Nanomedicine strategy for optimizing delivery to outer hair cells by surface-modified poly(lactic/glycolic acid) nanoparticles with hydrophilic molecules
Authors Wen X, Ding S, Cai H, Wang J, Wen L, Yang F, Chen G
Received 19 July 2016
Accepted for publication 22 September 2016
Published 10 November 2016 Volume 2016:11 Pages 5959—5969
Checked for plagiarism Yes
Review by Single anonymous peer review
Peer reviewer comments 2
Editor who approved publication: Dr Linlin Sun
Xingxing Wen,1,2 Shan Ding,1,2 Hui Cai,1,2 Junyi Wang,3 Lu Wen,1 Fan Yang,1,2 Gang Chen1,2
1School of Pharmacy, 2Guangdong Provincial Key Laboratory of Advanced Drug Delivery, 3School of Public Health, Guangdong Pharmaceutical University, Guangzhou, People’s Republic of China
Abstract: Targeted drug delivery to outer hair cells (OHCs) in the cochlea by nanomedicine strategies forms an effective therapeutic approach for treating hearing loss. Surface chemistry plays a deciding role in nanoparticle (NP) biodistribution, but its influence on such distribution in the cochlea remains largely unknown. Herein, we report the first systematic comparison of poly(lactic/glycolic acid) nanoparticles (PLGA NPs) with or without surface modification of hydrophilic molecules for optimizing the delivery to OHCs both in vitro and in vivo. NPs that were surface modified with poloxamer 407 (P407), chitosan, or methoxy poly(ethylene glycol) and the unmodified NPs were highly biocompatible with L929 and House Ear Institute-organ of Corti 1 cells as well as cochlear tissues. Interestingly, among all the examined NPs, P407-PLGA NPs showed the greatest cellular uptake and prominent fluorescence in cochlear imaging. More importantly, we provide novel evidence that the surface-modified NPs reached the organ of Corti and were transported into the OHCs at a higher level. Together, these observations suggest that surface modification with hydrophilic molecules will allow future clinical applications of PLGA NPs, especially P407-PLGA NPs, in efficient hearing loss therapy.
Keywords: inner ear drug delivery, PLGA nanoparticles, surface chemistry, cochlea, HEI-OC1 cell
According to the report from the World Health Organization, 5% of the world’s population (approximately 360 million people) suffers from a disabling hearing impairment.1 It is reported that noise exposure, ototoxic agents, aging, and some other factors result in the functional loss of outer hair cells (OHCs), bringing about hearing loss.2–4 To improve the efficiency for treating hearing loss associated with OHC pathology, targeted drug delivery to OHCs in the organ of Corti (OC) of cochlea is required.5,6 Novel nanosized drug vehicles are thought to overcome the limitations of classic approaches through controlled or sustained release into the inner ear fluids, cellular cytoplasm, or the nucleus of targeted cells.7,8 Therefore, drugs have been delivered to the inner ear based on nanomedicine strategies using different types of nanocarriers.6,9 Among these nanocarrier materials, poly(lactic/glycolic acid) (PLGA), approved by the US Food and Drug Administration in multiple drug delivery systems in humans, has attracted considerable attention due to its high biodegradability and biocompatibility.10 More interestingly, it has been illustrated in our previous study that PLGA nanoparticles (NPs) loaded with single or compound drugs enhanced the local bioavailability of drugs following inner ear administration.11
Since the NP surface contacts with biological systems, their characteristics greatly impact NP performance in vivo and the overall effectiveness.5,12,13 Changing the surface chemistry of the engineered NPs with biocompatible hydrophilic polymers or copolymers increases the circulation time and delays the removal of NPs by the mononuclear phagocyte system, which prevents rapid clearance before reaching the targeted tissues and delivering drugs.12,14,15 Based on these background studies, we theorized that attachment of these hydrophilic molecules onto the NP surface would enhance nanocarrier delivery to OHCs in the cochlea. To verify this hypothesis, a deeper and comprehensive comparison of surface-modified PLGA NPs with various hydrophilic molecules for OHC delivery was performed.
We have recently developed a PLGA-based NP platform with different surface decorations by poloxamer 407 (P407), chitosan (CS), and methoxy poly(ethylene glycol) (mPEG), respectively. Herein, we systematically compare the NPs with and without surface modification as nanocarriers for delivery to OHCs both in vitro and in vivo. Our study highlighted that the efficiency for NP delivery to the inner ear and OHCs was improved by modifying the NP surface with hydrophilic molecules, especially with P407 decoration, as an optimizing strategy.
Materials and methods
Coumarin-6 and polyvinyl alcohol 4-88 (PVA, molecular weight [MW] 31 kDa) were purchased from Sigma-Aldrich Co. (St Louis, MO, USA). 1,1′-Dioctadecyl-3,3,3′,3-tetramethylindotricarbocyanine iodide (DiR) was purchased from Molecular Probes (Thermo Fisher Scientific, Waltham, MA, USA). PLGA (LA/GA =75:25, MW 10 kDa) and mPEG-PLGA (LA/GA =75:25, MW 10 kDa; mPEG, MW 1.9 kDa) were supplied by Shandong Medical Institute (Shandong, People’s Republic of China). P407 (Pluronic F127) was a gift from BASF (Ludwigshafen, Germany) and used as supplied. CS (MW 300 kDa) was purchased from Zhejiang Golden-Shell Pharmaceutical Co., Ltd (Zhejiang, People’s Republic of China). Cell counting kit-8 (CCK-8) was purchased from Dojindo Molecular Technology Inc. (Shanghai, People’s Republic of China). 4′,6-Diamidino-2-phenylindole (DAPI) was purchased from Beyotime Institute of Biotechnology (Shanghai, People’s Republic of China). All reagents were used as received without further purification.
Preparation and size measurement of NPs
PLGA NPs were prepared by the emulsion/solvent evaporation method. Briefly, 1 mL of dichloromethane–ethyl acetate (7:3) containing 30 mg of PLGA and 60 μg of coumarin-6 was added to 5 mL of 3% (w/v) PVA aqueous solution on ice using a probe sonicator set at 190 W of energy output (Scientz Biotechnology Co. Ltd, Ningbo, People’s Republic of China) for 100 s with pulses of 5 s on and 5 s off to form an oil-in-water emulsion. Then, this emulsion was diluted with a 0.5% (w/v) PVA aqueous solution, followed by evaporation of organic solvents under magnetic stirring for 3 h to create coumarin-6 nanosuspension. CS-PLGA NPs were prepared by dissolving 30 mg of PLGA and 60 μg of coumarin-6 in 1 mL of ethyl acetate, and for P407-PLGA NPs, PLGA and coumarin-6 were dissolved in 1 mL of dichloromethane, respectively. The organic phase was added to an aqueous solution consisting of 1% PVA (w/v)–0.3% CS (w/v, CS was dissolved in 1% acetic acid solution) and 1% PVA (w/v)–1% P407 (w/v, P407 was dissolved in distilled water), respectively. For mPEG-PLGA NPs, 30 mg of mPEG-PLGA and 60 μg of coumarin-6 were dissolved in 1 mL of dichloromethane. Further steps performed were similar to those for PLGA NPs. DiR-loaded PLGA NPs were prepared with the same method as that for coumarin-6-loaded NPs, and the only difference was addition of 0.5 mg of DiR in the organic solvent. The size of NPs was determined by a Delsa™ Nano C particle analyzer (Beckman Coulter Instruments, Brea, CA, USA).
In vitro experiments
The uptake and toxicity of NPs were examined in vitro using cells from a mouse fibroblast cell line L929 (Type Culture Collection of the Chinese Academy of Sciences, Shanghai, People’s Republic of China), which were kept in modified Eagle medium (a-MEM; HyClone) supplemented with 10% fetal bovine serum, 100 IU/mL penicillin, and 100 IU/mL streptomycin at 37°C in 5% CO2 using a humidified incubator (Thermo HERAcell 150i; Thermo Fisher Scientific).
Then, the House Ear Institute-organ of Corti 1 (HEI-OC1) cells, which were derived from the OC and obtained from the House Ear Institute (Los Angeles, CA, USA), were used to further test the cytotoxicity and cellular uptake of NPs. The cells were cultured in high-glucose Dulbecco’s Modified Eagle’s Medium (DMEM; Thermo Fisher Scientific) containing 10% fetal bovine serum at 33°C in 10% CO2 using a humidified incubator (Thermo Forma 371, Thermo Fisher Scientific).
Cytotoxicity of NPs in L929 and HEI-OC1 cells detected by CCK-8 assay
Cell viability of NPs was determined using CCK-8 assay. L929 and HEI-OC1 cells were seeded at 1×104 cells per well onto 96-well plates and incubated for 24 h, respectively. Blank NPs at different concentrations (0.005, 0.5, 5, 10, 20, 25, and 40, 60, 80 mg/mL) in diluted medium were added into both types of cells, respectively. After treatment for 24 h, the NPs suspension was removed and the cells were rinsed twice with phosphate-buffered saline (PBS). Then, 10% CCK-8 solution was added to each well and incubated for 2 h. The absorbance was monitored at 450 nm in a microplate reader (RT-2100C; Rayto Life and Analytical Sciences Co. Ltd, Shenzhen, People’s Republic of China). Cell viability was quantified by the ratio to the control, and the untreated cells were assigned a cell viability of 100%.
Observation of NP cellular uptake by confocal microscopy
The cellular uptake and intracellular localization of NPs were confirmed by confocal microscopy. L929 and HEI-OC1 cells were seeded at 5×104 cells per well onto confocal special dishes and incubated for 24 h, respectively. Then, the cells were incubated with coumarin-6-loaded NPs at a concentration of 40 μg/mL in serum-free medium for 1 h. Afterward, the NPs were removed following a two-step washing with PBS, and then fixed with fresh 10% formalin for 10 min at room temperature. Next, these cells were incubated for 10 min with DAPI, a nuclei-specific dye with contrasting fluorescence, washed twice with PBS, and then analyzed under confocal microscope (LSM 710 Meta; Carl Zeiss Inc., Thornwood, NY, USA) with the following excitation and emission wavelengths: coumarin-6: excitation 453 nm, emission band pass 504–530 nm and DAPI: excitation 405 nm, emission 454–495 nm.
Quantification of NP cellular uptake by flow cytometry
The quantitative cellular uptake of NPs in L929 cells and HEI-OC1 cells was measured by flow cytometry. Briefly, the L929 and HEI-OC1 cells were seeded at 1×105 cells per well onto six-well plates and incubated for 24 h, respectively. To determine the NPs uptake and loading extent, the cells were incubated with coumarin-6-loaded NPs at a concentration of 40 μg/mL in serum-free medium for 1 h. Afterward, the cells were washed with PBS three times and harvested by trypsinization to obtain the suspension in PBS for monitoring. Green fluorescence-emitting coumarin-6 incorporated into different NPs served as a marker to quantitatively determine their cellular uptake by flow cytometer (BD Accuri C6; Becton Dickinson, Mississauga, ON, Canada), while 1×104 events were collected for each sample.
In vivo experiments
A total of 42 albino guinea pigs (250–300 g) of both sexes with normal Preyer reflexes were used in this study. They were obtained from the Laboratory Animal Center of Southern Medical University (Guangzhou, People’s Republic of China). All animal studies were performed in accordance with the protocols approved by the Animal Ethical Committee (Guangdong Pharmaceutical University, Guangzhou, People’s Republic of China); humane care was provided to all animals used in the studies. These animals had free access to food and water and were allowed a 1-week acclimation period before starting the experiment.
NPs application to the inner ear
The histocompatibility and distribution of four types of PLGA NPs in the inner ear were examined 24 h following intratympanic administration. Animals were anesthetized with ethyl carbamate (1 g/kg) before the administration. Following each in vivo experiment, four types of NPs at a concentration of 25 mg/mL (0.1 mL) were injected into the unilateral tympanic cavity of the guinea pigs (n=3), respectively. Meanwhile, the control animals (n=2) were treated with normal saline (NS).
Detection of NPs in the cochlea by near-infrared fluorescence (NIRF) imaging system
NPs in the cochlea were detected by an NIRF imaging system. After 24 h of treatment with DiR-loaded NPs or NS, the animals were decapitated under deep anesthesia, and bubbles were harvested rapidly and fixed with 10% formalin at 4°C. Then, the signal of DiR in the NPs was evaluated by the NIRF imaging system (NIGHTOWL LB 983 NC100; Berthold Technologies, Bad Wildbad, Germany) with the excitation and emission wavelengths of 700 and 780 nm, respectively. The statistical data obtained were expressed as the total amount of fluorescence and standard deviation.
Distribution of NPs in the cochlear tissues and evaluation of the safety using paraffin sections
Distribution of the NPs in cochlear tissues was examined on paraffin sections by confocal microscopy and their safety was evaluated through cochlear histopathology. Animals were sacrificed 24 h after administration of coumarin-6-loaded NPs or NS under deep anesthesia. After cardiac perfusion with NS and 10% formalin, bubbles were harvested rapidly and fixed with the same fixative at 4°C. The fixed inner ears were immersed in diluted nitric acid and stirred gently for approximately 48 h. The decalcified specimens were dehydrated with ethanol solutions at gradient concentrations, cleared in xylene, and finally embedded in paraffin. Serial 4 μm sections were cut from each paraffin block and mounted on glass slides. Then, the slides were used to observe the NPs in the cochlea under a fluorescence microscope (green channel) (Olympus Corporation, Tokyo, Japan), which were stained with DAPI to label the cell nucleus for observation in different cochlear tissues under confocal microscope (LSM 710 Meta, Carl Zeiss Inc.) or stained with hematoxylin and eosin to examine the histomorphology of the cochlear tissues in brightly fluorescent regions under the fluorescence microscope (Olympus Corporation).
Location of NPs in OHCs by cochlear surface preparation
Location of NPs in OHCs was visualized by cochlear surface preparation. As mentioned earlier, animals were sacrificed at intervals 24 h after the administration of NPs or NS; acoustic bullas were removed from them. Then, the bullas were rapidly opened and the fluid spaces were perfused with 10% formalin through the oval window and a fenestra in each semicircular canal. Membranous organs of the inner ear were then carefully dissected and fixed for 2 h at 4°C under high magnification. After washing in PBS, the fixed tissues were stained with DAPI for 10 min and washed twice with PBS. After staining, the basilar membrane with OC was placed on glass slides in glycerin and coverslipped. Then the coverslips were sealed with nail polish to protect the specimens from desiccation and the specimens were examined by confocal microscope (LSM 510 Meta, Carl Zeiss Inc.).
The fluorescence intensity was determined by AxioVision Rel. 4.7 (Carl Zeiss Inc.), and the average fluorescence value in each frame was computed using region of interest analysis. Herein, regions of interest are the areas corresponding to each cell or cochlear tissue. Analysis of variance followed by multiple comparisons test was used in Statistical Package for the Social Sciences (SPSS) 19.0 (IBM Corporation, Armonk, NY, USA) to determine significant differences between groups, and P-values less than 0.05 were considered statistically significant. The half-maximal inhibitory concentration (IC50 value) was obtained using SPSS software 19.0. Semi-quantitative fluorescent analysis was used to compare the uptake or biodistribution of different surface-modified PLGA NPs, and F-value was introduced to represent the ratio of the uptake or biodistribution of various PLGA NPs to that of unmodified PLGA NPs.
where Fx is the mean fluorescence intensity (MFI) of different types of PLGA NPs, F0 the MFI of unmodified PLGA NPs, and B is the MFI of control background.
Results and discussion
The application of nanomedicine in hearing loss therapy is primarily driven by the need for increasing the therapeutic index of a given drug, which may be achieved by optimizing the nanocarriers based on surface modification. Various hydrophilic molecules (P407, CS, and mPEG) were chosen to decorate PLGA NPs. Since it has been proven that nanocarriers transport across the middle–inner ear barriers in a size-dependent manner,16 we prepared various surface-modified NPs using different solvent systems to obtain NPs with similar sizes.17 In our study, we formulated four types of PLGA-based NPs with or without surface modification, that is, PLGA NPs, P407-PLGA NPs, CS-PLGA NPs, and mPEG-PLGA NPs, respectively (Figure S1). CS coating was achieved by electrostatic interaction between negatively charged PLGA chains and positively charged CS.18 P407 copolymers, containing polyethylene oxide (hydrophilic) and polypropylene oxide (hydrophobic) moieties, were adsorbed to particle surfaces from an aqueous solution through hydrophobic interaction of the hydrophobic moiety (the anchor block) with the particle surface,19 and mPEG-PLGA polymer was used to prepare mPEG-modified PLGA-NPs. These NPs possessed similar tailored average hydrodynamic sizes (100–200 nm) and relatively uniform size distribution (Table S1; Figures S2 and S3).
We first investigated the cytotoxicity and the uptake of NPs in L929 cells after treatment with various NPs, as depending on the modified molecules, the cytotoxicity and the uptake profiles can change.20 L929, a normal cell line, has been widely used in a series of studies including drug delivery to the inner ear.21,22 As shown in Figure 1A, the viability of L929 cells remained high after being treated with the four types of NPs at various concentrations, even up to 25 mg/mL (the original NPs suspension), suggesting that PLGA-based nanocarriers were biocompatible with normal cells. The IC50 values of unmodified, P407-, CS-, and mPEG-PLGA NPs were 53.56±1.03, 41.51±2.41, 56.06±6.36, and 51.03±2.43 mg/mL, respectively (n=6). Then, the cellular uptake and intracellular localization of coumarin-6-loaded NPs into L929 cells were observed by confocal microscopy. Figure 1B shows the colocalization of NPs (green) and DAPI-stained cell nucleus (blue) in L929 cells, suggesting PLGA-based NPs were internalized with a spotty distribution around the nucleus. Clearly, surface modification was a governing factor for the uptake of PLGA-based NPs by L929 cells, as indicated by the fluorescence intensity of internalized NPs. Semi-quantitative fluorescence analysis revealed that P407-PLGA NPs had the greatest cellular uptake with significantly higher F-value than those of other kinds of NPs (all P<0.001), followed by the unmodified, mPEG-, and CS-PLGA NPs, successively (Figures 1C and S4). The uptake efficiencies of unmodified, P407-, CS-, and mPEG-PLGA NPs in L929 cells were further quantified by flow cytometry and were found to be 95.3%, 98.7%, 76.2%, and 87.8%, respectively (Figures 1D and S5). Therefore, all the PLGA-based NPs, especially P407-PLGA NPs, had considerable uptake in L929 cells.
HEI-OC1, another cell model chosen in our study, is a conditionally immortalized mouse cell line derived from the postnatal OC displaying various phenotypes for nonsensory cells and used as a potential model system to screen otological drugs.23 We then investigated the viability of HEI-OC1 cells and the uptake of NPs in them after treatment with PLGA-based NPs. All PLGA-based NPs, and even the original NP suspension, were nontoxic to HEI-OC1 cells after coincubation for 24 h (Figure 2A). Taking the results of L929 cells into consideration simultaneously, 25 mg/mL NPs suspension was safe and appropriate for cochlear application in the following animal experiments to ensure their visualization in vivo. The IC50 values of unmodified, P407-, CS-, and mPEG-PLGA NPs were 71.30±4.16, 60.53±0.55, 65.39±0.47, and 81.70±1.04 mg/mL, respectively (n=6). Identical to the cytotoxicity against L929 cells, P407-PLGA NPs had the highest IC50 value, which may be explained by the higher uptake amount of NPs than those of others. The uptake of different NPs by HEI-OC1 cells was observed by confocal microscopy and quantified by flow cytometry. Similar to the intracellular localization and uptake of NPs in L929 cells, PLGA-based NPs were uniformly distributed throughout the cytoplasm and P407-PLGA NPs had the greatest cellular uptake, which was 1.33-, 1.46-, and 3.14-fold those of unmodified, CS-, and mPEG-PLGA NPs, respectively (all P<0.01) (Figures 2B, C, and S6). The uptake efficiencies of unmodified, P407-, CS-, and mPEG-PLGA NPs were 79.7%, 91.4%, 58.3%, and 48.1%, respectively (Figures 2D and S7). Remarkably, quantification of the flow cytometric analysis revealed that uptake in both cells was increased by applying P407 for surface decoration. Changing the physicochemical parameters of NP surface by coating P407 may facilitate this uptake process, during which the interaction between poloxamer and the cell membrane promotes endocytosis of NPs.24,25 It has been confirmed that glycerol monooleate-based NPs with high positive surface charge were more prone for uptake by L929 cells,21 but the uptake of CS-PLGA NPs with positive surface charge was less than that of unmodified PLGA NPs in our study. This difference may result from the surface charge density of NPs. At the positive surface charges of 20%–40%, NPs remain on the bilayer surface instead of being taken up by cells.26,27 For mPEG-PLGA NPs, significant increase in surface hydrophilicity may decrease the uptake efficiency compared to that of unmodified NPs. It is well documented that hydrophilic NPs tended to reside on the membrane surface,28,29 whereas hydroxyl-functionalized fullerenes were adsorbed on the bilayer surface because the cellular uptake rate was reduced by nine orders of magnitude.30
We also assessed whether different NPs would induce histological changes in the cochlea through intratympanic administration, as effectively delivering therapeutic agents to the inner ear without damaging the integrity of delicate structures is most challenging.31 Light microscopy with hematoxylin and eosin-stained paraffin sections did not reveal any inflammation in the inner ear. Individual cochlear tissues, including stria vascularis, spiral ligament, OC, and spiral ganglion cells, barely underwent morphological alterations after application of NPs for 24 h (Figure S8). This was consistent with the observation of cytotoxicity against L929 and HEI-OC1 cells.
Next, we encapsulated a near-infrared dye DiR into the NPs to study their cochlear entry by using an NIRF imaging system, owing to the extremely low tissue autofluorescence and high tissue penetration depth in the NIR spectrum window.32 By 24 h postinjection of P407-PLGA NPs, stronger fluorescence signal emitted from the excised cochleae than from those applied other NPs (Figure 3A). Moreover, as shown in Figure 3B, the excised cochleae treated with modified NPs showed higher fluorescence intensity than those treated with unmodified NPs. Particularly, the fluorescence intensity of P407-PLGA-NP-treated cochleae was 2.4-, 2.0-, and 1.55-fold those of the cochleae treated with unmodified, CS-, and mPEG-PLGA NPs, respectively (all P<0.05). Therefore, hydrophilic coating of PLGA NPs, especially P407 modification, played a key role in inner ear transport.
We then investigated NP distribution in the whole cochlear tissue and the individual cochlear structures by fluorescence microscopy or confocal microscopy, since the impact of surface modification of NPs with hydrophilic groups on the distribution of NP in the cochlear tissue has not been evaluated until now. In the paraffin sections of the cochlear tissue, more prominent fluorescence signal was observed from the apex and basal turns of the cochlea for surface-modified NPs compared with those of unmodified PLGA NPs (Figure 4). The signal of P407-PLGA NPs was significantly stronger (1.44-fold) than that of unmodified NPs, as evidenced by the semi-quantitative fluorescence analysis (P<0.05) (Figure 4G). Besides, surface-modified PLGA NPs were considerably localized in spiral ligament, stria vascularis, OC, and spiral ganglion cells, whereas unmodified PLGA NPs were marginally distributed (Figure S9). Moreover, PLGA NPs with P407 modification accumulated to the greatest extent in the cochlear tissues (Figure 4H). This was in line with the result of NIRF imaging for the excised cochleae that engineered NP surfaces with hydrophilic molecules promoted the entry of NPs into the cochlea and their approach to the cochlear tissues. Particularly, P407 modification had a notable effect on NP distribution in vivo.
Finally, we monitored the entry of different NPs to OHCs in vivo by cochlear surface preparation (Figure 5). Stronger fluorescence signal around the OHC nucleus was found in animals given surface-modified NPs than that in unmodified NP-injected ones. Moreover, the fluorescence signals of P407-PLGA and mPEG-PLGA NPs were obviously detected in OHCs along the full length of the cochlea, whereas that CS-PLGA NPs were weaker. Semi-quantitative fluorescence analysis suggested that P407-PLGA NPs accumulated extensively and were located more homogeneously in OHCs. Meanwhile, the amount of fluorescence of P407-PLGA NPs taken up by the OHCs was 1.95-, 1.76-, and 1.39-fold those of unmodified, CS-, and mPEG-PLGA NPs, respectively (all P<0.001). Accordingly, coating PLGA NPs with hydrophilic molecules, especially P407, facilitated their transport into the OHCs. In general, in order to achieve cellular targeting in the cochlea, ligands known to bind the surface receptors of selected cells should be conjugated to engineered NPs. For example, polymersome surface functionalized with hNgf EE peptide (a nerve growth factor-derived ligand) shows great potential for specific targeting to spiral ganglion neurons,33 while engineered the polymersomes with prestin-binding peptides can promote their targeting to the OHCs.5 In our study, the PLGA-based NPs modified with hydrophilic molecules delivered their cargo to the OHCs more effectively than unmodified NPs did, indicating that hydrophilic molecules could also play the role of ligands for entry to OHC.
The results of our study confirmed the hypothesis that surface modification with hydrophilic molecules promoted NP distribution in the cochlea and the OHCs. Surface attachments, P407, CS, and mPEG, enhanced cochlear entry in vivo, which may be attributed to the change in NP surface chemistry that prevents the clearance by ciliated epithelia in the tympanic cavity by blocking the hydrophobic interactions.14,34 Furthermore, by interacting with the cell membranes, P407 decreased the microviscosity and formed pores on the membrane,35–38 which may result in higher cellular uptake in the OHCs. Notably, in contrast to the little cellular uptake in vitro, mPEG-PLGA NPs were well distributed in vivo, probably due to their highest accumulation in the tissue among all kinds of NPs.39 Similarly, despite less cellular uptake in vitro, more CS-PLGA NPs reached OHCs than PLGA NPs did. Possibly, the NPs passed through the tight epithelial layer by a transcellular pathway in vivo and then through the loosely arranged connective tissue layer and the endothelial layer by an intercellular pathway.21,40
In summary, we prepared a series of surface-modified PLGA NPs using different hydrophilic molecules and investigated their transport into OHCs in vitro and in vivo, as well as compared them with unmodified NPs. The cytotoxicity, cellular uptake, biocompatibility, cochlear distribution, and location of these NPs were ascertained, which suggested that the PLGA-based nanocarriers were biocompatible and the hydrophilic coating had a notable effect on NP distribution. It was confirmed that the optimizing design using surface-modified PLGA NPs with hydrophilic molecules, especially for PLGA NPs functionalized with P407, had greater capability to facilitate their entry into OHCs, indicating that the hydrophilic molecules could also play the role of ligands for OHC entry. As a result, nanomedicine strategy employing hydrophilic molecule-coated PLGA NPs will broaden the way for a more efficient and more specific treatment for hearing loss originating from the impairment of OHCs.
This work was supported by the National Nature Science Foundation of China (Grant No 81274097), the Pearl River S&T Nova Program of Guangzhou (Grant No 2013J2200059), and the Cultivation Foundation for Distinguished Young Teachers in Higher Education of Guangdong (Grant No Yq2013099).
The authors report no conflicts of interest in this work.
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