Penetration and Silencing Activity of VEGF Dicer Substrate siRNA Vectorized by Chitosan Nanoparticles in Monolayer Culture and a Solid Tumor Model<i> In Vitro</i> for Potential Application in Tumor Therapy

Raja, Maria Abdul Ghafoor; Katas, Haliza; Abd Hamid, Zariyantey

doi:https://doi.org/10.1155/2016/7201204

Journal of Nanomaterials

On this page

Abstract Introduction Methods Results Conclusions Acknowledgments Supplementary Materials References Copyright Related Articles

Research Article | Open Access

Volume 2016 | Article ID 7201204 | https://doi.org/10.1155/2016/7201204

Penetration and Silencing Activity of VEGF Dicer Substrate siRNA Vectorized by Chitosan Nanoparticles in Monolayer Culture and a Solid Tumor Model In Vitro for Potential Application in Tumor Therapy

Maria Abdul Ghafoor Raja,¹Haliza Katas,¹and Zariyantey Abd Hamid²

Academic Editor: Hua Zou

Received05 Apr 2016

Accepted25 Jul 2016

Published18 Aug 2016

Abstract

Penetration and distribution of drug through the avascular regions of human solid tumors after extravasation are crucial concerns for antitumor efficacy. To address this issue, an in vitro solid tumor model of multicellular layers (MCLs) of human colorectal cancer cells (DLD-1) was established. In an attempt to deliver Dicer substrate small interfering RNA (DsiRNA), chitosan (CS) nanoparticles have been developed for targeting vascular endothelial growth factor (VEGF) gene for tumor growth inhibition. The DsiRNA-CS nanoparticles prepared by ionic gelation method had provided maximal protection of DsiRNA in full human serum up to 48 h incubation. RT-PCR studies revealed significant concentration- and time-dependent knock-down of VEGF mRNA and its product due to uniform penetration of DsiRNA-CS nanoparticles throughout MCLs. Taken together, this study also demonstrated that DsiRNA-CS nanoparticles could effectively knock down VEGF gene as therapeutic target in monolayer culture or in solid tumor model for potential treatment of human colorectal carcinoma.

1. Introduction

RNA interference (RNAi) was first identified in C. elegans in 1998 and subsequently in mammalian cells as a posttranscriptional gene silencing mechanism [1]. Within a decade, RNAi has developed into a tool for functional molecular genetics, target gene validation in drug discovery, and a novel therapeutic strategy [2, 3]. Small interfering RNA- (siRNA-) induced RNAi is considered to be a treatment modality for human diseases including cancers [4, 5]. However, nonspecific effects triggered by siRNAs complicate the use of RNAi for specifically downregulating gene expression [6]. It has been recently shown that chemically synthesized DsiRNA (27 bp duplexes) is more potent than traditional siRNA (21 bp duplexes) [7]. Use of DsiRNA to trigger RNAi should result in enhanced efficacy and increased longevity of RNAi, at lower concentrations than that of siRNA [8]. Unlike siRNA, DsiRNA is bound and cleaved by Dicer and then passed into the RNAi-induced silencing complex (RISC) assembly in a sequence-specific orientation [6].

Stability in biological fluids and effective delivery constitute the main challenges for RNA-based therapeutics [9–11]. Thus, carrier or transport system is the main constituent in any in vitro/in vivo DsiRNA experiment. Despite the advantages of DsiRNA, the selection of a correct transfection agent that will proficiently protect and deliver DsiRNA to the tissues and provide a sustained release for additional processing is vital. Viral delivery systems are frequently associated with safety and immunogenicity concerns [12]. Thus, nonviral transfection systems are more attractive to researchers and allow for better control of siRNA concentration and more foreseeable toxicity patterns. Among the nonviral delivery carriers, chitosan (CS) is a widely used cationic polymeric gene carrier [13–15]. CS is a linear polysaccharide composed of glucosamine and N-acetyl glucosamine residues and can be derived by the partial deacetylation of chitin [16]. CS is known to be biocompatible, minimally toxic, nonimmunogenic, and degradable by enzymes [17–20].

Human malignancies are target diseases for siRNA-based therapeutics, with a long list of potential targets related to aberrant signaling pathways in cancer cells [21]. Angiogenesis in human solid tumors has drawn much attention as a direct treatment strategy and a basis for universal chemosensitization [22]. VEGF is an important angiogenic factor associated with tumor growth and metastasis in a wide variety of solid tumors [23–25]. Three-dimensional (3D) in vitro models of human solid tumors mimic the in vivo conditions of solid tumor avascular microregions, including the 3D architecture, cell density, abundance of extracellular matrix (ECM), and cell-cell and cell-ECM communications. These models are the best in vitro models for studying spatial drug distribution as a function of tissue depth (distance from drug exposure side) and possibly drug activity in situ [26, 27].

In the present study, DsiRNA was successfully loaded into CS nanoparticles using the ionic gelation method. DsiRNA-CS nanoparticles were characterized by their particle size, zeta potential, morphology, binding and entrapment efficiency, in vitro release, cytotoxicity, cellular uptake, and gene silencing activity in 2D cell culture. The stability of the DsiRNA-CS nanoparticles was also determined in FBS and human serum. Moreover, a solid tumor model (3D) of DLD-1 cells was successfully established in vitro. The solid tumor model was used to evaluate the penetration of VEGF DsiRNA vectorized by CS nanoparticles and its ability to inhibit tumor growth. The penetration study was performed using 6-FAM-labeled DsiRNA entrapped in CS nanoparticles against naked 6-FAM DsiRNA. Finally, their efficacy was determined by in vitro gene silencing and ELISA analysis of the solid tumor model.

2. Material and Methods

2.1. Materials

Low-molecular-weight (192 kDa) CS with a 75–85% degree of deacetylation (DD) was obtained from Sigma-Aldrich (St. Louis, MO, USA) and pentasodium tripolyphosphate (TPP) was obtained from Merck (Darmstadt, Germany). DsiRNA targeting the VEGF gene [5′-rGrGrArGrUrArCrCrCrUrGrArUrGrArGrArUrCrGrArGrUAC-3′ (sense strand) and 5′-rGrUrArCrUrCrGrArUrCrUrCrArUrCrArGrG rGrUrA rCrUrCrCrCrA-3′ (antisense strand)] of 27 bp in length was purchased from Integrated DNA Technologies (IDT) (USA). Chinese hamster lung fibroblasts (V79) and human colorectal adenocarcinoma cells (DLD-1) were obtained from American Type Culture Collection (ATCC, USA). Human umbilical vein endothelial cells (HUVECs), Medium 200, low serum growth supplement (LSGS), Roswell Park Memorial Institute medium (RPMI) 1640, and Dulbecco’s Modified Eagle’s Medium (DMEM) were purchased from Gibco (USA).

PureLink RNA Mini Kit, Lipofectamine RNAiMAX, PureLink DNase, SuperScript VILO MasterMix First Strand Synthesis SuperMix for RT-PCR, and PlatinumTaq DNA Polymerase were purchased from Life Technologies (Carlsbad, USA). Hoechsct 33342 stain was obtained from Thermo Scientific Dharmacon (USA). The live/dead cell viability assay kit and human VEGF Elisa kit were purchased from Invitrogen (USA). Fluorescein-labeled siRNA and DsiRNA were purchased from IDT (USA). The collagen-coated microporous membrane (0.4 μm pore size) was purchased from Invitrogen (USA). The 4% w/v precast agarose gel electrophoresis cassettes were purchased from Invitrogen, USA. Hematoxylin and Eosin (H & E) stains were purchased from Sigma-Aldrich (USA). The alamarBlue reagent was purchased from Invitrogen (USA).

2.2. Methods

2.2.1. Preparation of CS Nanoparticles

CS nanoparticles were prepared via the ionic gelation method with some modifications [28]. A series of CS solutions (0.1%, 0.2%, 0.3%, and 0.4% w/v) were prepared by dissolving the required amount of CS in 2% v/v glacial acetic acid. TPP solution of 0.1% w/v was prepared by separately dissolving TPP in deionized distilled water. CS nanoparticles were prepared by adding 1.2 mL of the TPP aqueous solution dropwise to the CS solution (0.1%, 0.2%, 0.3%, and 0.4% w/v) at 700 rpm for 30 min. Centrifugation (Optima L-100 XP Ultracentrifuge, Beckman-Coulter, CA, USA) was performed at 35,000 rpm at 10°C for 30 min to collect nanoparticles.

2.2.2. DsiRNA Entrapment

To incorporate DsiRNA into CS-TPP nanoparticles, 15 μL of DsiRNAs (1.6 μg/μL) was added to 1.2 mL of TPP aqueous solution (0.1% w/v), and this was added to 3 mL of CS solution (0.1%, 0.2%, 0.3%, and 0.4% w/v) under constant magnetic stirring (700 rpm) at 25°C. The particles were then left at 25°C for another 30 min before further analysis.

2.2.3. Preparation of MCLs

DLD-1 cells were maintained in RPMI-1640 and supplemented with 5% pen-strep and 10% heat-inactivated FBS in a humidified, 5% (v/v) CO₂ atmosphere at 37°C. Cells were grown on collagen-coated microporous (0.4 μm) membranes in transwell inserts with a plating density of 3 × 10⁵ cells/100 μL [29].

The transwell inserts containing 2 mL of complete RPMI-1640 medium in each insert were placed in a 6-well plate containing 2.5 mL of complete RPMI-1640 medium in each well, followed by occasional agitation [30]. The RPMI-1640 medium was replaced with fresh RPMI-1640 complete medium daily. After 6 days of culturing, MCLs were obtained. MCL thickness was measured using an optical microscope (Olympus, Japan). Each transwell insert was transferred to a new 6-well plate containing 5 mL of RPMI-1640 complete medium in each well for subsequent exposure to DsiRNA and DsiRNA-CS nanoparticles. Briefly, the transwell inserts were supplemented with 2 mL of complete RPMI-1640 medium in which naked DsiRNA/DsiRNA-Lipofectamine (negative/positive control) and DsiRNA-CS nanoparticles were added to the RPMI-1640 medium for direct exposure with MCLs. The 6-well plates were maintained in an incubator with a humidified atmosphere containing 5% CO₂ at 37°C and supplemented with complete RPMI-1640 medium throughout the duration of the experiment.

2.2.4. In Vitro Characterization of DsiRNA-CS Nanoparticles

Determination of Particle Size, Zeta Potential, and Polydispersity Index (PDI). The mean particle diameter (z-average), polydispersity index (PDI), and zeta potential (surface charge) of freshly prepared CS nanoparticles were determined by photon correlation spectroscopy (PCS) using a ZS-90 Zetasizer (Malvern Instruments, Worcestershire, UK). All measurements were performed after the samples were harvested by centrifugation and resuspended in deionized distilled water. Each sample was assayed in triplicate at 25°C, and data are reported as mean ± standard deviation.

Morphological Analysis. Morphological characterization of DsiRNA-CS nanoparticles was carried out using transmission electron microscopy (TEM) (Tecnai Spirit, FEI, Eindhoven, The Netherlands) and AFM NTEGRA Prima (NT-MDT, Russia).

Entrapment Efficiency. The entrapment efficiency of DsiRNA (% entrapped) was measured using a UV-vis spectrophotometer (Shimadzu UV-1800, Shimadzu Scientific Instruments, Japan) at 260 nm. Briefly, the free DsiRNA in the supernatant recovered from centrifugation (13,000 ×g at 10°C for 30 min) was quantified by measuring its absorbance at a wavelength of 260 nm with a dual beam UV-vis spectrophotometer. The concentration of free DsiRNA was determined using Beer’s Law () where is the concentration of DsiRNA, is the absorbance at 260 nm, is the extinction coefficient, and is the path length of the cuvette. Extinction coefficient of DsiRNA is 518500 L mol⁻¹ cm⁻¹ and entrapment efficiency was calculated using the following formula:where is the concentration of DsiRNA added and is the concentration of DsiRNA in the supernatant. All measurements were performed in triplicate, and data are reported as mean ± SD.

Gel Retardation Assay. The binding efficiency of DsiRNA to CS nanoparticles was determined using 4% w/v agarose gel electrophoresis and SYBR® Green (Invitrogen, Carlsbad, CA, USA) staining. Twenty microliters of sample (prepared at various CS concentrations) containing 0.15 μg of DsiRNA was loaded into the wells.

Heparin Displacement Assay. Heparin sodium (10 mg/mL) was added into DsiRNA-CS nanoparticles suspended in deionized distilled water (containing 0.6 μg of DsiRNA). The mixture was incubated at 25°C for 1 h to displace DsiRNA from CS-TPP nanoparticles. The binding affinity was observed by 4% w/v gel electrophoresis. Electrophoresis was performed for 30 min at 110 V and DsiRNA bands were visualized under a real-time UV transilluminator at 480 nm (Invitrogen, Carlsbad, CA, USA).

2.2.5. Stability Studies

Serum Protection Assay (FBS and Human Serum). This assay and the following experiments were performed for DsiRNA-CS nanoparticles prepared with a CS concentration of 0.3% w/v. This concentration was selected because of the desired characteristics (small nanosize, net positive charge, high entrapment efficiency, and binding efficiency) exhibited by the resultant particles. A volume of 200 μL of DsiRNA-CS nanoparticles was incubated at 37°C with an equal volume of RPMI supplemented with 10% FBS. Naked DsiRNA acted as a control and was treated in the same manner. At each predetermined time interval (0 and 30 min and 2, 4, 24, and 48 h), 40 μL of the mixture was removed and stored at −20°C to stop the reaction. Prior to gel electrophoresis, the samples were incubated in a bath incubator at 60°C for 3 min to terminate serum activity. A volume of 5 μL of heparin (1000 U/mL) was then added to displace DsiRNA from the CS nanoparticles. The structure integrity of DsiRNA displaced from nanoparticles was then analyzed by gel electrophoresis with 4% w/v agarose gel stained with SYBR Green (Invitrogen, Carlsbad, CA, USA). Moreover, a human serum protection assay was also performed in which 200 μL of DsiRNA-CS nanoparticles was incubated with an equal volume of human serum at 37°C. Naked DsiRNA was used as a control.

Quantification of DsiRNA. DsiRNA bands obtained from the serum protection assay were quantified using ImageJ software, developed by the National Institutes of Health (NIH) (Maryland, US). The mean area, percent, and relative density of each band were determined using the software.

Storage Stability. DsiRNA-CS nanoparticles were suspended in deionized distilled water/PBS and stored at 4 and 25°C for 15 days. The storage stability of the nanoparticles was determined by measuring their particle size at predetermined time points. Deionized distilled water was used in this experiment in order to investigate the stability of nanoparticles in their resuspending medium. This was performed to help identify a strategy for stabilizing the particles.

2.2.6. In Vitro Release Studies

The release profile of the DsiRNA-CS nanoparticles was studied in PBS at pH 7.4. Samples (4 mL) were centrifuged at 35,000 rpm for 30 min at 25°C, and the pellets were resuspended in PBS (3 mL) at pH 7.4. The mixture was placed on magnetic stirrer with a stirring speed of 100 rpm at 37°C for 15 days. At predetermined time intervals, samples were centrifuged at 35,000 rpm for 30 min at 25°C. Then, a whole volume of supernatant was taken for analysis and replaced with an equivalent volume of fresh buffer solution. The amount of DsiRNA released in the supernatant was analyzed by a UV-vis spectrophotometer (Shimadzu 1800) at a wavelength of 260 nm.

2.2.7. Cytotoxicity Studies

The V79 cell line (ATCC, Manassas, VA, USA) was cultured in DMEM supplemented with 10% FBS and 1% pen-strep at a seeding density of 2 × 10⁴ cells per well. The DLD-1 cells (ATCC, Manassas, VA, USA) were cultured in RPMI-1640 medium supplemented with 10% FBS and 1% pen-strep at a seeding density of 4 × 10⁴ cells per well. Moreover, the HUVECs (Gibco, USA) were cultured in medium 200 at a seeding density of 3 × 10⁴ cells per well. The HUVECs were supplemented with 10% LSGS and 1% pen-strep. All cells were incubated with DsiRNA-CS nanoparticles for 24 and 48 h.

After 24 and 48 h incubation of samples with cells, a final dilution of 1/10 per cell volume of alamarBlue reagent was added to the treated cells, followed by incubation for 4 h prior to analysis. The absorbance of each sample at 570 nm (A570) was measured using a microplate reader (Varioskan Flash, Thermo Scientific, Waltham, MA, USA). All cells were maintained at 37°C in a humidified 5% CO₂/95% air atmosphere.

Cell viability of all the samples was determined using the following equation:

2.2.8. LIVE/DEAD Cell Viability Assay

A cell viability assay was performed to measure the functional status of the cells by detecting cytoplasmic esterase activity using the LIVE/DEAD Viability/Cytotoxicity kit for mammalian cells (Invitrogen, Carlsbad, CA, USA). The kit contains calcein, which stains living cells (green), and ethidium bromide, which stains dead cells (red). This assay was performed in 96-well plates. Briefly, DLD-1 cells were plated at a seeding density of 4 × 10⁴ cells per well. The cells were supplemented with 10% FBS and 1% pen-strep and maintained at 37°C in a humidified 5% CO₂/95% air atmosphere. The cells were treated with DsiRNA-CS nanoparticles for 24 and 48 h. Subsequently, the cells were rinsed twice with PBS, followed by adding fluorochromes (calcein/ethidium bromide). The cells were treated with DsiRNA-CS treated with DsiRNA-CS nanoparticles for 24 and 48 h and incubating for 45 min. The reagents were removed by rinsing with PBS followed by analysis using a Floid Cell Imaging Station (Molecular Probes Life Technology, France).

2.2.9. Cellular Internalization

DLD-1 cells (4 × 10⁴) were seeded in a 6-well tissue culture plate and incubated for 24 h (80% confluence). The cells in each well were incubated for 4 h in a medium with 10% FBS at 37°C with free 6-FAM-DsiRNA or with DsiRNA-CS nanoparticles. After incubation, the cells were washed twice with PBS and then stained with 1 μg/mL of Hoechst stain 33342 for 15 min at 37°C. Cellular internalization of DsiRNA was examined using a Floid Cell Imaging Station (Molecular Probes Life Technology, France).

2.2.10. In Vitro Gene Silencing

Investigation of VEGF mRNA Suppression Using RT-PCR. To evaluate the gene silencing activity of DsiRNA-CS nanoparticles in comparison to controls, DLD-1 cells were seeded with 2 mL of RPMI 1640 containing 10% FBS on a 6-well plate at 5 × 10⁴ cells/well. After 24 h, samples and controls were added with fresh medium (80 pmol DsiRNA) and incubated for another 24 h. The cells were then harvested and RNA was extracted using a PureLink RNA Mini Kit and PureLink DNase, as recommended by the manufacturer (Life Technologies, Carlsbad). In this experiment, samples consisted of a negative control (Lipofectamine and scrambled DsiRNA), positive control (Lipofectamine and VEGF DsiRNA), and DsiRNA-CS nanoparticles. The concentration of DsiRNA was kept constant in all formulations.

After obtaining RNA from the cells, the quality of RNA was assessed by 1% w/v agarose gel electrophoresis at 90 V for 60 min in Tris-acetate-EDTA (TAE) buffer and visualized by ethidium bromide staining. RNA was quantified using the Infinite 200 PRO NanoQuant (Tecan, Switzerland). The gel images were taken by an image reader (Fujifilm LAS-3000, Tokyo, Japan). In the next step, complementary DNA (cDNA) was prepared from 1.5 μg total RNA by reverse transcription using SuperScript VILO Master Mix (Life Technologies, Carlsbad) for RT-PCR according to the manufacturer’s instructions. For the VEGF gene, the forward and reverse primers were 5′-AGTGGTCCCAGGCTGCAC-3′ and 5′-TCCATGAACTTCACCACTTCGT-3′, respectively, whereas for the reference gene, GAPDH, the forward and reverse primers were 5′-ACCACAGTCCATGCCATCAC-3′ and 5′-TCCACCACCCTGTTGCTGTA-3′, respectively (1st Base, Singapore). The RT-PCR was carried out in an Eppendorf Mastercycler Nexus Gradient Thermal Cycler (Hamburg, Germany). Amplification products were resolved by 1% w/v agarose gel electrophoresis at 90 V for 60 min in TAE buffer and visualized by ethidium bromide staining. The images of the gel were taken by an image reader (Fujifilm LAS-3000, Tokyo, Japan). The densitometric analysis was performed using imageJ software.

Morphology and Thickness of MCLs. The morphology of the collagen layer and MCLs was observed using scanning electron microscopy (SEM). Cross-vertical sections (10 μm) of MCLs were stained with H & E and observed under an optical microscope. Thickness of MCLs was measured by using the optical microscope software. All measurements were performed in triplicate, and data are reported as mean ± SD.

Gene Silencing within MCLs. MCLs were exposed to naked DsiRNA and DsiRNA-CS nanoparticles (DsiRNA concentrations of 20 and 80 pmol) for 24 and 48 h at 37°C in a humidified 5% CO₂/95% air atmosphere. At the end of the exposure time, MCLs with collagen membranes attached were cut out of the transwell inserts using a surgical blade (size number 10), fixed with 4% paraformaldehyde, and embedded in paraffin wax and later stained with H & E. Cross-vertical sections (10 μm) were observed using an optical microscope.

ELISA Analysis of VEGF Protein in Medium. MCLs were exposed to naked DsiRNA, Lipofectamine-DsiRNA, and DsiRNA-CS nanoparticles for 24 and 48 h in cell culture conditions. In each sample, the concentration of DsiRNA used was 80 pmol. At the end of the exposure time, the culture medium in the bottom chamber was collected and centrifuged to remove cell debris. The amount of VEGF secreted from the MCLs was determined using the Quantikine® human VEGF immunoassay kit (Ambion, USA), according to the manufacturer’s instructions. All measurements were performed in triplicate and data are reported as mean ± SD.

DsiRNA Distribution within MCLs. MCLs were exposed to DsiRNA by adding naked 6-FAM-labeled DsiRNA (control) and DsiRNA-CS nanoparticles (80 pmol) to the transwell and incubated for 24 and 48 h. At the end of incubation, cells were rinsed with PBS (pH 7.4) and fixed with 4% paraformaldehyde for 1 h. Thereafter, samples were embedded in liquid nitrogen-cooled optimal cutting temperature compound (Tissue-Tek®, Miles Laboratories, USA). Then, 20 μm thick cross-vertical sections of MCLs were prepared using a cryostat (Leica CM1900, Wetzlar, Germany). The slides were mounted using polyvinyl alcohol mounting medium with 1,4-diazabicyclo[2.2.2]octane and a cover slip. The DsiRNA distribution was observed by fluorescence microscope (Carl Zeiss, Germany).

2.3. Statistical Analysis

Data was presented as mean ± SD. The data were analyzed using independent -test or analysis of variance (One-way ANOVA, followed by Tukey post hoc analysis) using SPSS 20.0 (SPSS Inc., Chicago, IL). Values of indicated statistical significance between the groups tested.

3. Results

3.1. Particle Size, PDI, Zeta Potential, and Morphology

The mean particle size of DsiRNA-CS nanoparticles was significantly increased by increasing the CS concentration from 0.1% to 0.4% w/v (Table 1). All the nanoparticles had a low to moderate PDI value in the range of 0.30 to 0.55, varying with CS concentration. This could be explained by the process of DsiRNA association during the preparation of CS nanoparticles. DsiRNA and TPP were mixed together to produce a solution that was later added dropwise to CS solution. This technique was expected to provide a better condition for efficient and controllable incorporation of DsiRNA into CS nanoparticles which yielded smaller particles. This finding is in accordance with previous reports [31, 32].

The zeta potential of DsiRNA-CS nanoparticles increased with increasing CS concentration at a constant DsiRNA concentration as shown in Table 1. Unloaded CS-nanoparticles had zeta potentials in the range of + to + (Table S1 in Supplementary Material available online at http://dx.doi.org/10.1155/2016/7201204) when CS concentration ranged from 0.1% to 0.4% w/v. However, these values were not significantly decreased when DsiRNA was entrapped into the nanoparticles. This could be due to the small number of DsiRNA phosphate groups that were available to interact with CS groups. Particle size of DsiRNA loaded nanoparticles was smaller compared to unloaded ones that could be attributed by better interactions between CS polymers and TPP in the presence of DsiRNA even in a small number of phosphate groups. In comparison to siRNA, the larger size of the DsiRNA duplex (27 mer, MW 16,558 g/mol) could be attributed to the small number of available negatively charged phosphate groups to compensate for groups of CS [33]. This explains the finding that DsiRNA loading had less of an effect on the overall surface charge of CS nanoparticles. This effect might be due to a large amount of DsiRNA buried in the matrices of CS nanoparticles by the entrapment method, resulting in less density of negative charge.

AFM micrographs of DsiRNA-CS nanoparticles prepared from 0.3% w/v CS revealed a spherical morphology (Figures 1(a) and 1(b)). Moreover, spherical morphology was also observed for DsiRNA-CS nanoparticles prepared at different CS concentrations using TEM as depicted in Figures 1(c), 1(d), 1(e), and 1(f). Thus, the results suggested that different CS concentrations and DsiRNA entrapment had no effect on the morphology of CS nanoparticles. The spherical shape of DsiRNA-CS nanoparticles could be governed by the electrostatic interactions between DsiRNA and CS as well as between TPP and CS, provided for controllable gelation of CS.

(a)

(b)

(c)

(d)

(e)

(f)

3.2. DsiRNA Entrapment and Binding Efficiencies

A higher DsiRNA entrapment efficiency was obtained (92% to 100%) for CS nanoparticles when CS concentration was increased from 0.1% to 0.4% w/v as measured by UV-vis spectrophotometry and shown in Figure 2(a). Entrapment efficiency of DsiRNA into CS nanoparticles was therefore influenced by CS concentration. Higher entrapment efficiency was achieved due to stronger electrostatic attraction between DsiRNA molecules with a higher density of oppositely charged CS.

(a)

(b)

(c)

Strong binding between DsiRNA and CS nanoparticles was observed (due to the absence of a trailing band), as shown in Figure 2(b). Absence of a band indicated immobilization of DsiRNA, which was probably due to efficient entrapment within the nanoparticles’ matrices and strong binding of DsiRNA that was located on the nanoparticles’ surfaces. However, DsiRNA is expected to be gradually released from the nanoparticles following degradation of the polymeric matrices [34, 35].

In heparin displacement assay experiment, heparin was used to displace DsiRNA from CS nanoparticles prepared with different CS concentrations (0.1%, 0.2%, 0.3%, and 0.4% w/v), as shown in Figure 2(c). The results suggested that DsiRNA was reversibly bound to CS nanoparticles. Despite that, a higher concentration of heparin (10 mg/mL) was needed to displace entrapped DsiRNA from CS nanoparticles suggesting stronger binding between entrapped DsiRNA (those located on/near to the particles’ surfaces) and CS nanoparticles. Meanwhile, the release of entrapped DsiRNA within the matrices might occur when the polymer’s matrices start to hydrate and swell. Moreover, a similar migration distance of the bands to the control (naked DsiRNA) further indicated that CS nanoparticles were able to load DsiRNA without altering its molecular structure.

3.2.1. Stability of DsiRNA-CS Nanoparticles

The ability of a carrier to protect its payload from nuclease degradation is an important property for efficient gene delivery. Similar to siRNA, DsiRNA must also be protected from nuclease digestion for maximal activity in the cells. To address this, a serum protection test was carried out for CS nanoparticles in 10% FBS. Naked DsiRNA started to degrade as early as 0 min due to degradation during mixing and freezing steps as shown in Figure 3(a). Naked DsiRNA was almost totally degraded after 48 h incubation in FBS. On the other hand, CS nanoparticles were able to completely protect the entrapped DsiRNA from nuclease degradation for up to 48 h incubation as indicated by DsiRNA bands with similar brightness and migration distance as those before the treatment (0 min). The bands were quantitatively analyzed using ImageJ software as shown in Figure 3(b). The relative density of DsiRNA bands released from CS nanoparticles was higher than naked DsiRNA. Therefore, CS nanoparticles were effectively protecting DsiRNA from the enzymatic activity of serum components.

(a)

(b)

Currently, to our knowledge, there is no information regarding the stability and integrity of DsiRNA-carriers in human serum. Knowledge about the effects of human serum on the stability of DsiRNA-carriers may help in the development of new, more promising DsiRNA-carriers. This experiment was conducted using DsiRNA-CS nanoparticles. Naked DsiRNA started to degrade at as early as 0 min incubation as shown in Figure 4. The smeared or diffused bands were observed after 30 min incubation of naked DsiRNA in human serum and the same observation was obtained after 48 h incubation. Moreover, migration distance of trailing bands after 30 min incubation increases in comparison to 0 min and control bands indicate degradation of DsiRNA by serum nucleases. The smeared naked DsiRNA is probably due to the presence of autofluorescent proteins or interactions with SYBR Green dye [36]. This finding is in accordance with the previous reports about naked siRNA in human serum [36, 37]. CS nanoparticles effectively protected DsiRNA from the activity of serum nucleases for up to 48 h of incubation as indicated by the appearance of bands of similar brightness and migration distance to the DsiRNA band before the treatment (0 min). However, interpretation and quantification of the relative density of the DsiRNA bands in the presence of human serum could not be obtained because the diffused bands were difficult to quantify.

3.2.2. Storage Stability

The study was performed in deionized distilled water or PBS (pH 7.4) for 15 days. The storage stability of DsiRNA-CS nanoparticles (CS concentration of 0.3% w/v) in deionized distilled water at 4°C and 25°C is shown in Figures 5(a) and 5(b), respectively. The results demonstrated that DsiRNA-CS nanoparticles were stable in deionized distilled water, as particle size remained unchanged at both temperatures. Similar findings were obtained when DsiRNA-CS nanoparticles were suspended in PBS and stored at 4°C and 25°C, as shown in Figures 5(c) and 5(d), respectively. The cross-linking effect of TPP in the formation of DsiRNA-CS nanoparticles confers its action as a stabilizer, producing structures, which are less prone to aggregations [38].

(a)

(b)

(c)

(d)

3.2.3. In Vitro Release

The in vitro release study of DsiRNA from CS nanoparticles (CS concentration of 0.3% w/v) was carried out using PBS at pH 7.4 for 15 days (Figure 6). A rapid release in the first four days was also observed for these nanoparticles, resulting in an 18% cumulative release of DsiRNA. The rapid release might be attributed by the release of loosely bound DsiRNA located near or on the particles’ surfaces. From day 5 until the last day of the experiment, DsiRNA was released from CS nanoparticles at a constant rate with 40% total cumulative release of DsiRNA. The release at this stage might be due to erosion or a combination of erosion and diffusion processes of the nanoparticles’ matrices as previously reported [39].

3.2.4. Cytotoxicity

The cytotoxic effect of DsiRNA-CS nanoparticles was investigated in V79, DLD-1, and HUVECs cell lines by an alamarBlue cell viability assay. In V79 cells, only a 5–11% loss of cell viability was observed for DsiRNA-CS nanoparticles as shown in Figure 7(a). The cytotoxicity of DsiRNA-CS nanoparticles was not significantly different between 24 and 48 h incubations. Generally, cell viability decreased as CS concentration used to prepare the nanoparticles increased from 0.1% to 0.4% w/v.

(a)

(b)

(c)

In the DLD-1 cell line, DsiRNA-CS nanoparticles caused a cytotoxic effect after 24 and 48 h incubation as shown in Figure 7(b). The cell viability decreased significantly as the CS concentration used to prepare CS nanoparticles increased from 0.1% to 0.4% w/v due to a higher density of positive charges in the CS. This condition induced unspecific interactions with the cell membranes, destroying the integrity of the cell membrane [40, 41]. The cytotoxicity of DsiRNA-CS nanoparticles in DLD-1 cells was further increased after 48 h incubation. The loss of cell viability of DLD-1 cells was expected to be greater than that of the normal cells because CS has the ability to inhibit the growth of human cancer cells through an antiangiogenic mechanism [42].

HUVECs are isolated from the vein of the umbilical cord and are commonly used for physiological and pharmacological investigations involving macromolecule transport, blood coagulation, angiogenesis, and fibrinolysis. In addition, HUVECs are also available which are prescreened for VEGF response. VEGF is an important signaling protein involved in both vasculogenesis and angiogenesis. In vitro, VEGF has been shown to stimulate endothelial cell mitogenesis, cell migration, sprouting, and microvascular permeability. In HUVECs, a 7–18% loss of cell viability was observed when the cells were treated with DsiRNA-CS nanoparticles (Figure 7(c)). Different CS nanoparticles made from various CS concentrations did not significantly affect the cell viability after 24 and 48 h incubation even though a deceasing trend in cell viability could be seen. A significant decrease in cell viability was observed after 48 h incubation compared to 24 h incubation, suggesting the progressiveness of the cytotoxicity effect over time. This could be due to the silencing activity of DsiRNA against the targeted VEGF gene resulting in cell death. Therefore, it can be concluded that CS nanoparticles have the potential ability to deliver DsiRNA into the target site and could be applied in cancer therapy by inhibiting angiogenesis, which may control tumor growth and metastasis [43]. However, further investigation is necessary to address this effect.

For LIVE/DEAD cell viability assay, the results showed that untreated cells did not produce any loss of cell viability (Figure 8(a)(A) and (D)), while some loss was observed in the cells treated with naked DsiRNA (Figure 8(a)(B) and (E)). These results are in accordance with the results from the cytotoxicity assays using alamarBlue that also showed some cell death (red color) after 24 h of the cells treated with DsiRNA-CS nanoparticles (Figure 8(a)(C)). Furthermore, an increase in cell death was observed after 48 h incubation as indicated by the presence of red color (dead cells), as shown in Figure 8(a)(F).

(a)

(b)

3.2.5. DsiRNA Internalization/Cellular Uptake

After incubation of DLD-1 cells with 6-FAM-DsiRNA entrapped within CS nanoparticles for 6 h, fluorescence could be detected within the cells. The fluorescence was mainly distributed in the cytoplasm, which is in agreement with previous observations for siRNA cellular uptake and an earlier report (Figures 8(b)(D)–(F)) [44]. However, fluorescence from the naked 6-FAM-DsiRNA could not be detected (Figure 8(b)(A)–(C)). Therefore, the results of this study suggested that DsiRNA entrapped within CS nanoparticles could efficiently deliver DsiRNA into cells, particularly the cytoplasm.

3.2.6. In Vitro Gene Silencing

In order to investigate the silencing activity of VEGF mRNA, RT-PCR was used to determine the VEGF mRNA level in DLD-1 cells. In this experiment, samples consisted of a negative control (Lipofectamine and scrambled DsiRNA), positive control (Lipofectamine and VEGF DsiRNA), and DsiRNA-CS nanoparticles. The concentration of DsiRNA (80 pmol) was kept constant in all formulations. The quality of housekeeping (Figure 9(a)) and VEGF mRNA (Figure 9(b)) was also assessed using 1% w/v agarose gel electrophoresis. A quantitative analysis of VEGF mRNA level was performed using imageJ software (Figure 9(c)). The results showed that the negative control did not show any silencing effect in the target gene. The highest gene silencing activity was observed in the positive control. However, DsiRNA-CS nanoparticles showed a significant decrease in VEGF mRNA level in comparison to the negative control, and this level was comparable to the positive control. The high gene silencing activity of DsiRNA-CS nanoparticles compared to a positive control was expected because, as previously discussed, these particles provided maximum stability in FBS and human serum. Interestingly, a very low concentration of DsiRNA (80 pmol) was used in this study which is lower than the concentration of siRNA (100–250 nmol) commonly used to silence target genes. Thus, DsiRNA was found to be more potent than siRNA in silencing the VEGF gene.

(a)

(b)

(c)

(d)

(e)

(f)

3.2.7. Morphology of MCLs

The morphology of the collagen layer and 6 days of growth of MCLs was examined using SEM (Figures 9(d), 9(e), and 9(f)). The results showed that MCLs were tightly attached to the collagen layer (basement membrane). Cells were difficult to view on the surface due to the secretion of a large amount of ECM, as reported previously [45]. The collagen layer can be observed in Figure 9(d). MCLs that attached to the collagen layer as a basement membrane can be observed in Figures 9(e) and 9(f).

3.2.8. VEGF Gene Silencing within MCLs

Across a wide range of human tumors and/or cell lines, expression of VEGF leads to the development and maintenance of a vascular network that promotes tumor growth. Moreover, evidence obtained from tumor studies indicates the involvement of both VEGF gene expression and VEGF production in tumor growth. Thus, the MCLs thickness is correlated with VEGF expressions reported elsewhere [29]. The thickness of MCLs without treatment was calculated using software (Analysis LS Report) and an optical microscope. The thickness was calculated to be in the range of . The expression of VEGF mRNA was determined within the MCLs after exposure to naked DsiRNA and DsiRNA-CS nanoparticles (20 and 80 pmol) targeting VEGF after 24 and 48 h incubations. This concentration was used because the risk of off-target effects can be reduced if the DsiRNA concentration is below 100 pmol when the effective transfection reagent and protocol are applied [7]. No significant changes in VEGF mRNA levels were observed in MCLs when treated with naked DsiRNA in comparison to the untreated control group (Figures 10(a)(A) and (B)), indicating the absence of a gene silencing effect. On the other hand, the VEGF mRNA level decreased significantly compared to the untreated control group when MCLs were exposed to DsiRNA-CS nanoparticles (20 and 80 pmol) after 24 and 48 h incubations (Figures 10(a)(C)–(F)). The results also showed that DsiRNA-CS nanoparticles caused a higher loss of VEGF mRNA at 80 pmol (Figures 10(a)(E) and (F)) in comparison to 20 pmol as shown in (Figures 10(a)(C) and (D)). Moreover, a higher reduction of VEGF mRNA was observed at both concentrations after 48 h incubation as shown in Figures 10(a)(D) and (F). Thus, the gene silencing effect in MCLs was concentration- and time-dependent, showing more suppression at higher concentrations and longer incubation periods. In addition, DsiRNA could be used to silence target genes associated with solid tumors at a 2.5-fold lesser concentration than siRNA, and this could help with avoiding off-target effects.

3.2.9. ELISA Analysis for VEGF Protein in MCLs

The VEGF levels in MCLs were determined by ELISA after exposure to naked DsiRNA, CS nanoparticles (unloaded), and DsiRNA-CS nanoparticles for 24 and 48 h. A DsiRNA concentration of 80 pmol was used in all formulations. The results showed that naked DsiRNA did not exert any significant reduction in the VEGF level in MCLs when compared to untreated cells (Figure 10(b)). This finding is in accordance with the previous report on siRNA [29]. Moreover, Figure 10(b) shows a significant reduction in VEGF levels when MCLs were treated with DsiRNA-CS nanoparticles in comparison to untreated cells. The significant decrease in VEGF level was also observed after 48 h exposure of DsiRNA-CS nanoparticles. This significant decrease in VEGF level might be due to maximum protection of DsiRNA provided by the CS nanoparticles in FBS and human serum as discussed above.

(a)

(b)

3.2.10. DsiRNA Distribution within MCLs

DsiRNA distribution in MCLs was evaluated upon exposure of 6-FAM-labeled naked DsiRNA entrapped into CS nanoparticles (80 pmol) for 24 and 48 h. The naked DsiRNA (control) only showed some fluorescence on the surface of MCLs with no penetration observed up to 48 h incubation (Figures 11(a) and 11(b)). For DsiRNA-CS nanoparticles, distribution was limited to the middle layer of MCLs after 24 h incubation (Figures 11(c) and 11(e)). However, after 48 h incubation complete and uniform penetration of DsiRNA was observed which could be detected by fluorescence throughout the MCLs (Figures 11(d) and 11(f)). Cell detachment from MCLs was also observed after 48 h, indicating that the silencing effect of the target gene had subsequently contributed to the antitumor effect. This effect is in accordance with the previous findings that showed a significant reduction in VEGF levels caused by DsiRNA-CS nanoparticles and the effect was more pronounced after 48 h. Fluorescence signals detected within MCLs demonstrated the ability of CS nanoparticles to deliver DsiRNA into cells and induce the RNAi effect as reported elsewhere [29].

(a)

(b)

(c)

(d)

(e)

(f)

4. Conclusions

DsiRNA-CS nanoparticles that had a small particle size, positive surface charge, regular morphology, high encapsulation efficiency, and exhibited sustained release of DsiRNA were successfully prepared by the ionic gelation method. Moreover, these nanoparticles provided maximal protection of DsiRNA in 10% FBS and human serum for up to 48 h incubation. Cytotoxic effects were determined to be dependent on the concentration of CS in the case of V79 and DLD-1 cells and otherwise in the case of HUVECs. Moreover, DsiRNA-CS nanoparticles were successfully internalized into DLD-1 cells. RT-PCR studies revealed that DsiRNA entrapped within CS nanoparticles could highly downregulate VEGF mRNA levels in DLD-1 cells. The solid tumor model (MCLs) was successfully established in vitro. MCLs possessed a compact morphology. The gene silencing effect of MCLs was concentration- and time-dependent, showing greater suppression at 80 pmol and for 48 h incubation. The findings are very promising because the highest DsiRNA concentration of 80 pmol used in this study could effectively result in a gene silencing effect. This concentration is much lower than the concentration needed for siRNA (200 pmol) reported previously [29]. Thus, DsiRNA was more effective for silencing the target gene in solid tumors at a concentration 2.5-fold less than siRNA, and this reduction could prevent off-target effects. Moreover, CS has great prospective applications for DsiRNA delivery. Thus, DsiRNA-CS nanoparticles could be used in future in vivo studies.

Competing Interests

The authors report no competing interests in this work.

Acknowledgments

The authors gratefully acknowledge all the members of Centre for Drug Delivery Research Group for their technical support and advice and the Ministry of Education, Malaysia, for financially supporting the project (ERGS/1/2011/SKK/UKM/02/11).

Supplementary Materials

Table S1 presents particle size, zeta potential and PDI of unloaded CS-TPP nanoparticles prepared at different CS concentration ranging from 0.1% to 0.4% w/v. The mean particle size of CS-TPP nanoparticles was increased significantly by increasing the CS concentration. PDI values of these nanoparticles were from 0.3 to 0.6 and within the acceptable range. The surface charge of CS-TPP nanoparticles ranged from +30.1 ± 1.0 to +59.7 ± 0.5 mV by varying CS concentrations from 0.1% to 0.4% w/v. This was expected because higher CS concentrations have more unneutralised NH3+groups of CS, thus resulting in higher zeta potential.

Supplementary Material

References

S. M. Elbashir, J. Harborth, W. Lendeckel, A. Yalcin, K. Weber, and T. Tuschl, “Duplexes of 21-nucleotide RNAs mediate RNA interference in cultured mammalian cells,” Nature, vol. 411, no. 6836, pp. 494–498, 2001.
View at: Publisher Site | Google Scholar
R. K. M. Leung and P. A. Whittaker, “RNA interference: from gene silencing to gene-specific therapeutics,” Pharmacology and Therapeutics, vol. 107, no. 2, pp. 222–239, 2005.
View at: Publisher Site | Google Scholar
J. S. Kang, Y. N. Yum, E. Han et al., “Evaluation of potential biomarkers for thioacetamide-induced hepatotoxicity using siRNA,” Biomolecules and Therapeutics, vol. 16, no. 3, pp. 197–202, 2008.
View at: Publisher Site | Google Scholar
T. C. Karagiannis and A. El-Osta, “RNA interference and potential therapeutic applications of short interfering RNAs,” Cancer Gene Therapy, vol. 12, no. 10, pp. 787–795, 2005.
View at: Publisher Site | Google Scholar
J. C. Cheng, T. B. Moore, and K. M. Sakamoto, “RNA interference and human disease,” Molecular Genetics and Metabolism, vol. 80, no. 1-2, pp. 121–128, 2003.
View at: Publisher Site | Google Scholar
S. D. Rose, D.-H. Kim, M. Amarzguioui et al., “Functional polarity is introduced by Dicer processing of short substrate RNAs,” Nucleic Acids Research, vol. 33, no. 13, pp. 4140–4156, 2005.
View at: Publisher Site | Google Scholar
D.-H. Kim, M. A. Behlke, S. D. Rose, M.-S. Chang, S. Choi, and J. J. Rossi, “Synthetic dsRNA Dicer substrates enhance RNAi potency and efficacy,” Nature Biotechnology, vol. 23, no. 2, pp. 222–226, 2005.
View at: Publisher Site | Google Scholar
D. Siolas, C. Lerner, J. Burchard et al., “Synthetic shRNAs as potent RNAi triggers,” Nature Biotechnology, vol. 23, no. 2, pp. 227–231, 2005.
View at: Publisher Site | Google Scholar
R. C. C. Ryther, A. S. Flynt, J. A. Phillips, and J. G. Patton, “siRNA therapeutics: big potential from small RNAs,” Gene Therapy, vol. 12, no. 1, pp. 5–11, 2005.
View at: Publisher Site | Google Scholar
J. M. Layzer, A. P. McCaffrey, A. K. Tanner, Z. Huang, M. A. Kay, and B. A. Sullenger, “In vivo activity of nuclease-resistant siRNAs,” RNA, vol. 10, no. 5, pp. 766–771, 2004.
View at: Publisher Site | Google Scholar
S. Choung, Y. J. Kim, S. Kim, H.-O. Park, and Y.-C. Choi, “Chemical modification of siRNAs to improve serum stability without loss of efficacy,” Biochemical and Biophysical Research Communications, vol. 342, no. 3, pp. 919–927, 2006.
View at: Publisher Site | Google Scholar
P. D. Cotter, C. Hill, and R. P. Ross, “Food microbiology: bacteriocins: developing innate immunity for food,” Nature Reviews Microbiology, vol. 3, no. 10, pp. 777–788, 2005.
View at: Publisher Site | Google Scholar
M. Dash, F. Chiellini, R. M. Ottenbrite, and E. Chiellini, “Chitosan—a versatile semi-synthetic polymer in biomedical applications,” Progress in Polymer Science, vol. 36, no. 8, pp. 981–1014, 2011.
View at: Publisher Site | Google Scholar
M. Hamidi, A. Azadi, and P. Rafiei, “Hydrogel nanoparticles in drug delivery,” Advanced Drug Delivery Reviews, vol. 60, no. 15, pp. 1638–1649, 2008.
View at: Publisher Site | Google Scholar
Z. Liu, Y. Jiao, Y. Wang, C. Zhou, and Z. Zhang, “Polysaccharides-based nanoparticles as drug delivery systems,” Advanced Drug Delivery Reviews, vol. 60, no. 15, pp. 1650–1662, 2008.
View at: Publisher Site | Google Scholar
L. Illum, “Chitosan and its use as a pharmaceutical excipient,” Pharmaceutical Research, vol. 15, no. 9, pp. 1326–1331, 1998.
View at: Publisher Site | Google Scholar
J. Malmo, K. M. Vårum, and S. P. Strand, “Effect of chitosan chain architecture on gene delivery: comparison of self-branched and linear chitosans,” Biomacromolecules, vol. 12, no. 3, pp. 721–729, 2011.
View at: Publisher Site | Google Scholar
S. P. Strand, M. M. Issa, B. E. Christensen, K. M. Vårum, and P. Artursson, “Tailoring of chitosans for gene delivery: novel self-branched glycosylated chitosan oligomers with improved functional properties,” Biomacromolecules, vol. 9, no. 11, pp. 3268–3276, 2008.
View at: Publisher Site | Google Scholar
O. Germershaus, S. Mao, J. Sitterberg, U. Bakowsky, and T. Kissel, “Gene delivery using chitosan, trimethyl chitosan or polyethylenglycol-graft-trimethyl chitosan block copolymers: establishment of structure-activity relationships in vitro,” Journal of Controlled Release, vol. 125, no. 2, pp. 145–154, 2008.
View at: Publisher Site | Google Scholar
P. Baldrick, “The safety of chitosan as a pharmaceutical excipient,” Regulatory Toxicology and Pharmacology, vol. 56, no. 3, pp. 290–299, 2010.
View at: Publisher Site | Google Scholar
M. Izquierdo, “Short interfering RNAs as a tool for cancer gene therapy,” Cancer Gene Therapy, vol. 12, no. 3, pp. 217–227, 2005.
View at: Publisher Site | Google Scholar
R. S. Kerbel, “Improving conventional or low dose metronomic chemotherapy with targeted antiangiogenic drugs,” Cancer Research and Treatment, vol. 39, no. 4, pp. 150–159, 2007.
View at: Publisher Site | Google Scholar
F. Fan, J. S. Wey, M. F. McCarty et al., “Expression and function of vascular endothelial growth factor receptor-1 on human colorectal cancer cells,” Oncogene, vol. 24, no. 16, pp. 2647–2653, 2005.
View at: Publisher Site | Google Scholar
D. J. Hicklin and L. M. Ellis, “Role of the vascular endothelial growth factor pathway in tumor growth and angiogenesis,” Journal of Clinical Oncology, vol. 23, no. 5, pp. 1011–1027, 2005.
View at: Publisher Site | Google Scholar
M. Calvani, D. Trisciuoglio, C. Bergamaschi, R. H. Shoemaker, and G. Melillo, “Differential involvement of vascular endothelial growth factor in the survival of hypoxic colon cancer cells,” Cancer Research, vol. 68, no. 1, pp. 285–291, 2008.
View at: Publisher Site | Google Scholar
B. Desoize, “Contribution of three-dimensional culture to cancer research,” Critical Reviews in Oncology/Hematology, vol. 36, no. 2-3, pp. 59–60, 2000.
View at: Publisher Site | Google Scholar
K. O. Hicks, F. B. Pruijn, J. R. Sturman, W. A. Denny, and W. R. Wilson, “Multicellular resistance to tirapazamine is due to restricted extravascular transport: a pharmacokinetic/pharmacodynamic study in HT29 multicellular layer cultures,” Cancer Research, vol. 63, no. 18, pp. 5970–5977, 2003.
View at: Google Scholar
P. Calvo, C. Remuñán-López, J. L. Vila-Jato, and M. J. Alonso, “Novel hydrophilic chitosan-polyethylene oxide nanoparticles as protein carriers,” Journal of Applied Polymer Science, vol. 63, no. 1, pp. 125–132, 1997.
View at: Publisher Site | Google Scholar
A. M. Al-Abd, S. H. Lee, S. H. Kim et al., “Penetration and efficacy of VEGF siRNA using polyelectrolyte complex micelles in a human solid tumor model in-vitro,” Journal of Controlled Release, vol. 137, no. 2, pp. 130–135, 2009.
View at: Publisher Site | Google Scholar
T. Sonoda, H. Kobayashi, T. Kaku, T. Hirakawa, and H. Nakano, “Expression of angiogenesis factors in monolayer culture, multicellular spheroid and in vivo transplanted tumor by human ovarian cancer cell lines,” Cancer Letters, vol. 196, no. 2, pp. 229–237, 2003.
View at: Publisher Site | Google Scholar
S. A. Papadimitriou, D. S. Achilias, and D. N. Bikiaris, “Chitosan-g-PEG nanoparticles ionically crosslinked with poly(glutamic acid) and tripolyphosphate as protein delivery systems,” International Journal of Pharmaceutics, vol. 430, no. 1-2, pp. 318–327, 2012.
View at: Publisher Site | Google Scholar
I. Hajdu, M. Bodnár, G. Filipcsei et al., “Nanoparticles prepared by self-assembly of chitosan and poly-γ-glutamic acid,” Colloid and Polymer Science, vol. 286, no. 3, pp. 343–350, 2008.
View at: Publisher Site | Google Scholar
M. Abdul Ghafoor Raja, H. Katas, Z. Abd Hamid, and N. A. Razali, “Physicochemical properties and in vitro cytotoxicity studies of chitosan as a potential carrier for dicer-substrate siRNA,” Journal of Nanomaterials, vol. 2013, Article ID 653892, 10 pages, 2013.
View at: Publisher Site | Google Scholar
N. Csaba, M. Köping-Höggård, and M. J. Alonso, “Ionically crosslinked chitosan/tripolyphosphate nanoparticles for oligonucleotide and plasmid DNA delivery,” International Journal of Pharmaceutics, vol. 382, no. 1-2, pp. 205–214, 2009.
View at: Publisher Site | Google Scholar
M. E. Martin and K. G. Rice, “Peptide-guided gene delivery,” The AAPS Journal, vol. 9, no. 1, article 3, pp. E18–E29, 2007.
View at: Publisher Site | Google Scholar
K. Buyens, B. Lucas, K. Raemdonck et al., “A fast and sensitive method for measuring the integrity of siRNA-carrier complexes in full human serum,” Journal of Controlled Release, vol. 126, no. 1, pp. 67–76, 2008.
View at: Publisher Site | Google Scholar
J. Haupenthal, C. Baehr, S. Kiermayer, S. Zeuzem, and A. Piiper, “Inhibition of RNAse A family enzymes prevents degradation and loss of silencing activity of siRNAs in serum,” Biochemical Pharmacology, vol. 71, no. 5, pp. 702–710, 2006.
View at: Publisher Site | Google Scholar
S. Rodrigues, A. M. R. da Costa, and A. Grenha, “Chitosan/carrageenan nanoparticles: effect of cross-linking with tripolyphosphate and charge ratios,” Carbohydrate Polymers, vol. 89, no. 1, pp. 282–289, 2012.
View at: Publisher Site | Google Scholar
K. S. Soppimath, T. M. Aminabhavi, A. R. Kulkarni, and W. E. Rudzinski, “Biodegradable polymeric nanoparticles as drug delivery devices,” Journal of Controlled Release, vol. 70, no. 1-2, pp. 1–20, 2001.
View at: Publisher Site | Google Scholar
W.-J. Yi, J. Yang, C. Li et al., “Enhanced nuclear import and transfection efficiency of TAT peptide-based gene delivery systems modified by additional nuclear localization signals,” Bioconjugate Chemistry, vol. 23, no. 1, pp. 125–134, 2012.
View at: Publisher Site | Google Scholar
R. P. Hickerson, A. V. Vlassov, Q. Wang et al., “Stability study of unmodified siRNA and relevance to clinical use,” Oligonucleotides, vol. 18, no. 4, pp. 345–354, 2008.
View at: Publisher Site | Google Scholar
Y. Xu, Z. Wen, and Z. Xu, “Chitosan nanoparticles inhibit the growth of human hepatocellular carcinoma xenografts through an antiangiogenic mechanism,” Anticancer Research, vol. 29, no. 12, pp. 5103–5109, 2009.
View at: Google Scholar
K. J. Kim, B. Li, J. Winer et al., “Inhibition of vascular endothelial growth factor-induced angiogenesis suppresses tumour growth in vivo,” Nature, vol. 362, no. 6423, pp. 841–844, 1993.
View at: Publisher Site | Google Scholar
R. Savić, L. Luo, A. Eisenberg, and D. Maysinger, “Micellar nanocontainers distribute to defined cytoplasmic organelles,” Science, vol. 300, no. 5619, pp. 615–618, 2003.
View at: Publisher Site | Google Scholar
J. M. Kelm, N. E. Timmins, C. J. Brown, M. Fussenegger, and L. K. Nielsen, “Method for generation of homogeneous multicellular tumor spheroids applicable to a wide variety of cell types,” Biotechnology and Bioengineering, vol. 83, no. 2, pp. 173–180, 2003.
View at: Publisher Site | Google Scholar

Copyright

Copyright © 2016 Maria Abdul Ghafoor Raja 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.

PDF Download Citation

Download other formats

Order printed copies

Views

1224

Downloads

1027

Citations