Modeling neural differentiation on micropatterned substrates coated with neural matrix components.

Topographical and biochemical characteristics of the substrate are critical for neuronal differentiation including axonal outgrowth and regeneration of neural circuits in vivo. Contact stimuli and signaling molecules allow neurons to develop and stabilize synaptic contacts. Here we present the development, characterization and functional validation of a new polymeric support able to induce neuronal differentiation in both PC12 cell line and adult primary skin-derived precursor cells (SKPs) in vitro. By combining a photolithographic technique with use of neural extracellular matrix (ECM) as a substrate, a biocompatible and efficient microenvironment for neuronal differentiation was developed.

Introduction

The interface of biomaterials and stem cells may provide new strategies for reconnecting severed nerve pathways in the nervous system after injury (Dalton and Mey, 2009; Orive et al., 2009). The ability to recreate the cellular microenvironment is also important to understand cell behavior and functionality in vitro (Schenke-Layland et al., 2009). In vivo, the existence of an organized extracellular matrix (ECM) promotes cell adhesion, differentiation and proliferation and hence maintenance of tissue homeostasis. In the nervous system, axonal pathfinding and regeneration are mediated by individual and/or synergistic stimulatory and inhibitory cues (Li et al., 2008). In fact, substrate discontinuities generate an orientation in cell locomotion known as “contact guidance”, which is ubiquitously found in development, growth, and regeneration of nerves (Corey and Feldman, 2003). In contrast, random spatial distribution and overlap of neurites is often found in standard cell culture.

A promising approach in manipulating the cellular microenvironment is the use of micromanufacturing technologies such as microcontact printing or photolithography, because of comparable physical dimensions to cellular constructs (Hook et al., 2009). Among others, micropatterning has been recently applied to human neural progenitor cells grown on polystyrene coated with entactin, collagen, and laminin (Blong et al., 2010), to spiral ganglion neurons and Schwann cells patterned on methacrylate (Clarke et al., 2011), to dissociated dorsal root ganglion neurons seeded onto laminin- and fibronectin-spotted surfaces (Fereol et al., 2011), primary adult human neural stem cells (Beduer et al., 2012) and differentiated human SH-SY5Y neuron-like cells (Hardelauf et al., 2011) grown on polydimethylsiloxane (PDMS) membranes, hippocampal neurons grown on poly-D-lysine micron-wide lines patterned onto a poly(ethylene glycol) (PEG) monolayer (Wissner-Gross et al., 2011) and dissociated central nervous system neurons (Hellman et al., 2010; Takayama et al., 2011), embryonic stem cell-derived motor neurons (Shi et al., 2010), and primary cortical neurons (Kunze et al., 2011) seeded into diverse microfluidic cell culture settings.

Although cells may adhere to a variety of untreated polymeric surfaces, several synthetic polymers (e.g., PEG) do not permit cell attachment in the absence of coating. For in vitro neural differentiation, polylysine and polyornithine have been widely used as adhesive treatments for the substrate. However neural ECM is far more complex in terms of structure, organization, and different constituent parts in vivo. To improve in vitro neural differentiation, we mimicked neural ECM by using the following substrate: (1) a commercially available soluble basement membrane extract, purified from mouse sarcoma (Cultrex®) that contains laminin, collagen type IV, heparan sulphate, entactin, and growth factors (Kleinman, 2001; Arnaoutova et al., 2012); (2) hyaluronic acid (Turley et al., 2002), and (3) netrins, i.e., laminin-related neuropeptides involved in neurite outgrowth and axonal guidance (Rajasekharan and Kennedy, 2009; McCormick and Leipzig, 2012). Similar basement membrane-based substrates have recently been reported for in vitro neural engineering, specifically for Schwann cells (Dewitt et al., 2009) and embryonic stem cell-derived neural precursor cells (Uemura et al., 2010).

The presence of collagen, laminin, entactin, and certain proteoglycans in the basal composition of ECM provides the signal that cells need to be anchored to the substrate and start differentiation. In particular, hyaluronic acid is an anionic polysaccharide that forms electrostatic complexes with cationic molecules such as collagen or polylysine (Pan et al., 2009); hence collagen ionic adsorption alters the cell repulsion that is inherent to hyaluronic acid (Takahashi et al., 2009), allowing the incorporation of this molecule into the matrix (Wang and Spector, 2009). On the other hand, netrins act as cellular and neurite-chemoattractant factors, as it occurs in the developing neural tissue (O'Donnell et al., 2009). In addition to its composition, thickness of the matrix is also fundamental in cell differentiation as recently demonstrated (Leipzig and Shoichet, 2009).

To model in vitro differentiation, we used both PC12 cell line and primary skin-derived neural precursor cells. PC12 cells have been widely used in both neurobiological and neurotoxicological studies as an in vitro model for neuronal differentiation (Das et al., 2004). The cell line originated clonally from rat pheochromocytoma. In response to nerve growth factor (NGF), PC12 cells undergo a dramatic change of phenotype and acquire properties of sympathetic neurons. NGF-treated PC12 cells cease proliferation, extend neurites and become electrically excitable (Greene and Tischler, 1976). Importantly, these cells have already been shown to grow and differentiate in micropatterns of different kinds (Foley et al., 2005; Ferrari et al., 2010; Yang et al., 2011).

Starting up from a protocol to isolate and culture CNS stem cells (Reynolds and Weiss, 1992), Miller and colleagues isolated skin-derived precursor cells (SKPs) from the dermis (Toma et al., 2001). These precursor cells have the potential to generate progeny of the neuronal and glial lineages, amongst other cell types (Fernandes et al., 2008; Hunt et al., 2009). Importantly, dopaminergic neurons have been generated in vitro from SKPs and transplanted into the striata of a Parkinson disease (PD) rat model (Kubo et al., 2009; Higashida et al., 2010). Although these recent findings will need validation by independent research groups, they hint the potential to isolate autologous dermal precursor cells and, after in vitro differentiation to the desired lineage, apply the differentiated neurons for cell replacement therapies of Parkinson's disease.

In the current study, we hypothesized that combining the topography of a micropatterned substrate by photolithographic technique- with the signals of neural matrix components would supply the cells the appropriate environment and signal cues for neural differentiation. We chose PC12 cells as a widely used cell model to study the biocompatibility and neuronal differentiation potential of our experimental set up, and observed neurite outgrowth in the absence of added NGF. Finally, we confirmed the enhancement of neuronal differentiation with primary SKPs isolated from adult rat skin. Taking into account the aforementioned studies on derivation of dopaminergic neurons from SKPs, our work might add on the necessary strategies to improve differentiation of neuronal precursor cells into substantia nigra dopaminergic neurons (Gaillard and Jaber, 2011).

Materials and methods

Generation of micropatterned substrates using photolithography

A mask template was made with a pattern consisting of a repetition of squares and rectangles of 300 × 300 μm and 300 × 400 μm, respectively, situated between interconnected channels of 200 × 200 μm (Figures 1A,B). Micropatterned substrates were manufactured using standard photolithographic techniques. Glass coverslips (Menzel-Gläser, 24 × 24mm) were chemically etched with a 1:2 (v/v) solution of hydrofluoric acid (Panreac) for 5 min in order to improve the adhesion of the photoresist to glass. Briefly, SU-8 2,100 photoresist (MicroChem Inc.) was spin-coated in an EVG-101 machine onto etched coverslip surfaces (1 ml/coverslip). Spinning conditions of 4,000 rpm and 1,000 rpm/s for 60 s were used in order to uniformly coat the glass coverslips with a layer of photoresist (approximately 15 μm thick). Coverslips were pre-baked previous to the UV (365 nm) exposure, in an EVG-620 mask aligner for 20 s; and post-baked, developed and thoroughly cleaned in isopropyl alcohol (Sigma). Finally, coverslips were baked on a hot plate at 150°C for approximately 30 min in order to remove any traces of volatile chemicals still present in the layer of SU-8.

Figure 1

Surface patterning of coverslips using photolithographic technique and coating with neural ECM. (A–B) Cartoon depicting the upper and lateral views of the micropatterned substrate (A) and optical microscopy image after conclusion of the photolithographic process, when “peaks” (red arrows) and “valleys” (blue arrows) were formed (B). (C) Polymerization and penetration of the ECM into micropatterned substrates. Hyaluronic acid of low molecular weight (HLMW) allowed for dispersion of the matrix along the valleys of the patterned surface. A 1:3 dilution of the ECM with HLMW achieved the desired fibrous structure. Scale bars, 200 μm.

Neural-like extracellular matrix (ECM) deposition

Micropatterned coverslips were cleaned with distilled water, sterilized by exposition to UV light for 30 min and incubated with a solution of Cultrex® basement membrane extract (without phenol red, R&D), hyaluronan of low (31 kDa, HLMW) or high (980 kDa, HHMW) molecular weight (R&D), Netrin-G1a and Netrin-4 (R&D) in phosphate-buffered saline (PBS, Gibco). In order to polymerize and adsorb the matrix on the exposed glass surface they were kept for 24 h at 37°C in sterile conditions. Next, excess PBS was eliminated and coverslips left to dry up for 1 h under laminar flow and UV light. Prior to cell seeding, polymeric substrates were sterilized by exposition to UV light for 30 min in a tissue culture hood. Excess matrix deposited over the “peaks” was eliminated by incubation with culture medium for 24–48 h at 37°C.

Micro and nano-characterization of ECM

The ECM topography was characterized by Atomic Force Microscopy (AFM) by using a Digital Instruments Nanoscope® IIIA. Samples were fixed with Vitrosec® 70 (Panreac) for 20 min. Measurements were acquired in tapping mode using a silicon tip and the resonance frequency set at 300 KHz. Topography measurements were performed both in dry and wet conditions. AFM data were analyzed with Multimode® SPM. For Scanning Electron Microscopy (SEM), polymeric substrates with or without cells were fixed with Vitrosec® 70 for 20 min and stained with Coomassie brilliant blue R-250 staining solution (Bio-Rad) for 5 min at room temperature. Excess staining solution was removed with water. Samples were dried and mounted onto aluminium disks and coated with gold-argon. Imaging was performed on a JEOL JSM-5910-LV SEM using a 20 kV acceleration voltage. Samples were analyzed by an INCA-300 energy dispersed system (EDS) coupled to the microscope.

PC12 cell line maintenance and differentiation

Rat PC12 cells (CRL-1721, ATCC) were maintained in Ham's F12 medium modified by Kaighn (F12K, Gibco) and supplemented with 2.5% fetal bovine serum (ATCC), 15% horse serum (ATCC) and 1% penicillin/streptomycin (P/S, Sigma). The differentiation of PC12 cells on micropatterned substrates was carried out for 7 days in the same maintenance medium (without NGF) at a cell density of 2,500–120,000 cells/ml.

Isolation, labeling, and differentiation of adult rat SKPs

All experiments were carried out in accordance with the guidelines established by the National Council on Animal Care. SKPs were isolated from the dorsal skin of adult Wistar female rats modifying previously described protocols (Biernaskie et al., 2006). Five cm2 of rat dorsal skin were incubated for 30 min on ice in Hank's balanced salt solution (HBSS, Gibco), supplemented with 2% P/S and 2% Fungizone™ (Gibco). Skin was cut into 2 mm2 pieces and incubated in collagenase type IA solution (2 mg/ml; 650 CDU/mg, Sigma) for 3 h at 37°C under gentle shaking. Undigested skin was mechanically dissociated by vigorous pipetting. The resulting cell suspension was filtered through 40 μm nylon cell strainers (BD), centrifuged at 1,500 rpm for 5 min, and resuspended in Neurobasal™ A medium (Gibco) supplemented with 2% B27 Supplement (Gibco), 1% L-glutamine solution 200mM (Sigma), and 1% P/S. Every 2 days, the medium was supplemented with 20 ng/ml epidermal growth factor (EGF, R&D), 40 ng/ml fibroblast growth factor basic (FGF2, R&D) and 2% low serum growth supplement (LSGS, Gibco). Under these culture conditions, neurosphere-like structures [here dubbed “dermospheres” (Gago et al., 2009)] were formed within 48 h culture. Cells were gently resuspended in medium before plating onto the ECM substrate. The differentiation of SKPs (10 dermospheres/coverslip) was carried out in the same maintenance medium plus with 1% N2 Supplement (Gibco) and 10% fetal bovine serum (ATCC). Every 2 days, half medium was replaced and supplemented with 50 ng/ml nerve growth factor β (NGFβ, Sigma), 50 ng/ml brain-derived neurotrophic factor (BDNF, Sigma), 200 ng/ml Sonic hedgehog (SHH, R&D), and 200 ng/ml fibroblast growth factor 8b (FGF8b, R&D). For quantitative assessment of differentiation, at least ten different fields out of three independent experiments were quantified.

Morphometric analyses, immunofluorescence and confocal microscopy

For morphometric analyses of differentiated PC12 cells, digitized images of cells stained with May-Grünwald's eosin methylene blue solution (Merck) or with Bodian's silver proteinate (Sigma) were taken with a DSFi1 camera attached to an Eclipse TS100 microscope (Nikon). Images were analyzed with NIS-Elements F2.30 software (Nikon). Total neurons, neurites by neuron and apparently connected neurites by neuron were quantified on each condition. At least ten different fields out of three independent experiments were quantified. After 20 days in neuronal differentiation conditions, rat SKPs were washed with 1X PBS and fixed in 4% paraformaldehyde aqueous solution (Electron Microscopy Sciences) for 20 min at room temperature. Cells were washed in PBS, permeabilized for 1 h in 0.3% Triton® X-100 (Sigma) in PBS (PBS-T) and 5% normal donkey serum (Sigma). Cells were incubated with the appropriate primary antibody diluted in PBS-T for 2 h at room temperature. Primary antibodies used were anti-neurofilament light (NFL; used at 1:100 dilution; Cell Signaling Technology #2835), anti-tyrosine hydroxilase (TH; 1:1,000; Millipore #AB152), anti-Nestin (1:200; Millipore #MAB353), anti-βIII-tubulin (1:10, R&D #964673) and anti-α-smooth muscle actin (α-SMA; 1:500; Sigma #A2547). Next, cells were 1X PBS washed 3 times (5 min each) and incubated with the appropriate secondary antibody diluted in PBS-T for 1 h at room temperature. Secondary antibodies used were goat anti-mouse Alexa Fluor® 488 (Invitrogen; 1:1,000) and donkey anti-rabbit Alexa Fluor® 546 (1:1,000; Invitrogen). Prior to mounting in Mowiol® mounting medium (Fluka), cells were incubated with 10 μg/ml Hoechst 33258 (Sigma) for 5 min and washed with distilled water. Images were obtained by using a Zeiss LSM 510 microscope coupled to Zeiss Axion camera and analyzed by using Zeiss ZEN image analysis software (2008; SP1.1).

Statistical analyses

Data are expressed as means ± standard deviations of the number of independent experiments. One-Way ANOVA and Bonferroni post-test analyses were performed with GraphPad Prism 5.04 for Windows software.

Results

Development and characterization of neural ECM deposition on micropatterned substrates

In order to generate patterned in vitro neuronal differentiation conditions, micropatterns were reproducibly manufactured by photolithography on glass coverslips, as detailed in Materials and Methods. To create interconnected channels large enough to accommodate several aligned and interconnected neuronal cells, surface microgeometry was designed as hydrophobic “peaks” delineating 200 μm wide, interconnected “valleys” (Figures 1A,B).

To attain preferential deposition of neural ECM on the valleys and to generate a three-dimensional structure suitable for cell culture, several combinations of basal membrane and hyaluronic acid were assayed (not shown). Coomassie blue staining of matrix proteins showed that high molecular weight hyaluronic acid (HHMW; both diluted and undiluted) prevented proper polymerization of the matrix. In contrast, low molecular weight hyaluronic acid (HLMW) dispersed the matrix along the valleys of the patterned surface, originating an adequate and homogeneous fibrous structure only when ECM was diluted 1:3 (Figure 1C). Thus, a 1:3 dilution of soluble basal membrane extract mixed with HLMW was chosen for proper polymerization of the matrix, showing both cell penetrating capacity throughout the patterned substrate and the desired fibrous structure for cell growth.

Micro- and nanostructural morphology of the matrix on the patterned substrates was then characterized by SEM and AFM, respectively (Figure 2A). Deposited proteins were stained with Coomassie blue (Figure 2B) and coated with a thin layer of evaporated gold to allow correct display of the matrix structure by SEM (Figure 2C). As shown in Figures 2D–G, the matrix presented a homogeneous fibrous network structure in which pores of different sizes were seen. To characterize the matrix at the nanometric scale, patterned substrates were analyzed by AFM (Figures 2H,I). An average surface roughness (Rms) of 125.91 nm was found in dry conditions. When the samples were hydrated by incubation in distilled water, average surface roughness (Rms) increased to 235.63 nm, possibly due to the hydration capacity conferred to ECM by hyaluronic acid.

Figure 2

Micro- and nanocharacterization of the neural ECM. (A–C) Before mounting, samples (A) were stained with Coomassie blue (B) and then coated by a thin gold layer (C). (D-G) Matrix characterization by scanning electron microscopy (SEM). At a lower magnification (D, 500×, scale bar 50 μm), a homogeneous coating of valleys in the patterned substrate may be appreciated. At higher magnifications (E, 1,000×, scale bar 10 μm; F, 5,000×, scale bar 5 μm; G, 20,000×, scale bar 1 μm), a fibrous structure with pores of different sizes is evident. (H,I) Atomic force microscopy (AFM) analyses under both dry (H) and wet (I) conditions showed that the matrix volume increased with hydration, as expected. Darker areas correspond to lower protein density areas, while lighter areas correspond to higher protein density areas.

Differentiation of PC12 cells in the absence of NGF generates tyrosine hydroxilase (TH)-positive neurons

To ascertain the effect of the substrate on neuronal differentiation and neurite outgrowth, PC12 cells were cultured in the absence of the differentiation-inducing factor NGF, which was purposedly excluded to isolate the effect of the matrix on PC12 differentiation from other external clues.

Micropatterned coverslips prepared in the absence of neural ECM produced disorganized cell networks that localized over both peaks and valleys (Appendix, Figure A1A). A similar effect was observed with ECM in the absence of micropatterning (Figure A1B). Only the presence of both ECM and surface microgeometry directed PC12 cells to ECM deposits on valleys, where they apparently formed proper neurons (Figure A1C).

Figure A1

Effects of micropatterned substrate and neural ECM on PC12 cell differentiation in the absence of NGF. PC12 cells were stained with May Grunwald's eosin methylene blue solution modified for microscope staining after 7 day-differentiation in vitro. (A) Cells differentiated in the presence of micropatterned substrate only. (B) Cells differentiated in the presence of ECM only. (C) Cells differentiated in the presence of both micropatterned substrate and ECM.

To determine the appropriate cell density to achieve an optimal cellular differentiation, different concentrations of PC12 cells were seeded and, after 10 days in vitro, analyzed by silver proteinate staining for detailed observation of the neuritic extensions (Figure 3A). A density range of 40–80 thousand cells/ml was suitable for cell differentiation in these conditions. Morphometric analyses showed that, although maximum neuron numbers were obtained at a density of 80,000 cells/ml (Figure 3B), improved differentiation as shown by the average number of total neurites per neuron (Figure 3C) as well as by their interaction (Figure 3D), peaked at 40,000 cells/ml. For these reasons, a cell seeding density of 40,000 cells/ml was established.

Figure 3

Quantification of neuronal differentiation of PC12 cells on micropatterned substrates. (A) PC12 cells were differentiated for 10 days and stained by Bodian's silver proteinate. Scale bar, 50 μm. (B) Quantification of the average number of neurons per field of view (approximately 20 mm2) as a function of cell density. **p = 0.0097. (C) Quantification of the average number of neurites per neuron as a function of cell density. (D) Quantification of the average number of neuritic connections as a function of cell density. At least ten different fields out of three independent experiments were quantified.

To further characterize the degree of neuronal development and orientation, cells were observed microscopically by histological and immunofluorescent stainings and also scanned at greater detail by SEM (Figure 4). May Grunwald's eosin methylene blue staining showed good interconnection of cells with apparent neuronal morphology (Figure 4A). SEM images confirmed the existence of neuritic extensions that connected the differentiated PC12 cells (Figures 4B–D). Furthermore, differentiated PC12 cells expressed neuronal marker NFL (95.7% ± 4.2) and dopaminergic neuronal marker TH (84.4% ± 7.5) (Figures 4E,F, respectively). Taken together, these results indicated that PC12 cells, differentiated in the absence of NGF, presented an apparently mature neuronal phenotype (TH+ and thus potentially capable of producing dopamine and norepinephrine).

Figure 4

PC12 cells differentiate to interconnected tyrosine hydroxilase (TH)-positive neurons. (A) Differentiated neurons after 10 days differentiation of PC12 cells and staining with May Grunwald's solution. (B–D) Neuronal interconnectivity was appreciated in more detail by SEM (B), showing the emission of neurites from differentiated PC12 cells (C, red arrow) and the contact between them (D). Note the presence of traces of neural extracellular matrix in the preparation (C, blue arrow) after 14 days in vitro. A putative dopaminergic neuronal phenotype was shown by intracellular expression of neurofilament L (NFL; panel E) and tyroxine hydroxilase (TH; panel F) markers, as seen by inmmunofluorescence and confocal microscopy (red). Cell nuclei were counterstained with Hoechst 33258 (blue).

Validation of the substrate with primary dermal precursor cells

To validate the neural differentiation potential of the substrate on primary cells, we isolated adult rat SKPs under non-adherent conditions. Rat SKPs grown and expanded for 7 days in vitro formed dermospheres of variable diameters in suspension (Figure 5A). In our hands, >50% of dermospheres (53.4 ± 13.3%) presented a diameter of 50–200 μm, which was determined as the most appropriate sphere size for differentiation experiments (Figure 5B and data not shown). Within 24 h, seeded dermospheres attached to the matrix and started their differentiation. After 3 days, colonization of the surrounding matrix by some cells with an apparent neuronal morphology was observed. At day 7 neural networks started to be apparent in the sphere surroundings (Figure 5C), that were later expanded throughout culture substrate (Figure 5D). Neuronal phenotype of these cells was confirmed by Bodian's staining (Figure 5E) (Gambetti et al., 1981). In all cases, neurons differentiated over a “cushion” of apparently undifferentiated cells (Figures 5C–E; blue arrows).

Figure 5

Validation of the micropatterned substrate by neural differentiation of primary SKPs. (A) Dorsal skin dermospheres of small (green arrow), medium (yellow arrow) and large (red arrow) diameter size formed after 7 days in vitro. (B) Quantification of spheres with a diameter size below 50, in between 50 and 200, and over 200 μm. At least ten different fields out of three independent experiments were quantified. *p < 0.05; ***p < 0.001. Small panels on the right show typical spheres of the three size ranges. (C) Dermospheres collected with a micropipette and seeded onto the developed extracellular matrix in neuronal inducing medium showed apparent neurons with a clear polar morphology and neurite emissions (red arrow), as well as seemingly undifferentiated stromal cells (blue arrow) after 7 days in differentiation conditions. (D) A neuronal network was apparent after 10 days differentiation (green arrow). (E) Neuronal phenotype was confirmed by Bodian's silver proteinate staining (red arrow), although stromal cells non-differentiated to the neural lineage were also seen (blue arrow).

Finally, the neural phenotype of differentiated SKPs was confirmed by staining with anti-Nestin and anti-βIII-tubulin antibodies. As shown in Figure 6A, Nestin+ cells (42.5% ± 3.5%) presented cytoplasmic projections consistent with an immature neuronal phenotype after 10 days of differentiation. Four days later a remarkable decrease of Nestin+ cells (12.5% ± 2.1%) was detected, which was not further investigated. Concomitantly, Nestin− cells overproliferated in the culture. The remaining Nestin+ cells further matured, as shown by a significant increase in the size of their neuritic extensions (Figure 6B). At day 20, similar proportions of βIII-tubulin+ cells (7.5% ± 1.9%; Figure 6C) were detected, indicating that Nestin+ cells had evolved to cells with an immature neuronal phenotype, that presented long neuritic extensions. As aforementioned, a confluent monolayer of cells undifferentiated to the neural lineage (βIII-tubulin−) was consistently found below immature neurons. These cells were α-SMA+, indicating their myofibroblastic phenotype (Figure 6D). It was not possible to further follow up differentiation since cultures started to degenerate after 20 days. In summary, neural ECM promoted the differentiation of primary rat SKPs into seemingly immature neurons.

Figure 6

SKPs differentiate onto seemingly immature neuronal cells. (A–B) After 10 days differentiation, SKPs differentiated into neuronal-like cells that expressed nestin (red; red arrow). Nestin negative cells (white arrow) were also present. (C) Immature neuronal phenotype was confirmed by βIII-tubulin staining (green). (D) Undifferentiated stromal cells expressed α-SMA marker (red). Nuclei were counterstained with Hoechst 33258 (blue).

Discussion

Previous studies on the adhesion, proliferation, orientation, and migration of cells on biocompatible surfaces show that surface microgeometry influences neuronal cell behavior and neuritic outgrowth, i.e., showing improved adhesion of cells to the substrate and growth parallel to the direction of the grooves (Lim and Donahue, 2007; Norman et al., 2009; Rao and Winter, 2009). In 1988, Kleinfeld first used photolithographied glass substrates for the culture of dissociated neurons (Kleinfeld et al., 1988). Since then, micropatterned substrates combined with adhesive surface coatings have enabled researchers to precisely control the position and orientation of individual neurons (Chang and Sretavan, 2008). Thus far, simple neural circuits that can be aligned with arrays of microelectrodes have been created, both flat and tridimensional (Francisco et al., 2007; Jaber et al., 2009; Williams, 2009; Carabelli et al., 2010). However, many polymers used in these processes are unsuitable for biological systems. They are not optimized to interact with cells and have neither the composition nor the functionality that would correspond to a true ECM (Delcroix et al., 2010). For these reasons, new scaffolds that combine biodegradable synthetic polymers with components of the natural ECM are needed.

As a first study, we chose relatively wide (200 μm) channels to fit a number of cells in parallel since our experimental approach was targeted for neural tissue engineering, not for neural circuits in which narrower channels are more appropriate. In a somewhat related work, Lee et al. showed that human embryonic stem cells seeded onto 350 nm ridge/groove pattern arrays differentiated into neuronal lineage after 5 days, in the absence differentiation-inducing agents (Lee et al., 2010). We have not thus tested the impact of channel sizing on development and differentiation of neuronal cells. However several recent studies have addressed the issue channel size and fiber topography can also play a vital role in regulating differentiation and proliferation of rat hippocampus-derived adult NSCs (rNSCs) on laminin-coated electrospun polyethersulfone fibers (Christopherson et al., 2009). For instance Béduer et al. elegantly showed that adult human neural stem cells have a preference for a channel width larger than cell soma diameter when seeded on micropatterned PDMS surfaces (Beduer et al., 2012).

Here we presented a polymeric substrate with two complementary components whose combination is novel: a synthetic surface microgeometry capable of supporting and directing the cells to a coupled differentiation process and a neural ECM formulated with proteins and molecules that induce neuronal differentiation.

With regard to its physical structure, our ECM has an adequate porous fibrosity to accommodate neuronal differentiation, similar to other neural matrices that have used distinct biomaterials and, more importantly, similar to the porosity of the natural rat brain matrix (Bettinger et al., 2009; Christopherson et al., 2009). Of note, our fibrous network tends to increase its volume in culture medium possibly due to hydration capacity provided by the presence of low molecular hyaluronic acid, which will facilitate, in turn, cell movement and neurite extension. However and as a word of caution, it should be noted that while the hyaluronic acid of high molecular weight (>500 kDa) is anti-angiogenic, anti-inflammatory and immunosuppressive, hyaluronic acid of low molecular weight (10–500 kDa) is highly angiogenic and proinflammatory (Csoka et al., 2001; Stern, 2004). In theory, this single fact would prevent further use of the substrate in vivo as formulated, unless rigorous testing shows an appropriate safety profile of the inserted constructs. In any case, the possibility of incorporating biologically active molecules combined with neurotrophic factors into the neural ECM is a promising tool for cell differentiation analyses in vitro. In fact, a reduced concentration of inducer molecules is needed to generate a response when incorporated into ECM as compared to soluble administration (Bhang et al., 2009; Valmikinathan et al., 2009).

Work by others have shown the influence of micro- and nanogeometries (Mahoney et al., 2005; Koh et al., 2008; Cao et al., 2009; Xie et al., 2009; Ferrari et al., 2010), conductive polymers (Green et al., 2009), functional groups (Lamour et al., 2009; Ren et al., 2009), surface-immobilized peptides and molecules (Cooke et al., 2010; Lamour et al., 2010) and cell density (Ruiz et al., 2008) on the differentiation and neurite extension of PC12 cell line and neural stem/progenitor cells. In the present article, we corroborate that substrate microgeometry in combination with the synergistic action of the matrix allows the development of large PC12 networks. However use of continuous cell lines such as PC12 has a relatively little impact on development of tissue engineering products for human use, as compared for instance to rodent and human neural precursor cells.

Foetal, neonatal and adult SKP cells from several species have been previously isolated and characterized by several groups, including our own (Gago et al., 2009). However there is ample room for improvement of current protocols to isolate, enrich, expand, and differentiate these cells into the neural lineage. In the present work, adult SKPs were chosen since their therapeutic application is more obvious. Dermosphere-derived cells expressed Nestin in early stages of differentiation. However, stromal cells (presumably acting as structural and trophic support vehicles to make neurons mature) presented a higher rate of proliferation on the substrate that finally provoked degeneration of differentiation cultures after day 20. This might be the reason why no MAP2/TH positive neurons have been detected from SKPs (data not shown), although other groups also failed to differentiate SKPs into mature neurons in vitro by using more standard culture conditions (Gingras et al., 2007; Fernandes et al., 2008). As an alternative, it will be interesting to explore the differentiation potential of SKPs into cells of the glial lineage such as Schwann cells (Biernaskie et al., 2006; Fernandes et al., 2006; McKenzie et al., 2006) on the newly developed substrates.

The neurons here obtained were characterized by Bodian's method which stains neurofilaments, i.e., neuron-specific cytoplasmic intermediate filament proteins (Gambetti et al., 1981). On the other hand, βIII tubulin antibody has been widely used in the literature to “specifically” immunostain both neurons and other neural precursor cells. Since SKPs are known to generate both immature neurons and Schwann cells in vitro, we would expect to have more βIII tubulin+ cells than Bodian+ cells, although the exact relationship between both cell types and concurrent stainings has not been properly addressed in this manuscript. It should also be noted that TH+ neurons are not necessarily dopaminergic (DA) and future studies will analyze other markers such as D2 dopamine receptor or dopamine transporter and the presence of neuronal processes characteristic of DA neurons. Likewise, electrophysiological recordings would best assess functional interconnectivity of the neurons.

In conclusion, a biocompatible micropatterned support with neural-like ECM that can efficiently induce the neural differentiation of precursor cells has been generated. Although we have not investigated the issue in detail, neuronal cells do not seem to sense geometry after a certain maximum channel wideness (about 50 μm) and apparently recognize big (>200 μm) channels as a flat surface (Yang et al., 2005; Solanki et al., 2010). For this reason we believe that matrix components deposited over micropatterned substrates allowed cell adhesion and differentiation into neurons. To our knowledge, the unique combination of proteins, signaling factors and biomaterials presented here represents a major improvement on the neural differentiation of SKPs in vitro. This biomaterial-ECM-cell differentiation system could also be tailored to generate other cell types, and also incorporate additional neural inducing factors that may be released progressively to the medium as desired. In our view, this new 3D culture system will represent a useful tool for modeling the effect of drugs on neural signaling pathways. Usefulness of this differentiation system for the transplantation of in vitro engineered neural tissue will need to be shown through preclinical validation, via in vivo experiments on the relevant animal models of disease.

Conflict of interest statement

The authors declare that the research was conducted in the absence of any commercial or financial relationships that could be construed as a potential conflict of interest.