In Vitro Intestinal Uptake And Permeability Of Fluorescently-Labelled Hyaluronic Acid Nanogels
Received 23 July 2019
Accepted for publication 4 October 2019
Published 21 November 2019 Volume 2019:14 Pages 9077—9088
Checked for plagiarism Yes
Review by Single anonymous peer review
Peer reviewer comments 2
Editor who approved publication: Prof. Dr. Thomas J. Webster
Miguel Xavier,1 Lorena García-Hevia,1 Isabel R Amado,1,2 Lorenzo Pastrana,1 Catarina Gonçalves1
1Department of Life Sciences, International Iberian Nanotechnology Laboratory, Braga 4715-330, Portugal; 2Department of Food and Analytical Chemistry, Faculty of Sciences, University of Vigo, Ourense 32004, Spain
Correspondence: Catarina Gonçalves
Department of Life Sciences, International Iberian Nanotechnology Laboratory, Av. Mestre José Veiga s/n, Braga 4715-330, Portugal
Email [email protected]
Background: Oral administration remains the most common mode of drug delivery. However, orally administered bioactive compounds must first survive digestion and then be absorbed at the intestine in order to reach other tissues or organs. The efficiency of both processes can be improved by encapsulation or conjugation with polymeric nanoparticles. Here we report the synthesis of amphiphilic hyaluronic acid (HyA) nanogels as nanocarriers for drug delivery.
Methods: HyA nanogels were prepared by self-assembly from amphiphilic HyA conjugates produced by grafting hydrophobic alkyl chains to the HyA backbone. The dye Cy5.5 was covalently bonded and used for tracking. The nanogels were characterised according to their structure, size and zeta potential, as well as biocompatibility towards an intestinal epithelial cell line. The uptake and intestinal permeability of the nanogels were assessed using in vitro models, which physiological relevance was verified regarding the morphology of the epithelium, the production of mucus, the expression of occludin and the transepithelial electrical resistance.
Results: The covalent binding of Cy5.5 did not affect significantly the size and surface charge of the nanogels at 125.1 ± 3.2 nm and −57.6 ± 6.2 mV respectively after labelling. Studies of biocompatibility showed that the nanogels were non-toxic to Caco-2 cells up to the concentration of 0.1 mg∙mL−1. The presence of mucus affected the nanogel uptake and highlighted the importance of considering mucus-producing cells in in vitro intestinal models. The uptake or adsorption to a Caco-2/HT29-MTX co-culture (8.1%) was higher than with single Caco-2 cell cultures (4.3%). Interestingly, both models led to minute (<0.5%) permeation of the nanogels across the intestinal barrier.
Conclusion: The HyA nanogels demonstrated to be mucoadhesive and effectively uptaken by intestinal cells. Both are determinant features for sustained release, but if systemic delivery is envisaged further modification with targeting moieties could be important to improve the nanogel permeability.
Keywords: oral delivery, in vitro models, nanogels, intestinal permeability, cellular uptake
Oral administration remains the preferred route for drug delivery owing to its low invasiveness, high efficiency and increased patient compliance.1 However, digestion through the gastro-intestinal tract and absorption in the small intestine constitute two obstacles that limit respectively the bioaccessibility and bioavailability of orally administered compounds.2 Thus, the development of smart carrier materials that are capable of resisting digestion and deliver their cargo through the intestinal epithelium is key to the success of newly developed drugs or food supplements. Equally important is the reliability of in vitro models to predict absorption at the intestine. These models not only allow the reduction of the use of animal models in in vivo studies, in line with the 3Rs principles of replacement, reduction and refinement, but also allow the use of human cells, thus reducing interspecies variability and potentially increasing the likelihood of new drugs to reach the market.1,3
In vitro models of the intestinal epithelium have existed for around 30 years.4 The gastro-intestinal epithelium consists of a layer of epithelial cells, which include but are not limited to, enterocytes, goblet cells, intraepithelial lymphocytes and dendritic cells.5,6 From these, the most abundant are enterocytes, which main function is the absorption of nutrients. Caco-2 are human colorectal adenocarcinoma epithelial cells. When reaching confluency, Caco-2 differentiate spontaneously to form a cell monolayer with an apical brush border and properties typical of absorptive enterocytes found in the small intestine.7 Cultivation of Caco-2 cells on filter supports further improves their morphological and functional differentiation and Caco-2 have been found to form a polarised epithelium with characteristic microvilli, closely sealed by tight junctions (TJs) and which expresses typical metabolic enzymes and membrane uptake/efflux transporters.1,2,7–9 Interestingly, Caco-2 monolayers are less permeable via the paracellular pathway when compared to the in vivo epithelium.2,10,11 Caco-2 cells also do not produce mucus, resulting in an enhanced transport of small molecules which diffuse more easily in the absence a mucous barrier. To better approximate the physiology of the intestinal mucosa, co-culture of Caco-2 cells with additional cell types, such as goblet cells, has become common practice in academia.12–16
Polymeric nanogels have been the target of extensive research as nanocarriers for bioactive compounds, offering prolonged blood circulation times and enhancing drug solubility.17–19 Hyaluronic acid (HyA) is a natural, hydrophilic glycosaminoglycan, which has been used for its biocompatibility, mucoadhesive properties, specificity to certain cellular receptors and, the presence of reactive groups that allow for functional chemical modifications.17–23 The conjugation of biopolymers with fluorescent probes is useful for tracking in both in vitro and in vivo biological studies. However, the incorporation of dyes in nanostructures must be stable in order to prevent leakage, which could lead to misinterpretation in studies on biodistribution or cellular uptake.24 In addition, the use of fluorophores may also alter relevant properties of the nanogels, such as their size or surface charge, potentially affecting their capacity to work as nanocarriers.25
In this work, the synthesis of fluorescently-labelled HyA nanogels for oral delivery of bioactive compounds is reported. The nanogels were prepared by self-assembly from amphiphilic HyA conjugates produced by grafting hydrophobic alkyl chains to the HyA backbone. The dye Cy5.5 was used as a reporter to quantify the cellular uptake of the nanogels and their permeation through the intestinal epithelium. The nanogels were characterised according to their structure, size and zeta potential, as well as biocompatibility towards an intestinal epithelial cell line. The uptake and permeation of the nanogels were tested using cell-based in vitro models, which included Caco-2, HT-29, HT29-MTX and co-culture combinations thereof to mimic the intestinal epithelium. The 5 culture conditions were characterised in terms of the topography of the cell layers, the expression of tight junction proteins and the integrity of the epithelial barrier. In addition, HT29-MTX, as mucin-secreting mature goblet cells,12,16,26,27 also allowed to study the mucoadhesion of the HyA nanogels.
Materials And Methods
Low molecular weight (4.8 kDa) hyaluronic acid (HyA) was purchased from Lifecore Biomedical (Chaska, MN, USA). Cy®5.5 hydrazide was obtained from GE Healthcare (Chicago, IL, USA). AG 50W-X8 resin was obtained from Bio-Rad (Hercules, CA, USA). Methanol was obtained from Honeywell Riedel-de-Haën™ (Seezel, Germany) and acetic acid from Fisher Scientific (Hampton, NH, USA). Minimum essential media (MEM) and 4ʹ, 6-diamidino-2-phenylindole, dilactate (DAPI, Invitrogen™) were purchased from Thermo Fisher Scientific (Waltham, MA, USA). 8-well chamber µ-slides were acquired from Ibidi GmbH (Gräfelfing, Germany). Trypsin-EDTA (0.25% trypsin; 0.1% EDTA), penicillin/streptomycin 100x, foetal bovine serum (FBS), Hank’s balanced salt solution (HBSS), non-essential amino-acids (NEAA), 1-µm pore size transwell® inserts and Amicon® Ultra-15 centrifugal filters were bought from Merck Millipore (Burlington, MA, USA). Chloroform, N-(3-Dimethylaminopropyl)-N′-ethylcarbodiimide (EDC), N-hydroxysuccinimide (NHS), Triethylamine (TEA), tetrabutylammonium fluoride (TBA-F), deuterium oxide (D2O), hexadecylamine (C16), sodium chloride (NaCl), dimethyl sulfoxide (DMSO), paraformaldehyde (PFA), 1% alcian blue solution in 3% acetic acid (alcian blue 8XG), Triton™ X-100, phalloidin-tetramethylrhodamine B isothiocyanate (phalloidin-TRITC), bovine serum albumin (BSA), fluoroshield™, L-glutamine solution 200 mM, sodium pyruvate solution 100 mM, resazurin sodium salt, and Dulbecco’s modified Eagle’s Medium-high glucose (DMEM) were obtained from Sigma-Aldrich (St. Louis, MO, USA).
Chemical Modifications Of Hyaluronic Acid (HyA)
Synthesis Of Amphiphilic Hyaluronic Acid Conjugate (C16-HyA)
The synthesis of amphiphilic HyA conjugates was adapted from previous methods.17 Briefly, HyA sodium salt was solubilised in DMSO following Na+ ion exchange by tetrabutylammonium (TBA) using a cation exchange resin (Figure 1A). EDC (155 mg) and NHS (93 mg) were added to the HyA-TBA solution in DMSO (500 mg; 1% w/v) followed by the addition of a solution of C16 (58 mg) in DMSO and 51 µL of TEA (Figure 1B). The mixture reacted under stirring for 24h at 50 °C, and the resulting solution was dialysed (3.5 kDa MWCO) against 150 mM NaCl for 3 days followed by diH2O for 2 days. The samples were dispersed in D2O at 10 mg∙mL−1 and the degree of substitution (DS) of C16 molecules in the HyA was determined by 1H NMR using a Varian Unity Plus 300 spectrometer operating at 299.94 MHz and 25 °C. The DS was obtained following Equation 1, where A and B are the integral values corresponding to the protons of the CH3 group of the alkyl chain (δ = 0.8–1.0 ppm) and the signal from the disaccharide protons (δ = 3.51–4.61 ppm) respectively.
Cy5.5-Labelling Of C16-HyA
Cy5.5 hydrazide (1 mg∙mL−1 in PBS) was added to a dispersion of C16-HyA (40 mg in 14 mL PBS) at a molar ratio of 1.6% over the free carbonyl groups of the HyA (after subtracting those used in the grafting of the C16 chains). The mixture was stirred overnight at 50 °C to promote the formation of stable amide bonds from the reaction of the hydrazide esters with the HyA carbonyl groups (Figure 1C). The resulting solution was dialysed (12–14 kDa MWCO) against PBS and diH2O, and purified using 10 kDa MWCO Amicon Ultra-15 centrifugal filters, until free Cy5.5 could not be detected in the eluate by fluorescence spectroscopy (λex=650 nm, λem=675-800 nm) measured using a BioTeK® Synergy H1 (Winnoski, VT, USA) multi-plate reader. The yield after filtration through the 10 kDa Amicon filters was estimated at 87% according to the fluorescence readings. The effective DS of Cy5.5 in the C16-HyA-Cy5.5 conjugate was not quantified as this was not relevant for this study, where Cy5.5 was used just for tracking.
Synthesis And Characterisation Of HyA Nanogels
Synthesis Of HyA Nanogels
Nanogels were obtained by dispersion of C16-HyA or C16-HyA-Cy5.5 in milli-Q diH2O at 0.5 mg∙mL−1 under stirring at 50 °C, followed by 2 sonication cycles (37 kHz; 104 W) for 15 min and filtration through a 0.45 µm PVDF syringe filter (Millex, Millipore). The stability of the nanogel dispersions was monitored by measuring the average size and polydispersity index (PdI) for up to 48 days.
Size And Zeta Potential
The hydrodynamic diameter (size) and surface charge (zeta potential) of the HyA nanogels were measured by dynamic light scattering (DLS) using a SZ-100 nanoparticle analyser (Horiba Scientific, Kyoto, Japan). Nanogels dispersed at 1 mg∙mL−1 were measured at 25 °C using a He-Ne laser (633 nm) and a detector angle of 173°. Polystyrene cells and folded capillary cells were used for size and zeta potential measurements respectively. Data are expressed as mean ± SD from 6 independent measurements.
All cells were maintained in media with 100 U·mL−1 penicillin and 100 μg·mL−1 streptomycin (1% Pen/Strep), in a humidified chamber at 37 °C and 5% CO2. The culture media was replenished every 2–3 days and the cells were routinely sub-cultured assuring a maximum confluence of 70–80%. To detach adherent cells, trypsin-EDTA was used for 5–10 min.
Caco-2 cells, clone HTB-37™, from human colon carcinoma (passages 25–40), were obtained from the American Type Culture Collection (ATCC®) and cultured in minimum essential media (MEM) supplemented with 20% FBS, 1% non-essential amino-acids (NEAA) and 1 mM sodium pyruvate.
HT-29 cells (passages 20–25), originally obtained from the American Type Culture Collection (ATCC®), were grown in DMEM supplemented with 10% FBS and 1 mM sodium pyruvate.
Mucus-secreting HT29-MTX-E12 cells (passages 60–65), were obtained from the European collection of Authenticated Cell cultures (ECACC) and cultured in DMEM, supplemented with 2mM L-glutamine, 10% foetal calf serum (FCS) and 1% NEAA.
In Vitro Cytotoxicity Assay
The cytotoxicity of the HyA nanogels was determined indirectly by the resazurin reduction assay. Caco-2 cells were plated in 96-well plates at 3×104 cells∙cm−1. After 24h, the media was removed and replenished with fresh media supplemented with 10 µg∙mL−1 resazurin sodium salt. HyA nanogels dispersed in PBS 1x were added (10% of total volume) to yield the final concentrations of 0.01, 0.05 and 0.1 mg∙mL−1. PBS (10% v/v) and DMSO (40% v/v) were used as negative and positive controls, respectively. The cells were incubated for 24h and 48h and the cell metabolic activity was determined by measuring the fluorescence of resofurin (λex=560 nm, λem=590 nm). The results are expressed as a percentage in relation to the negative control.
In Vitro Intestinal Epithelium Models
To evaluate the capacity to mimic the intestinal epithelium, monocultures of Caco-2, HT-29 and HT29-MTX, as well as co-cultures of Caco-2/HT-29 and Caco-2/HT29-MTX were used. For the co-cultures, the ratio of Caco-2 over HT-29 or HT29-MTX was 9:1 and the media used was MEM supplemented with 20% FBS, 1% non-essential amino-acids (NEAA) and 1 mM sodium pyruvate. To assess the production of mucus, the expression of the tight junction protein occludin, the uptake of the HyA nanogels and, the topography and polarization of the cell layers, cells were plated in 8-well µ-slides at a seeding density of 4.4×104 cells∙cm−2 and grown for 21 days. To determine the integrity of the epithelial barrier and its permeability to the HyA nanogels, Caco-2 or Caco-2/HT29-MTX co-cultures were seeded at 1×105 cells∙cm−2 and grown for 21 days on the apical chamber of 1-µm pore size transwell® inserts.
Alcian Blue Staining
Cultures were washed with PBS and fixed in cold methacarn (60% methanol, 30% chloroform, 10% acetic acid) for 15 min at 4 °C to preserve the mucus layer.14 Cells were then washed in a 3% acetic acid solution in H2O, stained with alcian blue 8XG for 15 min at RT, washed with water and imaged using an optical microscope.
To evaluate the topography and polarization of the cells and the expression of the tight junction protein occludin, cells were fixed in 4% (w/v) paraformaldehyde for 20 min and permeabilised by incubation with a 0.2% (v/v) Triton X-100 solution in PBS for 10 min. The fixed cultures were then incubated in a 2% (w/v) BSA solution in PBS to minimise non-specific antibody bonding. After blocking, cells were incubated with 5 µg∙mL−1 Alexa Fluor® 488-conjugated occludin monoclonal antibody (OC-3F10) for 1h followed by incubation with phalloidin-TRITC for 1h. Finally, cells were washed extensively, counter-stained with DAPI (0.2 µg∙mL−1) for 10 min and preserved in Fluoroshield mounting medium. The stained cell layers were imaged using a Zeiss LSM780 confocal laser scanning microscope (Oberkochen, Germany) and analysed using Zen 2010 software and ImageJ.
Cellular Uptake Of The HyA-Cy5.5 Nanogels
To assess the uptake of the HyA nanogels, Caco-2 and Caco-2/HT29-MTX co-cultures were incubated for 18h with a dispersion of HyA-Cy5.5 nanogels in complete culture media. Following incubation, the cells were extensively washed, and the actin filaments stained using phalloidin-TRITC and imaged as detailed in 2.6.2.
Trans-Epithelial Electrical Resistance (TEER) Measurement
The TEER was measured to assess barrier integrity, following a protocol for static epithelial models.28 The cell-culture inserts were allowed to equilibrate to RT for 10 min and the TEER was measured using a Millicell® ERS-2 volt-ohm-meter (Merck Millipore, Billerica, MA, USA) with STX chopstick electrodes. TEER values in Ω∙cm2 were calculated by subtracting the TEER of cell-free transwells® from the cell-cultured transwell inserts, and multiplying by the surface area of the well.
Transport Across The Intestinal Epithelium
To evaluate the capacity of the HyA-Cy5.5 nanogels to cross the intestinal epithelium, Caco-2 monocultures and co-cultures of Caco-2/HT29-MTX grown on transwell® inserts were distributed evenly, based on TEER, into 12-well plates pre-filled with 1.5 mL of warm HBSS. HyA-Cy5.5 nanogels in HBSS were added to the apical chamber and the cells were incubated in a humidified chamber at 37 °C for 1 h under agitation (100 rpm). At pre-determined time-points (1, 2, 3 and 4h), 200 µL were collected from the basolateral chamber and replenished with fresh HBSS. At the 4h time-point, the samples from the apical chamber were collected and pooled for analysis. The cells were washed and incubated for 30 min in warm HBSS before measurement of the TEER to validate the integrity of the barrier. Finally, the cells were lysed with a 1% triton X-100 solution in HBSS, spun down and the supernatant collected for analysis. The HyA-Cy5.5 nanogels fluorescence was quantified by fluorescence spectroscopy (λex=650 nm, λem=690 nm).
Results are displayed as Mean ± SD unless otherwise stated. The statistical significance was tested using the Student’s t-test for independent samples or a two-way ANOVA with Tukey’s post-hoc test using GraphPad Prism 8.2.1 (San Diego, CA, USA).
Results And Discussion
Synthesis And Characterisation Of HyA Nanogels
Amphiphilic hyaluronic acid conjugates were synthesised by grafting 16-carbon alkyl chains to the HyA backbone. The reaction was confirmed by 1H NMR (ESI Figure 1) and the degree of substitution calculated showing a ratio of 16 alkyl chains grafted per every 100 disaccharide units (16%). C16-HyA was fluorescently labelled with Cy5.5 by the formation of stable amide bonds after reaction with Cy5.5 hydrazide in diH2O. Figure 2A shows the fluorescence spectra of the C16-HyA-Cy5.5 before and after filtration through the 10 kDa MWCO Amicon Ultra-15 centrifugal filters, as well as of the filtrate. For sterility, C16-HyA-Cy5.5 was further filtered through a 0.45-µm PVDF syringe filter, which did not alter the fluorescence intensity (ESI Figure 2).
C16-HyA and C16-HyA-Cy5.5 nanogels were formed by self-assembly in water. To assess whether grafting of the Cy5.5 fluorophore affected the properties of the nanogels, both formulations were tested for their size, polydispersity index (PdI) and zeta potential by dynamic light scattering (DLS). As could be anticipated, both formulations showed high negative zeta potential (−66.4 ± 1.4 mV and −57.6 ± 6.2 mV for C16-HyA and C16-HyA-Cy5.5, respectively) due to the presence of ionisable carboxylic groups in the HyA backbone. High zeta potential values (positive or negative), are indicative of a predominance of repulsive over attractive electrostatic forces, leading to stable colloidal dispersions. In contrast, low zeta potential values are typically linked to aggregation or flocculation, though stable dispersions can also be achieved with low or neutral zeta potential.29–31 The decrease in the zeta potential of the C16-HyA-Cy5.5 nanogels is likely due to a reduction of free carbonyl groups, used for the formation of amide bonds after reaction with the Cy5.5 hydrazide. Though statistically significant (p<0.01, Student’s t-test), the difference of 8.8 mV, should not affect the stability of the nanogels dispersion since the surface charge remains highly negative. In addition, negatively charged particles have been linked to higher uptake and lower toxicity when compared to positively charged particles.32
The average size of the C16-HyA and C16-HyA-Cy5.5 nanogels was 140.1 ± 3.6 nm and 125.1 ± 3.2 nm respectively. Interestingly, the modification with Cy5.5 led to a reduction in the average particle size. The achieved particle size is favourable within the context of drug delivery as nanoparticles of sizes around 100 nm have been shown to outperform other particle sizes ranging from 50 to 1,000 nm in terms of uptake by Caco-2 cells.33
The stability of the C16-HyA and C16-HyA-Cy5.5 nanogels was evaluated by measuring the average particle size and PdI after storage for 48 days at 4 °C. A minor decrease in the particle size of C16-HyA nanogels could be observed (Figure 2B) but despite the statistical significance (p<0.05, Student’s t-test), owing to small standard deviations, this was just in the order of 3% and should be disregarded. The size of the C16-HyA-Cy5.5 remained unchanged and thus it can be concluded that both nanogel formulations remained stable for the period of 48 days.
Finally, given the nanogels were designed to be delivered orally, the stability of the nanogels was assessed at pH 5.0 and 3.0 (representative of digestion conditions) for up to 6 days (ESI Figure 3). The dispersion of the nanogels at pH 3 led to a slight increase in the average size of the nanogels to 160.9 ± 5.1 nm. Nevertheless, both size and PdI of the nanogels remained stable at both pH for up to 6 days when stored at room temperature. There was again a minor decrease in the particle size of the C16-HyA nanogels at pH 3 over time, which was statistically significant (p<0.05), but should have no effect on the functionality of the nanogels. This showed that the C16-HyA nanogels remain stable at the range of pH found in the gastrointestinal tract during digestion.
Biocompatibility Of The C16-HyA Nanogels
The biocompatibility of the C16-HyA nanogels was assessed as a function of their concentration (0.01; 0.05 and 0.1 mg∙mL−1) after incubation with Caco-2 cells for 24 and 48h. The cell viability was determined indirectly by assessing cell metabolic activity using the resazurin reduction assay. Figure 3 shows that the viability of the Caco-2 cells was significantly reduced (p<0.001) after incubation with DMSO (positive control). In contrast, irrespective of incubation time, incubation with the C16-HyA nanogels did not produce any effect in the metabolic activity of Caco-2 cells for the range of concentrations tested. These results show that the C16-HyA nanogels are non-toxic to Caco-2 cells up to the concentration of 0.1 mg∙mL−1.
Uptake And Transport Of C16-HyA-Cy5.5 Nanogels Using In Vitro Models Of The Intestinal Epithelium
Prior to the uptake and transport studies, Caco-2, HT-29 and HT29-MTX cell lines, and co-culture combinations thereof, were evaluated for their capacity to replicate a functional intestinal epithelium. Accordingly, mucus secretion, the morphology of the epithelium, tight-junction protein expression and the barrier integrity were evaluated.
The capacity to secrete mucus is fundamental to the establishment of a physiologically relevant in vitro intestinal model. Indeed, the presence of a mucus layer is considered the first level of defence against the entry of pathogens through the gastrointestinal tract.34 From a drug delivery perspective, mucus acts as an additional barrier limiting diffusion35 but also potentially increasing the residence time of mucoadhesive carriers.36–40 This evidences the importance of addressing this fundamental parameter in the development of carriers for sustained release.
Single cultures of Caco-2, HT-29 and HT29-MTX, as well as co-cultures of Caco-2/HT-29 and Caco-2/HT29-MTX were grown for 21 days and the production of mucus assessed by staining using alcian blue. Figure 4 shows that, as anticipated, Caco-2, HT-29 and the Caco-2/HT-29 co-culture were negative for the alcian blue staining and thus do not produce mucus. In opposition, both HT29-MTX and the co-culture of Caco-2 with HT29-MTX showed extensive mucus production. Interestingly, while the presence of mucus on the HT29-MTX cultures was dispersed over the cell layer, on the Caco-2/HT29-MTX co-culture, the mucus was concentrated in patches (Figure 4, black arrows), likely related to the 9:1 seeding ratio of the two cell lines.
Morphology And Formation Of Tight Junctions
The morphology of the cell layers was assessed following 21 days of culture by staining F-actin using rhodamine-labelled phalloidin. Figure 5 shows staggering differences between the 5 cultures conditions tested. The most significant difference was the thickness of the cell layers which rounded 10 µm for the Caco-2 and Caco-2/HT-29 co-culture but was at least twice as thick for the monocultures of both goblet cell types (more columnar), as well as for the co-culture of Caco-2/HT29-MTX. In addition, while the distribution of F-actin (green) appears to be fairly homogeneous for the monocultures of Caco-2 and HT29 and the co-culture of these, it appears more concentrated in the apical side for the HT29-MTX and the co-culture of Caco-2/HT29-MTX, suggesting that this co-culture conditions lead to the formation of a polarised epithelium, with apical microvilli forming brush borders.41 Given that HT-29 and HT29-MTX are distinguished by the capacity of the latter to produce mucus, this suggests that the presence of mucus is important to lead to cell polarisation and achieve a physiologically relevant predictive model. It was also interesting to perceive that the Caco-2/HT29-MTX co-culture recreates undulating human intestinal villi with areas of higher thickness interspersed with areas of lower thickness.42 This phenomenon is further verified by the images in Figure 6. Here, in addition to F-actin (red), the tight-junction specific protein occludin (green) was labelled to assess the formation of a tight intestinal epithelial barrier. Though not quantitative, it is apparent that the expression of occludin is more marked on the Caco-2 monoculture when compared to the Caco-2/HT29-MTX co-culture. Note that the exposure time and power of the lasers were kept constant for the acquisition of both images. These results are in keeping with previous observations that Caco-2 monolayers show very low permeability but that the co-culture with additional cell types has the capacity to better approximate the physiology of the in vivo scenario.2
Figure 5 Laser scanning confocal microscopy images of F-actin (green) and nuclei (DAPI, blue) of Caco-2, HT-29 and HT29-MTX monocultures and co-cultures of Caco-2/HT-29 and Caco-2/HT29-MTX.
Cellular Uptake And Intestinal Permeability
To assess the uptake of the C16-HyA-Cy5.5 nanogels, single cultures of Caco-2 and HT29-MTX, and Caco-2/HT29-MTX co-cultures were incubated with a C16-HyA-Cy5.5 nanogel solution for 18 hrs and observed by laser scanning confocal microscopy. Figure 7 shows images of a representative slice and orthogonal views of the 3 culture conditions. The orthogonal views showed that the C16-HyA-Cy5.5 nanogels were not internalised in the single cultures of HT29-MTX. This was likely due to the presence of a homogeneous mucus layer and suggests mucoadhesive properties of the HyA nanogels which remained adsorbed after several washes. In contrast, the nanogels were uptaken by both the Caco-2 monoculture and the Caco-2/HT29-MTX co-culture where they appear disperse in the cytoplasm (Figure 7, bottom). Between these two culture conditions, the uptake seemed higher for the single culture of Caco-2 but it was difficult to discern from this study alone.
Studies of the intestinal permeability allowed to quantify the cellular uptake of the single cultures of Caco-2 and the Caco-2/HT29-MTX co-cultures. Here, cells were cultured on 1-µm pore size Transwell® inserts for 21 days. At day 21, the cultures were incubated with the C16-HyA-Cy5.5 nanogels in HBSS for 4 hrs and the amount of nanogels that were uptaken and/or permeated through the intestinal barrier was quantified by fluorescence. As a control, the amount of nanogels that remained in the apical chamber after the 4-h incubation was also determined (92.3% and 89.8% for the Caco-2 and the Caco-2/HT29-MTX cultures, respectively). During the 21 days of culture, the TEER was monitored to assess the barrier integrity. From the day of the first measurement (Day 5), the TEER of the single cultures of Caco-2 was significantly higher (p<0.001) than the Caco-2/HT29-MTX co-cultures (Figure 8A). This trend was maintained during the 21 days of culture, which is in line with previous studies of co-cultures of Caco-2/HT29-MTX,13,14,16 and supports the statement that co-cultures increase the permeability of Caco-2 approximating it to more physiological levels.2,12 Although not statistically significant, the amount of C16-HyA-Cy5.5 nanogels that were found either uptaken by the cells or adsorbed to the cellular layer was higher for the co-culture than for the single cultures of Caco-2 (8.1 ± 2.5% vs 4.3 ± 0.2%; Figure 8B). The amount of nanogels that effectively permeated the intestinal barrier was found to be lower than 0.5% of the initial added C16-HyA-Cy5.5 nanogel mass. Though this is a statement toward the integrity of both in vitro models, it also suggests that if the nanogels carry a bioactive that is to be administered orally and reach the systemic circulation, some degree of modification should be added to promote active transport of the nanogels.
This work showed the synthesis of amphiphilic hyaluronic acid by grafting of 16-carbon alkyl chains (C16). The C16-hyaluronic acid was further labelled fluorescently with a Cy5.5 dye for tracking of the cellular uptake and intestinal permeability, with no significant effect on the size and surface charge of the nanogels, which remained stable for up to 48 days. In addition, the achieved particle size of 125.1 ± 3.2 nm is favourable within the context of drug delivery as nanoparticles of sizes around 100 nm have been shown to outperform other particle sizes ranging from 50 to 1,000 nm in terms of uptake by Caco-2 cells.
Studies of biocompatibility using the resazurin reduction assay showed that the nanogels were non-toxic to the Caco-2 cell line up to the concentration of 0.1 mg∙mL−1. The uptake and permeability of the nanogels were studied using in vitro intestinal models with verified production of mucus, expression of the tight-junction protein occludin and barrier integrity – monitored by the TEER. To evaluate the physiological relevance of the in vitro model, different single and co-culture conditions were studied using Caco-2, HT-29 and HT29-MTX cells. The presence of the mucus-producing HT29-MTX cells led to a thicker cell layer with columnar and polarized cells with actin concentrated in the apical side recreating the in vivo scenario. The uptake studies highlighted the importance of mucus in in vitro models mimicking the intestinal epithelium. 4.3% and 8.1% of the total mass of the added nanogels were uptaken by Caco-2 and the Caco-2/HT29-MTX co-culture respectively after 4 hrs, and less than 0.5% actually permeated the barrier to the basolateral side. The HyA nanogels were effectively uptaken and appear to be mucoadhesive remaining on the cell layer after several washes. If systemic delivery is envisaged, further modification with targeting moieties should be considered to improve the nanogel permeability. Regarding the in vitro models, based on these data, a microfluidic dynamic model is currently under development including simulated-peristaltic motion to understand the effect of continuous flow and mechanic stimulation on cell differentiation.
The authors would like to acknowledge Doctor Andreia Gomes from the University of Minho for providing the HT-29 cells. This work was funded by MICRODIGEST project (grant agreement 037716) co-funded by FCT and ERDF through COMPETE2020, the FODIAC project (grand agreement 778299) funded by the European Commission through H2020-MSCA-RISE-2017 and CVMar+I project (INTERREG V-A España – Portugal – POCTEP 2014–2020, Ref. 0302_CVMAR_I_1_P).
Isabel Amado received funding from the People Programme (Marie Curie Actions) of the European Union’s Seventh Framework Programme (FP7/2007-2013) under REA grant agreement no. 600391. The authors report no other conflicts of interest in this work.
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