammatory cells, airway hyperresponsiveness, increased levels of IL-4, IL-5, and IL-13, and the increased NF-κB levels in lungs after OVA inhalation were significantly reduced by the administration of silver nanoparticles. In addition, we have also found that the increased intracellular reactive oxygen species (ROS) levels in bronchoalveolar lavage fluid after OVA inhalation were decreased by the administration of silver nanoparticles. These results indicate that silver nanoparticles may attenuate antigen-induced airway inflammation and hyperresponsiveness. And antioxidant effect of silver nanoparticles could be one of the molecular bases in the murine model of asthma. These findings may provide a potential molecular mechanism of silver nanoparticles in preventing or treating asthma.
Nanomaterials are a diverse class of small-scale (<100 nm) substances, formed by molecular-level engineering and designed to offer unique mechanical, optical, electrical, and magnetic properties.1 Recently, much effort has been devoted to the development of biomedical applications for nanoparticles (NPs). NPs are also being examined for potential medical applications, such as drug delivery, because they are able to pass readily through cell membranes.2 Metal NPs have been attracting increasing attention due to their important applications in a number of subject areas, such as catalysis and nanoscale electronics.3–6 While significant advances in biological labeling have been made, few therapeutic applications for metal NPs have been reported in the literature.7,8 Some noble metal NPs are catalysts for reduction reactions; thus, they may be usable as antioxidants, reducing reactive oxygen species (ROS) in the living body.9–11 Another candidate material for NPs is silver, which has long been known as a strong antimicrobial agent and disinfectant, which may be due to the blockage of the respiratory enzyme pathways, alterations in microbial DNA, and cell wall modification.12 Silver has been used for centuries to prevent and treat a variety of diseases, including its use in pleurodesis, cauterization, and healing of skin wounds.13,14 The use of silver in the past has been restrained by difficulties in the production of pure silver compounds, thereby increasing potential side effects. Nanotechnology has provided a way of producing pure silver NPs. Some studies of silver NPs have demonstrated that they exhibit cytoprotective activities toward HIV-1-infected cells and anti-inflammatory effects, through cytokine modulation upon topical application.15–17 However, the exact mechanism of their anti-inflammatory effects is not fully understood.
Widespread application of nanomaterials holds enormous potential for safe human exposure and environmental release. Elemental silver occurs naturally. It is considered non-toxic, non-allergic, is not cumulative, and is not known to harm either wildlife or the environment. Products made with silver nanoparticles have been approved by a range of authorities, including the US FDA, US EPA, the SIAA of Japan, Korea’s Testing and Research Institute for Chemical Industry and the FITI Testing and Research Institute. Many consumer goods (eg, toys, baby pacifiers, clothing, food storage containers, face masks, HEPA filters, laundry detergent) already incorporate silver NPs for their antimicrobial properties. While ingestion and skin penetration are potential exposure routes for engineered nanomaterials, the inhalation route for airborne nanomaterials has perhaps received the most attention.18,19
In the present study, we used a mouse model of allergic airway disease to evaluate the effect of silver NP inhalation on airway hyperresponsiveness and inflammation and to investigate the related molecular mechanisms.
For morphological studies of silver NPs, we had assistance from the National Nanofab Center, Korea Advanced Institute of Science and Technology in Daejeon. To enable the characterization of the samples using TEM imaging with a reasonable resolution, a silver NP solution was diluted in alcohol and was dispersed evenly for prevention of aggregating particles and elimination of water. It was coated with mesh grid during imaging. The fine structure and particle size images of the silver NPs powder were obtained using a TEM (JEM-3020, 300 kV, JEOL, Japan).
Female C57BL/6 mice, 8–10 weeks of age and free of murine specific pathogens, were obtained from Damul Science Inc. (Daejeon, South Korea) and were maintained under standard laboratory conditions in a pathogen-free cage, with ad libitum access to food and water. All animal experiments in this study were conducted in accordance with the guidelines of the Institutional Animal Care and Use Committee of the Chungnam National University Medical School.
Mice were sensitized on days 1 and 14 via an intraperitoneal (ip) injection of 20 μg of ovalbumin (OVA) (Sigma-Aldrich, St. Louis, MO, USA) emulsified in 1 mg of aluminum hydroxide (Pierce Chemical Co., Rockford, IL, USA) in a total volume of 100 μL. On days 21–23 after the initial sensitization, the mice were challenged for 30 min with an aerosol of 3% (weight/volume) OVA in saline (or saline alone as a control) using an ultrasonic nebulizer (NE-U12, Omron, Japan). Bronchoalveolar lavage (BAL) was performed 72 hours after the final challenge. At the time of lavage, the mice (8 per group) were sacrificed with an overdose of pentobarbital sodium (100 mg/kg body weight, ip). The chest cavity was exposed to allow for expansion, after which the trachea was carefully intubated and the catheter was secured with ligatures. Pre-warmed 0.9% NaCl solution was slowly infused into the lungs and withdrawn. The aliquots were pooled and kept at 4°C. A part of each pool was centrifuged, and the supernatant was kept at −70°C until use. Total cell numbers were counted using a hemocytometer. Smears of BAL cells were prepared using a cytospin (Cellspin; Hanil Science Industrial Co, Ltd, Inchon, South Korea). To examine cell differentials, the smears were stained with Diff-Quik solution (Dade Diagnostics of PR Inc, Aguada, Puerto Rico, USA). Two independent, blinded investigators counted the cells under a microscope. Approximately 400 cells were counted in each of four random locations. The inter-investigator variation was <5%, and the mean number of cells from both counts was used to estimate cell differentials.
Silver NPs were obtained from Nano Chemical Inc. (Daejeon, South Korea). Silver NPs were dissolved in PBS and administered by nebulizer (20 ppm, 40 mg/kg body weight/day) five times to each animal at 24-hour intervals for 5 days prior to each challenge day (days 19–24), beginning 1 hour before the first challenge.
Airway responsiveness was evaluated 48 hours after the final challenge, with the mice in an unrestrained conscious state. The mice were placed in a barometric plethysmographic chamber (All Medicus Co., Seoul, Korea), and baseline readings were taken and averaged for 3 min. Increasing concentrations (2.5–50 mg/mL) of aerosolized methacholine were nebulized through an inlet into the main chamber for 3 min. Readings were taken and averaged for 2 min after each nebulization. Enhanced pause (Penh) was used as a measure of airway responsiveness to methacholine. Penh is a dimensionless value that represents a function of the proportion of maximal expiratory to maximal inspiratory box pressure signals and a function of the timing of expiration. It was calculated according to the manufacturer’s protocol as: Penh = (expiratory time/relaxation time −1) × (peak expiratory flow/peak inspiratory flow). The results are expressed as the increase in Penh following challenge with each concentration of methacholine, where the baseline Penh (after saline challenge) is defined as 1.
Blood samples were obtained within 24 hours after the administration of silver NPs by nebulizer (20 ppm, 40 mg/kg body weight/day) five times to each animal at 24 hour-intervals for 5 days. Mouse blood or serum was obtained from female, BALB/c inbred mice. Hematologic parameters were analyzed in EDTA blood samples with XE-2100 (Sysmex, Kobe, Japan), hematology analyzer.
Blood chemistry was determined in serum samples from the control and silver NPs inhaled group 24 hours after silver NPs administration (by nebulizer, 20 ppm, 40 mg/kg body weight/day).
ROS were measured using a previously described method.20 BAL cells (1 × 104 cells) were washed in PBS, incubated for 10 min at room temperature in PBS containing 3.3 μmol/L dichlorofluorescein diacetate (DCF-DA) (Molecular Probes, Eugene, OR, USA), transferred to polystyrene tubes with cell-strainer caps, and analyzed using a Cytomics FC 500 CXP flow cytometry system (Beckman Coulter Inc., Fullerton, CA, USA). We then measured the average percentage of cells that were either DCF-DA-unstained or -stained. Fluorescence images of intracellular ROS were acquired and analyzed using a fluorescence microscope (IX-71; Olympus Optical Co., Tokyo, Japan).
The lungs were removed and homogenized in 2 volume of buffer A (50 mmol/L Tris-HCl, pH 7.5, 1 mmol/L EDTA, 10% glycerol, 0.5 mmol/L dithiothreitol [DTT], 5 mmol/L MgCl2, and 1 mmol/L phenylmethanesulfonyl fluoride [PMSF]) containing protease inhibitor cocktail. The homogenates were centrifuged at 1,000 × g for 15 min at 4°C. The supernatants from the homogenates were incubated on ice for 10 min and centrifuged at 100,000 × g for 1 hour at 4°C, to obtain cytosolic proteins for the analysis of NF-κB p65 levels. To prepare soluble nuclear proteins, the pellets from the homogenate were washed twice in buffer A, re-suspended in buffer B (1.3 mmol/L sucrose, 1.0 mmol/L MgCl2, and 10 mmol/L potassium phosphate buffer, pH 6.8), and centrifuged at 1,000 × g for 15 min. The pellets were re-suspended in buffer B with a final sucrose concentration of 2.2 mol/L and centrifuged at 100,000 × g for 1 hour. The resulting pellets were washed once with a solution containing 0.25 mol/L sucrose, 0.5 mmol/L MgCl2, and 20 mmol/L Tris-HCl, pH 7.2, and centrifuged at 1,000 × g for 10 min. These pellets were solubilized with a solution containing 50 mmol/L Tris-HCl (pH 7.2), 0.3 mol/L sucrose, 150 mmol/L NaCl, 2 mmol/L EDTA, 20% glycerol, 2% Triton X-100, 2 mmol/L PMSF, and protease inhibitor cocktail. The mixture was kept on ice for 1 hour with gentle stirring and then centrifuged at 12,000 × g for 30 min. The resulting supernatants were used as soluble nuclear proteins for the analysis of NF-κB p65. Protein levels were analyzed on Western blots, using an antibody against NF-κB p65 (Cell Signaling Technology, Beverly, MA, USA) as described above.
Total RNA from lung tissues was isolated using a rapid extraction method (TRI-Reagent; Montgomery Rd, OH, USA) as previously described.21 NA was quantified by measuring absorption at 260 nm and was stored at −80°C before use. Total RNA (4 μg) was reverse-transcribed to cDNA in a buffer containing 50 mM Tris-HCl (pH 9.0), 16 mM (NH4)2SO4, 1.75 mM MgCl2, 0.1 M DTT; 1 μL oligo(dT) (500 μg/mL), 10 mM dNTP, 40 units RNase inhibitor, and 1 μL SuperScript II RT (200 units/μL, Life Technologies, Grand Island, NY, USA), in a final vol of 20 μL. This mixture was incubated for 50 min at 42°C and was heated for 15 min at 70°C for enzyme inactivation. The first-strand cDNAs were used for PCR amplification of IL-4, IL-5, IL-13, or the housekeeping gene, GAPDH. PCR amplification was performed by mixing 3 μL of the RT reaction mixture with 47 μL of buffer containing 2.5 U of Taq DNA polymerase (Promega, Madison, WI, USA) and 10 pmol of specific primer pairs for mouse cDNA of IL-4, IL-5, IL-13, or GAPDH, designed from published mouse gene sequences. The primers used were as follows: IL-4 (predicted length 400 bp) sense: 5′-CATCCTGCTCTTCTTTCTCGT-3′, antisense: 5′-GTACTACGTGTAATCCATTTG-3′; IL-5 (predicted length 201 bp) sense: 5′-GAGCACAGTGGTGAAAGAGAC-3′, antisense: 5′-ATGACAGGTTTTGGAATAGCATTT-3′; IL-13 (predicted length 182 bp) sense: 5′-GCCAGCCCACAGTTCTACAGC-3′, antisense: 5′-GTGATGTTGCTCAGCTCCTCA-3′ and GAPDH (predicted length 609 bp) sense: 5′-GCCATCAACGACCCCTTCATTGAC-3′, antisense: 5′-ACGGAAGGCCATGCCAGTGAGCTT-3′. PCR reactions were performed in a thermocycler (GeneAmp® PCR System 2400, Foster City, CA, USA) using the following reaction conditions; after an initial incubation for 5 min at 95°C, samples were subjected to 27 cycles (GAPDH) or 35 cycles (IL-4, IL-5, IL-13) of 5 min at 94°C, 30 sec at 60°C (GAPDH), 60°C (IL-4), 58°C (IL-5), 60°C (IL-13) and 1 min at 72°C. A final extension step at 72°C for 10 min was performed. The RT-PCR products were electrophoretically fractioned on 2% agarose gels stained with ethidium bromide. DNA bands were visualized after exposure to UV light.
Lung tissues were homogenized in the presence of protease inhibitors, and protein concentrations were determined using the Bradford assay (Bio-Rad Laboratories Inc., Hercules, CA, USA). Samples were loaded onto a gel and subjected to SDS-PAGE at 120 V for 90 min. The separated proteins were transferred to nitrocellulose membranes (GE Healthcare Bio-Sciences, Piscataway, NJ, USA) via the wet transfer method (250 mA, 90 min). Nonspecific sites on the membranes were blocked by incubation for 1 hour in 5% non-fat dry milk in Tris-buffered saline containing Tween 20 (TBST; 25 mmol/L Tris, pH7.5, 150 mmol/L NaCl, 0.1% Tween 20), and the blots were then incubated overnight at 4°C with an anti-IL-4 antibody (Serotec Ltd, Oxford, UK), anti-IL-5 antibody (Santa Cruz Biotechnology, Santa Cruz, CA, USA), or anti-IL-13 antibody (R&D Systems, Inc., Minneapolis, MN, USA). Anti-rat or anti-mouse horseradish peroxidase-conjugated IgG was used to detect antibody binding. The membranes were stripped and re-probed with an anti-actin antibody (Sigma-Aldrich) to verify equal loading of proteins in each lane. Specific antibody binding was visualized by exposure of the membranes to photographic film, after treatment with enhanced chemiluminescence system reagents (GE Healthcare Bio-Sciences, Piscataway, NJ, USA).
For histological analysis, the mice were sacrificed 72 hours after the final challenge, and the lungs and trachea were filled with fixative (0.8% formalin, 4% acetic acid). The trachea was ligated, and the lungs and trachea were dissected out. The lung tissues were fixed with 10% (volume/volume) neutral-buffered formalin. Specimens were dehydrated and embedded in paraffin, and 4-μm-thick sections were cut using a Leica model 2165 rotary microtome (Leica Microsystems Nussloch GmbH, Nussloch, Germany). The sections were placed on slides, deparaffinized, and stained sequentially with hematoxylin 2 and eosin-Y (Richard-Allan Scientific, Kalamazoo, MI, USA). All stained slides were evaluated via light microscopy under identical conditions with respect to magnification (20×), gain, camera position, and background illumination.22 The degrees of peribronchial and perivascular inflammation were scored by three independent, blinded investigators using a subjective scale of 0–3 (0, no detectable inflammation; 1, occasional cuffing with inflammatory cells; 2, most bronchi or vessels surrounded by a thin layer of between one and five inflammatory cells; 3, most bronchi or vessels surrounded by a thick layer of more than five inflammatory cells), as described elsewhere.23 Total lung inflammation was defined as the average of the peribronchial and perivascular inflammation scores.
All immunoreactive signals were scanned and densitometric analyses were performed using a Gel-Pro Analyzer (Media Cybernetics, Silver Spring, MD, USA). Data are expressed as the mean ± SEM. Statistical comparisons were made using one-way analysis of variance (ANOVA) followed by Scheffe’s test. Significant differences between two groups were determined using an unpaired Student’s t-test. Statistical significance was set at P < 0.05.
TEM was used to study the morphology and particle size of the silver NPs (Figure 1). The particles have a spherical shape. Mean particle size is 6.0 ± 0.29 nm.
To determine systemic effects of silver NPs, we introduced hematologic and serum chemistry profiles. For example, C-reactive protein, an acute-phase protein, is used as a biomarker of inflammation and lactate dehydrogenase is used as a marker of cytotoxicity. No significant changes in any of the hematological or serum chemistry parameters measured were observed in the inhalation exposure to silver NPs compared with the control (Tables 1 and and2).2). Only minor differences on serum chemistry levels were observed (Table 2).
Intracellular ROS generation was examined under a fluorescence microscope, and ROS levels were quantified via FACScan analysis. ROS generation in BAL cells was significantly higher at 72 hours after OVA inhalation compared with ROS generation after saline inhalation (31.3 ± 1.1 vs 24.5 ± 1.4%, respectively). This increase in ROS generation was substantially attenuated by the administration of silver NPs (28.0 ± 1.2%) (Figure 2).
Western blot analysis showed a significant increase in NF-κB p65 in the nuclear protein extracts from lung tissues at 72 hours after OVA inhalation, compared with the level in control mice (Figure 3). This increase in NF-κB p65 after OVA inhalation was decreased significantly with the administration of silver NPs. In contrast, NF-κB p65 in the cytosolic protein fractions from lung tissues was decreased after OVA inhalation, compared with the level in control mice, and this decrease in cytosolic NF-κB p65 was also attenuated by the administration of silver NPs.
RT-PCR revealed that IL-4, IL-5, and IL-13 mRNA levels were increased substantially in lung tissues at 72 hours after OVA inhalation, compared with the levels after saline inhalation (Figure 4A). These increases were inhibited by the administration of silver NPs. Consistent with these results, Western blot analysis also demonstrated that cytokine levels in lung tissues were increased significantly at 72 hours after OVA inhalation, compared with the levels in control mice (Figures 4B and 4C) and that these increases were inhibited by the administration of silver NPs.
The numbers of total cells, eosinophils, lymphocytes, and neutrophils in BAL fluids were increased significantly at 72 hours after OVA inhalation, compared with the cell counts after saline inhalation (Figure 5F), and the administration of silver NPs blocked these increases in cell counts after OVA inhalation. Similarly, the scores for total lung inflammation were significantly increased at 72 hours after OVA inhalation, compared with the scores after saline inhalation (Figure 5E). The total lung inflammation scores after OVA inhalation were significantly lower with the administration of silver NPs.
Airway responsiveness was assessed based on the increase in Penh in response to increasing doses of methacholine. In OVA-sensitized and OVA-challenged mice, the Penh dose-response curve was shifted to the left compared with the control curve (Figure 6). In addition, Penh produced by the administration of 50 mg/mL methacholine was significantly greater in OVA-inhaled mice than in control mice. OVA-sensitized and OVA-challenged mice treated with silver NPs showed a substantial reduction in Penh at 50 mg/mL methacholine compared with untreated mice after OVA inhalation. These results indicate that silver NP treatment reduces OVA-induced airway hyperresponsiveness.
Bronchial asthma is a chronic inflammatory disease of the airways characterized by airway eosinophilia, goblet cell hyperplasia with mucus hypersecretion, and hyperresponsiveness to inhaled allergens and nonspecific stimuli.24,25 There is increasing evidence that inflammation, which is characteristic of asthma, results in increased oxidative stress in the airways.26 Eosinophils, alveolar macrophages, and neutrophils from asthmatic patients produce more ROS than do those from normal subjects.27–30 ROS are involved in airway smooth muscle contraction, impairment of β-adrenergic receptors, decreased number and function of epithelial cilia, increased mucus production, altered release of inflammatory mediators, influx of inflammatory cells, and increased vascular permeability.31
The overproduction of ROS or depression of protective mechanisms also results in bronchial hyperreactivity, which is characteristic of asthma.32–34 ROS directly cause contraction of airway smooth muscle preparations, and this effect is enhanced when the epithelium is injured or removed.32 Studies in animal models have indicated that ROS contribute to airway hyperresponsiveness by increasing vagal tone due to damage of oxidant-sensitive β-adrenergic receptors as well as decreased mucociliary clearance.35,36
ROS appear to directly stimulate the release of histamine from mast cells and mucus secretion from airway epithelial cells.37 Increased ROS release may directly result in oxidative damage to epithelial cells and cell shedding.29 Previous studies have suggested that ROS may lead to endothelial barrier dysfunction, with subsequent increased permeability to fluid, macromolecules, and inflammatory cells.31
The present study using an OVA-induced model of allergic airway disease demonstrated that ROS production was increased in cells from BAL fluids and that the administration of silver NPs significantly attenuated ROS generation, Th2 cytokine expression, bronchial inflammation, and airway hyperresponsiveness in OVA-challenged mice.
We also noted that the increased levels of nuclear NF-κB induced by OVA inhalation were decreased with the administration of silver NPs. NF-κB is a multiprotein complex that is known to activate a large number of genes involved in early cellular defense reactions in higher organisms. In non-stimulated cells, inactive NF-κB is found in the cytosol.38 NF-κB plays an important role in immune and inflammatory responses and is present in most cell types.39–43 The role of ROS in the activation of NF-κB signal transduction was initially observed in cells treated with H2O2.44 A recent study reported that the development of an oxidant/antioxidant imbalance in asthma leads to the activation of the redox-sensitive transcription factor NF-κB.45 ROS have been directly implicated as second messengers in the activation of NF-κB, based upon the ability of oxidants to activate NF-κB via oxidation of its cysteine-SH group or via ubiquitination and proteolysis of IκB.46–48
NF-κB activation induces the transcription of a variety of inflammatory genes that are abnormally expressed in asthma, including cytokines (eg, IL-4, IL-5, IL-9, IL-15, and tumor necrosis factor [TNF]-α), chemokines (eg, regulated upon activation, normal T-cell expressed and secreted; eotaxin; and monocyte chemotactic protein-3), and adhesion molecules (eg, intercellular adhesion molecule-1 and vascular cell adhesion molecule-1).21,43,49,50 In a recent study, the antioxidant L-2-oxothiazolidine-4-carboxylic acid (OTC) was shown to inhibit airway inflammation in a murine model of asthma.51 In that study, OTC administration significantly reduced NF-κB translocation into the nucleus and the expression of adhesion molecules, chemokines, and cytokines. These results show that OTC inhibits NF-κB activity by preventing the ROS-induced translocation of this transcription factor into nucleus. Antioxidants have also been reported to inhibit NF-κB activation by preventing IκB degradation in response to various stimuli.52–56 Taken together, these findings indicate that the activation of NF-κB by ROS is a critical signaling mechanism for evoking inflammatory responses.
Our results suggest that silver NPs attenuate airway inflammation and hyperresponsiveness through the modulation of ROS generation, which subsequently attenuates the expression of inflammatory cytokines and NF-κB activation in mice with allergic airway disease. Thus, silver NPs appear to act as antioxidative and/or anti-inflammatory agents, based on this study. Nanocrystalline silver (NPI 32101) has been demonstrated to have anti-inflammatory properties through both its topical and oral use, as shown in previous experimental studies.57–60 In these studies, nanocrystalline silver was shown to significantly suppress the expression of IL-β, IL-12, metalloproteinase-9, and TNF-α.57,59 When nanocrystalline silver was introduced intravesically in a rat cystitis model, it decreased the number of mast cells and the extent of mast cell degranulation.60 However, there are also experiments showing that silver NPs induced inflammation.61,62 Proinflammatory cytokines, such as TNF-α, are rapidly secreted upon stimulation with various nanoparticles in macrophage RAW 264.7 cells.63,64 It has been proposed that nanosilver modulates cytokine production in a concentration-dependent manner.62 These conflict between various studies regarding the properties of nanoparticles, including silver NPs, illustrate that the role of the immune system is still being clarified. Among various inorganic nanoparticles, gold nanoparticles, platinum nanoparticles, and nano red elemental selenium have been reported to show antioxidative effects.9–11,21–23 However, the precise mechanism of quenching induced by platinum nanoparticles remains unclear, and although selenium is one of the essential metals in the body, contamination with sodium serenite makes the use of nanoselenium difficult in biological applications. In the present study, we were unable to identify the exact mechanism underlying the effects of silver NP treatment, but the results of our 2′,7′-DCF-DA and FACS analysis support an antioxidative effect in this murine model of asthma. To our knowledge, this is the first report demonstrating the antioxidative effects of silver NPs. However, studies indicating that silver NPs may generate free radicals have also been published.65,66
Despite the potential usefulness of silver NPs as antioxidative or anti-inflammatory agents, as indicated by this study, unresolved issues remain. First, the pharmacokinetics of silver NPs are not fully understood. Second, it is unclear where silver NPs scavenge ROS in the body of the mouse. That is, we did not determine the exact location of silver NP activity at the cellular level. Third, it may be important to control the concentration of silver NPs in order to scavenge only excess ROS and maintain the optimal ROS level. Fourth, controversy remains regarding the inflammatory/anti-inflammatory effects of silver NPs. Recent studies have reported that silver NPs exerted anti-inflammatory effects through the modulation of cytokine production, particularly Th1 cytokines, and mast cell activation.57,60,62 Other studies have suggested that silver NPs have inflammatory effects.61,63,67 These conflicting results may be attributable to several confounding factors such as particle size, surface charge, delivery method, route of administration, duration of administration, dose, and/or disease conditions (intra/extracellular milieu), which may alter the bioactive characteristics of nanoparticles in particular cells or tissue types.
In summary, although further studies are needed, our study suggests that oxidative stress is an important determinant of allergic airway disease and that silver NPs attenuated oxidative stress in the murine asthma model. Also, by administration of silver NPs, Th2 inflammation, which is one of the main asthma-inducing immune factors, was significantly decreased. We suggest that silver NPs may be useful as a therapeutic strategy through their properties as antioxidant and anti-inflammatory agents.
The English in this document has been checked by at least two professional editors, both native speakers of English.
We give special thanks to Prof Minho Shong, Chungnam National University, who supported much of the experimental work. We also thank Prof Yong Chul Lee, Chonbuk National University, for insightful recommendations and advice.
This research was supported by Chungnam National University Hospital Research Fund, 2006.
No conflict of interest has been declared.