Three-Dimensional Environment Sustains Morphological Heterogeneity and Promotes Phenotypic Progression During Astrocyte Development

Abstract

Astrocytes are critical for coordinating normal brain function by regulating brain metabolic homeostasis, synaptogenesis and neurotransmission, and blood–brain barrier permeability and maintenance. Dysregulation of normal astrocyte ontogeny contributes to neurodevelopmental and neurodegenerative disorders, epilepsies, and adverse responses to injury. To achieve these multiple essential roles, astrocyte phenotypes are regionally, morphologically, and functionally heterogeneous. Therefore, the best regenerative medicine strategies may require selective production of distinct astrocyte subpopulations at defined maturation levels. However, little is known about the mechanisms that direct astrocyte diversity or whether heterogeneity is represented in biomaterials. In vitro studies report lack of normal morphologies and overrepresentation of the glial scar type of reactive astrocyte morphology and expression of markers, questioning how well the in vitro astrocytes represent glia in vivo and whether in vitro tissue engineering methods are suitable for regenerative medicine applications. Our previous work with neurons suggests that the three-dimensional (3D) environment, when compared with standard two-dimensional (2D) substrate, yields cellular and molecular behaviors that more closely approximately normal ontogeny. To specifically study the effects of dimensionality, we used purified glial fibrillary acidic protein (GFAP)-expressing primary cerebral cortical astrocyte cultures from single pups and characterized the cellular maturation profiles in 2D and 3D milieu. We identified four morphological groups in vitro: round, bipolar, stellate, and putative perivascular. In the 3D hydrogel culture environment, postnatal astrocytes transitioned from a population of nearly all round cells and very few bipolar cells toward a population with significant fractions of round, stellate, and putative perivascular cells within a few days, following the in vivo ontogeny. In 2D, however, the population shift from round and bipolar to stellate and perivascular was rarely observed. The transition to distinct cellular morphologies in 3D corresponded to the in vivo expression of phenotypic markers, supporting the generation of mature heterogeneous glial populations in vitro. This study presents quantitative data supporting that 3D culture is critical for sustaining the heterogeneity of astrocytes in vitro and for generating a representation of the in vivo portfolio of heterogeneous populations of astrocytes required for therapeutic interventions in neurodevelopmental disorders, epilepsy, and brain injury.

Introduction

Traditionally, adult astrocytes were considered as a homogeneous population that supports neuronal function.¹ In the last three decades, this view has changed to recognize that the in vivo astrocyte population is heterogeneous and dynamic, allowing the cells to perform a variety of complex functions in the central nervous system (CNS).^2–6 In the mouse, astrocytes are generated during the late embryonic and neonatal periods.^7–11 Astrocytes arise from neuroprogenitor cells after the generation of neurons,¹² and it is estimated that 10–15% of astrocytes derive from radial glia.¹³ In the mouse, the first three postnatal weeks are a period of massive astrocyte expansion and migration, followed by maturation.¹⁴

During development, astrocytes guide the migration of neurons and direct axonal outgrowth and synapse formation.^15–19 Astrocyte dysfunction has been observed in developmental disorders of autism, Fragile X and Rett syndromes, as well as adult psychiatric diseases and seizure disorders.^20–26 In the healthy adult brain, astrocytes are responsible for functions, such as homeostasis of fluids, ions, pH, and neurotransmitters, as well as synaptic transmission and blood flow regulation.^5,27 Most recently, astrocytes have been reported to communicate with adjacent neurons using gliotransmitters and to have the capacity of neural stem cells (NSCs).²⁸ Upon injury, astrocytes have the potential to transform into a reactive state: become hypertrophied and release cytokines and extracellular matrix molecules to form a glial scar, which is hypothesized to prevent further tissue damage while severely impairing neuronal function.^29–32 Recent findings of reactive astrocytes in neurodegenerative disorders point to possible roles in Alzheimer's and Parkinson's diseases and amyotrophic lateral sclerosis.^25,33 It is not known if all astrocytes possess the capacity for the attributed functions or whether specific abilities are attributed to subpopulations of cells. Accumulating evidence supports astrocyte diversity with respect to developmental origin, morphology, gene expression, and function.

Astrocytes at different stages of postnatal development are morphologically and functionally diverse. At least four morphological forms of astroglial cells exist during astrocyte development: radial glial progenitors, proliferating intermediate progenitors, maturing postnatal astrocytes, and adult astrocytes, which include stellate and perivascular types.³⁴ Little is known about the mechanisms that regulate astrocyte heterogeneity or the pathways that favor astrocyte subtypes with therapeutic potential.²⁸ However, embryonic origin seems to contribute to astrocyte diversity, such that cerebral cortical astrocytes differ biochemically and physiologically from those generated by the hippocampus.³⁵ Numerous studies have highlighted differences in astrocyte gene expression in differential brain regions, with respect to injury response, and between in vivo and in vitro growth environments.^{1,5,6,11,28,34,36} Thus, we propose that the development of more effective treatments requires a more detailed understanding of astrocyte heterogeneity and ontogeny in tissue engineering applications.

Currently, astrocytes are identified in mixed cultures from embryonic and neonatal brains by the expression of glial fibrillary acidic protein (GFAP). Often GFAP-expressing (GFAP⁺) cells obtained from the differentiation of NSCs or induced pluripotent stem cells are surmised to be astrocytes. While astrocytes do express GFAP early in the postnatal period, adult astrocytes (especially gray matter protoplasmic astrocytes) exhibit little or no GFAP in the healthy CNS.³⁷ Rather, during normal ontogeny, GFAP expression is downregulated. Therefore, the current in vitro approaches do not generate phenotypic in vivo astrocytes, although newer isolation methods are narrowing the gap for short-term culture of adult astrocytes.³⁸ Thus, to achieve cells that represent the normal in vivo phenotypes and serve to redirect aberrant trajectories of human disease, better tissue engineering substrates and methods are required.

The standard method of isolating and culturing postnatal brain astrocytes in tissue culture polystyrene flasks was developed >30 years ago by McCarthy and de Vellis.³⁹ Although this method yields a high number of nearly pure GFAP immunoreactive astrocytes, recent work has established that astrocytes cultured on traditional two-dimensional (2D) substrates may not fully represent in vivo astrocytes. These astrocytes do not appear to progress through normal ontogeny through the downregulation of the early marker of GFAP and upregulation of mature astrocyte markers. The continued expression of GFAP has been interpreted to represent the reactive astrocyte phenotype,⁴⁰ yet these GFAP⁺ astrocytes do not show hypertrophy of reactive astrocytes⁴¹ or the glutamate-dependent calcium signaling of mature astrocytes.⁴² We hypothesize that changing the culture environment can direct the purified astrocytes through normal ontogeny and provide a source for engineering astrocytes for clinical applications.

Three-dimensional (3D) cultures potentially provide a bridge between cell biological experiments, which employ 2D substrates (e.g., polystyrene, glass) and in vivo studies of cell behavior in the native 3D environment.^43,44 Our group has previously demonstrated that the morphology and signaling pathways of sensory neurons are dramatically altered when the cells are placed within a 3D versus 2D microenvironment, with the cellular response occurring in 3D collagen gels being a better representation of the in vivo scenario than 2D cultures.^45,46 In this work, we hypothesize that an engineered 3D microenvironment has the potential to direct astrocytes to follow innate programmed instructions to enable phenotypic diversity in vitro.

To characterize astrocyte heterogeneity with varying microenvironment dimensionality, we started with purified perinatal mouse cerebral cortical gray matter astrocytes and grew them on the traditional 2D collagen-coated coverslips and in 3D collagen gel in defined media. We observed distinctive differences in astrocyte morphology between 2D and 3D, specifically, a stellate-like morphology was observed in 3D, but not in 2D, cultures. We characterized physical and chemical conditions and their role in astrocyte phenotype determination. The work presented herein is a first step toward understanding astrocyte heterogeneity in 2D versus 3D culture. Our results indicate that astrocytes sense the dimensionality of their environment, and then modulate morphology, proliferation rate, and the expression of phenotypic markers. We report an improved in vitro culture method for producing astrocyte populations, which better reflects the in vivo cellular heterogeneity and allows observation of morphological and biochemical changes during normal maturation and in response to neuronal injury. Altogether, our quantitative findings suggest that the context of the cellular microenvironment is critical toward the progression of innate cellular programs.

Materials and Methods

Materials were obtained from Sigma-Aldrich or Invitrogen-Life Technologies unless otherwise noted.

Mice

C57BL/6^J mice (Jackson Laboratory) were used. All animal studies were approved by the University of Maryland School of Medicine Institutional Animal Care and Use Committee and performed in accordance with NIH guidelines. The day of birth was counted as postnatal day (P) 1.

Astrocyte culture

Astrocytes were dissected from P1–P3 mouse cerebral cortices following standard protocols to isolate gray matter astrocytes.³⁹ Astrocytes were expanded in tissue culture flasks (Corning) for 10–14 days and purified by shaking at 250 rpm for 8 h, after which the nonadherent cells were removed. This classic procedure yields cultures that were >98% astrocytes as assessed by positive GFAP immunoreactivity. Each flask contained the cells isolated from a single mouse pup cerebral cortex. Astrocytes were seeded at 7.5 × 10³ cells/cm² onto 2D collagen-coated coverslips (∼7 μg/cm²) and at 7.5 × 10⁵ cells/mL within 3D collagen gels (2 mg/mL, 25 μL) and then cultured for 4 or 10 days, with media changes every 2 days. The plating densities were chosen to reflect the densities of glial progenitors and astrocytes in the early postnatal brain.⁴⁷ In all cases, rat tail type I collagen (BD Biosciences) was used; methods to generate 2D coverslips and 3D gels were adapted from Ribeiro et al.⁴⁵

Cells were maintained in serum-containing medium (Dulbecco's modified Eagle's medium [DMEM, high glucose, 4.5 g/L] supplemented with 10% fetal bovine serum and penicillin [100 U/mL] and streptomycin [100 μg/mL]) or in serum-free medium (DMEM supplemented with 1 × N2 supplement and penicillin [100 U/mL] and streptomycin [100 μg/mL]). For 2 mg/mL collagen gels, ice-cold reagents, including 10 × DMEM, 7.5% sodium bicarbonate, sterile deionized water, and collagen, were combined with cells to generate 3D substrates. The collagen/cell solution was allowed to gel in a culture incubator for 30 min before addition of culture medium. For each experiment, cells from a single flask were used for both 2D and 3D substrates. Unless otherwise noted, the cells were plated at 7.5 × 10³ cells/cm² on 2D or 7.5 × 10⁵ cells/mL in 3D. To test the effects of plating density, cells were plated at low (5 × 10³ cells/cm² on 2D or 5 × 10⁵ cells/mL in 3D), medium (7.5 × 10³ cells/cm² on 2D or 7.5 × 10⁵ cells/mL in 3D), and high density (1.5 × 10⁴ cells/cm² on 2D or 1.5 × 10⁶ cells/mL in 3D).

Immunofluorescence and image analysis

Samples were fixed in 24-well plates in buffered 4% formaldehyde solution for 20 min and permeabilized with Tris-buffered saline (TBS) containing 0.1% Triton X-100 and incubated with 10% lamb serum in TBS blocking solution for 30 min (in 2D) and 2 h (in 3D). The astrocytes were incubated in primary antibodies to GFAP (1:300; Abcam), S100β (1:300; Abcam), RC2 (1:250; Millipore), and nestin (1:300; Santa Cruz) for 1 h for 2D cultures, followed by appropriate fluorescently conjugated secondary antibodies (Jackson ImmunoResearch) for 30–60 min. A solution of 4′,6-diamidino-2-phenylindole (DAPI, 300 nM) was used to visualize cell nuclei. Immunofluorescence procedures for the 3D gels used the same antibody concentrations, but had longer washing steps (>30 min each) and overnight antibody incubations. Samples were imaged with confocal microscopy (Leica TCS SP5) and analyzed with LAS AF software (Leica) under the same confocal settings. For immunohistochemistry controls, some samples were incubated with only the primary or the secondary antibodies. Viability was assessed using the LIVE/DEAD assay according to the manufacturer's instructions (Molecular Probes Products, ThermoFisher Scientific).

Proliferation study

Cell proliferation during culture was measured using the Click-iT EdU kit (Life Technologies). Astrocytes were incubated with EdU for 4 days in culture, with media changes every 2 days. The cells were then fixed, permeabilized, incubated with Click-iT detection cocktail for 30 min for 2D cultures and overnight for 3D cultures, and followed by DAPI staining. Cell nuclei that proliferated during EdU incubation fluoresced green due to detection of EdU using AlexaFluor 488. DAPI (blue) stains all nuclei. The cultures were imaged and the numbers of EdU⁺ and DAPI⁺ cells were counted.

Statistical analyses

Each flask represented cells that were harvested from a single pup and therefore each flask represented an independent sample of cells (∼1 × 10⁶). For each experiment, the cells from a single flask were tested in each of the dimensions: 2D and 3D (Fig. 1A). In some cases, the effects of medium composition (serum-containing or defined serum-free) were also tested. During each experiment, at least three to four individual cell populations (flasks) obtained from separate litters were evaluated. Plated cells were cultured for 4 or 10 days and then assessed for morphology, marker expression, and proliferation. For the characterization of cell morphology, 5–10 images were captured per sample, representing 50–100 cells for each sample. GFAP⁺ cells were scored manually according to the morphologies defined in Figure 2A–F. Each experiment represents at least n = 3 independent cell populations, and the experiments were repeated in triplicate. In Figure 3, the dataset passed the tests of normality and therefore statistically significant differences between experimental groups (p < 0.05) as influenced by dimensionality and media were determined by two-way analysis of variance (ANOVA), followed by Holm–Sidak post hoc analyses, if appropriate. To determine the significance (p < 0.05) of variation of cell group distribution due to the influence of culture parameters, we used a chi-square test. If the distributions were significantly different, then individual groups were compared using a Mann–Whitney rank sum test with a t-test for normally distributed data (determined by Shapiro–Wilk) or a Mann–Whitney U statistic.

FIG. 1.

Schematic of experimental strategy. (A) Gray matter cerebral cortical astrocytes were isolated from individual mouse pups at P1–P3. The astrocytes from a single pup are grown and purified in an individual flask and then used to compare the cellular responses to 2D and 3D environments. Each color represents an individual pup and cells obtained from it. Each experiment simultaneously compared astrocytes derived from three to four individual pups grown in 2D and 3D substrates and, in some cases, different medium formulations for each substrate. (B) Cells grown at a plating density of 7.5 × 10³ cells/cm² on a 2D substrate appear as flattened cobblestones and are immunoreactive for GFAP (red fluorophore). (C) Cells grown within the 3D substrate (7.5 × 10⁵ cells/ml) are distributed throughout the scaffold and are observed at multiple focal planes. The cells are immunoreactive for GFAP (red fluorophore) and appear much smaller than those in 2D (B). DAPI (blue) is used to stain cell nuclei. Scale bar: 50 μm. 2D, two-dimensional; 3D, three-dimensional; GFAP, glial fibrillary acidic protein. Color images available online at www.liebertpub.com/tea

FIG. 2.

Astrocytes exhibited unique profiles of morphologies dependent upon in vitro growth environment. Representative confocal images of primary astrocytes grown on 2D collagen-coated coverslips (A, C, E) or within 3D collagen gels (B, D, F) for 4 days in serum-containing media show immunoreactivity for the astrocyte marker, GFAP, as shown in red and cell nuclei are labeled with DAPI (blue). Multiple morphologies were observed in the GFAP⁺ cells: round, without distinct processes or projections (A, B), bipolar cells, which had two opposing processes (C, D), and stellate cells, with multiple processes emerging from a centrally located soma (E, F). The stellate cells resembled mature astrocytes in vivo. (G) Distribution of morphologies in 2D and 3D cultured substrates. Asterisks denote significant differences between the percentages of cells grown in 3D exhibiting each morphology compared with those on 2D substrates (p < 0.001 level). Scale bar: 20 μm. Please note that the cell in (B) is much smaller than the others. Color images available online at www.liebertpub.com/tea

FIG. 3.

Growth medium composition and substrate dimensionality contributed to the profiles of astrocyte morphologies. Astrocytes were cultured for 4 days in either serum-containing (A, C, E) or serum-free defined media (B, D, F). Plating density was not a major factor determining the percentage of GFAP⁺ cells with round (A, B), bipolar (C, D), or stellate morphologies (E, F). Substrate dimension significantly altered each cell morphology category for all plating densities in serum media. Serum-free media induced significant distributions in cell morphologies that were dependent upon plating density and often different from serum-containing media. Dimensionality contributed dramatic shifts in the distributions of cell morphologies, with interactions with plating density and medium composition. For 2D experiments: low density is 5 × 10³ cells/cm², medium density is 7.5 × 10³ cells/cm², and high density is 1.5 × 10⁴ cells/cm². For 3D experiments, low density is 5 × 10⁵ cells/mL, medium density is 7.5 × 10⁵ cells/mL, and high density is 1.5 × 10⁶ cells/mL. Each bar represents the mean ± SEM of at least n = 3 independent samples of >50 astrocytes per sample. An asterisk denotes a significant difference between cells comparing 2D and 3D substrates at the p < 0.05 level.

Results

Effects of culture dimensionality on astrocyte morphology

To test whether 3D culture influences the morphological heterogeneity of astrocytes, we compared the morphology of astrocytes cultured at medium density: 7.5 × 10³ cells/cm² on 2D collagen-coated coverslips and 7.5 × 10⁵ cells/mL in 3D collagen gels (Fig. 1A). First, experiments were carried out for 4 days in serum-containing media, after which the cells were fixed and processed for GFAP immunoreactivity (Fig. 1B, C). Examination of the astrocyte morphologies revealed that distinct differences existed between cells cultured on 2D collagen-coated glass substrates and within 3D collagen gels (Fig. 2).

We identified three main groups of GFAP⁺ astrocyte morphologies at 4-day culture period: round, bipolar, and stellate. Round astrocytes formed the majority of the population. On 2D substrates, round astrocytes were predominantly flat and large (∼25 μm diameter) (Fig. 2A), while round astrocytes in 3D environment were relatively small (∼10 μm) and spherical (Fig. 2B). Bipolar astrocytes had a small round soma with two opposing processes (Fig. 2C, D), resembling the in vivo radial glial phenotype, and were observed both on 2D and in 3D cultures.^48–52 Stellate astrocytes resembled the star-shaped astrocytes found in vivo (Fig. 2E, F)^53–55 and were predominantly observed in 3D cultures. The unique morphologies of the GFAP⁺ cells resemble the in vivo ontogeny from glial precursor to mature astrocyte. We observed significant differences in the distributions of morphologies of the GFAP⁺ cells cultured on 2D and 3D substrates (Fig. 2G, χ² = 38.792, p < 0.001). In 3D, there were significantly fewer round cells (t = 9.047, p < 0.001), but more bipolar (t = 6.770, p < 0.001) and stellate cells (t = 45, p < 0.001). These data suggest that the substrate environment could influence glial ontogeny.

Quantitative assessment of astrocyte morphology in 2D and 3D environments

We initially tested the effects of several factors that may influence glial morphology and maturation after 4 days in vitro, including cell density, composition of the culture medium (serum-containing or serum-free), and dimensionality of the culture substrate (Supplementary Fig. S1 and Fig. 3; Supplementary Data are available online at www.liebertpub.com/tea). With serum-containing media, the majority of GFAP⁺ cells on the 2D substrates plated at medium density were round (96% ± 1%) with a small number of cells appearing bipolar (4% ± 1%) or stellate (<1%). By comparison, in 3D at medium density, fewer of the GFAP⁺ cells were round (83% ± 2%) and greater proportion of the cells were bipolar (13% ± 1%) or stellate (6% ± 1%). Comparing astrocytes grown in 2D, we observed overall differences in the distributions of morphologies with respect to serum content in the medium (χ² = 72.248, p < 0.001) and with respect to plating density in serum (χ² = 17.329, p = 0.002) and serum-free media (χ² = 18.463, p = 0.001, Supplementary Fig. S1A).

In 3D, the distributions of morphologies were different when comparing serum-containing and serum-free media (χ² = 88.211, p < 0.001 for low density, χ² = 57.769, p < 0.001 for medium density, and χ² = 56.884, p < 0.001 for high density, Supplementary Fig. S1B). However, the distributions of morphologies were not different when compared across densities in serum-containing medium (χ² = 2.468, p = 0.650). In the absence of serum, the distributions were different (χ² = 61.576, p < 0.001). Comparisons of the distributions with respect to dimensionality (2D vs. 3D) revealed that under all media and density conditions, astrocytes grown in 3D displayed different percentages of round, bipolar, and stellate cells than the same astrocyte population in 2D (χ² > 25.585, p < 0.001 for all comparisons).

The marked significant differences observed in the distributions of astrocyte morphologies led us to examine the effects of dimensionality, serum content, and density on the individual morphological groups. For clarity, data from each morphological group are presented in separate graphs (Fig. 3) to determine the effects of dimensionality and plating density. For round cells in serum-containing media, there was an effect of dimensionality (F = 163.168, p < 0.001), but no effect of plating density (F = 1.847, p = 0.169, Fig. 3A). In serum-free media, the round phenotype was not affected by either dimensionality (F = 0.0474, p = 0.828) or plating density (F = 0.0784, p = 0.925, Fig. 3B). For the bipolar morphology, there was a main effect of dimensionality (F = 66.899, p < 0.01), but not plating density (F = 2.765, p = 0.073) in serum-containing media (Fig. 3C). In serum-free media, the bipolar shape was affected by both dimensionality (F = 17.893, p < 0.001) and plating density (F = 4.231, p = 0.020, Fig. 3D). Finally, for the stellate group of cells grown in serum-containing media, there was a main effect of dimensionality (F = 71.161, p < 0.001), but not plating density (F = 0.110, p = 0.896, Fig. 3E). In serum-free media, the stellate shape was affected by both dimensionality (F = 13.329, p < 0.001) and plating density (F = 3.430, p = 0.041), with a significant interaction between the parameters (F = 6.641, p = 0.003, Fig. 3F). Overall, dimensionality and serum content of the media had significant influences on all observed astrocyte morphologies. Because the impact of plating density was generally small and often not significant, we chose a standard density of 15,000 cells within 25 μL collagen gels (7.5 × 10⁵ cells/mL) for the rest of the experiments.

Influence of physical location within the 3D environment on cell morphology

We independently tested the effects of the relative physical location in the gel to determine if the observed morphologies were the same throughout the substrate. Based on chi-square analysis, there was no effect of the physical position of the cells within the gel, that is, whether the cells were located in the center or near the edge in serum-containing (χ² = 9.511, p = 0.484, Supplementary Fig. S2A) or serum-free media (χ² = 3.301, p = 0.192, Supplementary Fig. S2B).

Effects of medium composition and culture dimensionality on astrocyte proliferation

We counted the total number of GFAP⁺ cells after 4 days in culture and found an overall effect of dimensionality (F = 18.166, p < 0.001), but no effect of medium composition (F = 3.680, p = 0.064) and a significant dimension x serum interaction (F = 10.115, p = 0.003). Post hoc analysis revealed that significantly more cells were present after being grown in 3D with serum-free media (p < 0.001, Fig. 4A). The total number of cells is the combined measure of the initial cells plated plus any born over 4 days minus those lost to cell death. To determine the influence of culture dimensionality and medium composition on astrocyte proliferation, we performed an EdU proliferation assay. EdU is a thymidine analog that is incorporated into DNA during the S-phase of cell division (Fig. 4B).⁵⁶ Analysis of the EdU incorporation provided an estimate of the newly born cells that exit the cell cycle. Cells that re-enter the cell cycle may lose the EdU signal through dilution of multiple divisions.^57–59 Our analysis revealed a main effect of dimension (F = 30.614, p < 0.001) and no effect of serum (F = 2.886, p = 0.099) or dimension × serum interaction (F = 57.878, p = 0.087). In serum-containing medium cultures, 19% ± 2% EdU⁺ cells were observed in 2D compared with 13% ± 2% in 3D, and in serum-free media, 19% ± 2% EdU⁺ were found in 2D compared with 8% ± 1% in 3D (Fig. 4C). In summary, dimensionality affected proliferation of GFAP⁺ astrocytes and altered EdU⁺ incorporation.

FIG. 4.

Dimensionality and medium composition interact to alter cell proliferation and lineage. Astrocytes were cultured on 2D collagen-coated coverslips and within 3D collagen gels in serum-containing or serum-free media for 4 days. (A) The overall total number of cells, in equivalent regions, was increased in the 3D serum-free culture condition. (B) EdU was used to label cells that were in S-phase as a measure of cell proliferation. Double immunohistochemistry for GFAP (red) and EdU (green) demonstrates that round and bipolar astrocytes were among the proliferative populations. Bar = 10 μm. (C) Analysis of the percent of the population that had incorporated EdU yielded an effect of dimensionality. (D) The distribution of morphologies of EdU⁺ cells was dependent upon medium composition and culture substrate dimension. Bars represent mean ± SEM from n > 3 samples; in each sample, n > 50 astrocytes were counted. An asterisk denotes a significant difference at the p < 0.05 level for an effect of substrate dimension. Color images available online at www.liebertpub.com/tea

While counting the cells, we had the impression that more EdU⁺ cells had bipolar and stellar morphologies. When we assessed the distributions of morphologies, they were significantly different with respect to dimensionality in serum-containing (χ² = 89.381, p < 0.0001) or serum-free cultures (χ² = 74.141, p < 0.0001) (Fig. 4D). Within each morphology, post hoc analysis revealed significant differences for the astrocytes grown in 3D, with main effects of dimension (round: F = 51.439, p < 0.001; bipolar: F = 50.348, p < 0.001; and stellate: F = 6.511, p = 0.016). In 3D, fewer cells adopted the round shape in serum-containing (p < 0.001) and serum-free media (p = 0.001). Similarly findings were found for bipolar cells (serum-containing, p < 0.001 and serum-free, p = 0.017). For the stellate shape, only cells grown in serum-free medium were significantly different (p = 0.001). Overall, substrate dimensionality increased the proportion of proliferating astrocytes that exhibited the bipolar and stellate phenotypes.

Longer culture times reveal additional cell morphology

Astrocytes were cultured in parallel experiments in 3D gels for 4 and 10 days in serum and serum-free media. We examined cell viability using the LIVE/DEAD assay. Cell viability was estimated using the LIVE/DEAD assay. In 2D, 90% ± 9.5% viability was observed, whereas in 3D, 84% ± 8.6% were alive after 4 days (t = 2.66, p = 0.004). It should be noted that dead cells in the 2D condition are able to float away and thus are not counted, whereas in 3D, the cells are trapped and counted. Therefore, while the 2D cultures consistently had more viable cells, the size of the effect was modest.

After 10 days in culture, the distribution of morphologies was significantly different compared with 4 days (χ² = 423.387, p < 0.001), with decreased populations of round cells (73% ± 2% for serum and 75% ± 2% for serum-free) and bipolar cells (6% ± 1% for serum and 5% ± 0.5% for serum-free), but increased proportion of stellate cells (9% ± 1% for serum and 7% ± 1% for serum-free) (Fig. 5A).

FIG. 5.

Long-term culture in 3D substrates revealed a novel cell morphology. (A) Astrocytes were cultured in 3D substrates for 4 and 10 days in serum-containing and serum-free media. After 10 days in culture, fewer round astrocytes were observed, but the percent of bipolar and stellate cells remained similar to 4 days. However, a new type of cell that resembles the perivascular astrocyte proximal to blood vessels in vivo was observed. (B) The perivascular type of astrocyte is GFAP⁺ and has a long central process and several fine endfeet. (C) Schematic of the progression of astrocyte phenotypes during perinatal maturation, adapted from Hunter and Hatten.⁶⁰ Bars represent mean ± SEM from at least n = 3 samples; in each sample, n > 50 astrocytes were counted. Asterisks denote significant effect of medium composition (p < 0.05), whereas ampersands show significant effects of time in culture (p < 0.05). Scale bar: 20 μm. Color images available online at www.liebertpub.com/tea

An additional rare morphology that resembled a perivascular astrocyte was observed (11% ± 1% for serum and 12% ± 2% for serum-free). The putative perivascular-like astrocytes did not fit to the general morphology of the other three categories and had a long prominent process and multiple finer processes that appeared to be glial endfeet that contact blood vessels (Fig. 5B).⁶⁰ The perivascular-like cell was rarely present in the 4-day 3D cultures and was never observed in the 2D samples.

Within each morphology, post hoc analysis revealed overall effects of time (round, F = 139.168, p < 0.001; bipolar, F = 9.016, p = 0.005; stellate, F = 10.361, p = 0.003; and perivascular, F = 317.11, p < 0.001, two-way ANOVA). Overall effects of serum content in the media were observed for round (F = 50.980, p < 0.001) and bipolar cells, (F = 58.651, p < 0.001), but not stellate (F = 2.251, p = 0.143) and perivascular cells (F = 3.309, p = 0.078). In summary, time and serum content of the media affected the distribution of morphologies observed in the 3D substrates. A proposed model of astrocyte ontogeny is shown in Figure 5C, including the putative perivascular group.

Phenotypic characterization of astrocyte groups in 2D and 3D environments

Astrocytes express characteristic markers depending on the stage of development.^{7,34,35,61–65} To correlate the astrocyte morphological populations with the in vivo phenotypes, we characterized astrocytes cultured on 2D collagen-coated coverslips and in 3D collagen gels for 10 days, with markers of cell development stage, including nestin,⁶⁶ RC2,⁶⁷ GFAP,⁶⁸ and S100β.^69,70 GFAP is an intermediate filament protein and a classic marker that is used in the immunocytochemical identification of astrocytes.⁵ The RC2 antibody recognizes a 295 kDa intermediate filament proximal protein expressed in radial glial cells in the developing CNS.^67,71 S100β, a calcium-binding protein, is strongly expressed in mature astrocytes.^72–74 Nestin is an intermediate filament protein that is expressed in immature astroglial cells, but is absent in resting adult astrocytes.⁷⁵ Nestin is reexpressed in reactive astrocytes in response to injury or neurodegenerative disorders in the adult brain.^76,77 We investigated the expression of biochemical markers on the two largest morphological subgroups: round (Fig. 6) and bipolar cells (Fig. 7). Stellate and perivascular astrocytes were negligible on 2D cultures and present only in 3D cultures, and both populations expressed GFAP and S100β, but they did not show any immunoreactivity with RC2 or nestin. The stellate and perivascular cells were observed too infrequently to obtain quantitative expression data.

FIG. 6.

Round GFAP⁺ cells mainly express the astrocyte marker, S100β. Representative fluorescent images of round astrocytes cultured on 2D collagen-coated coverslips (A, B, E, F) and in 3D collagen gels (C, D, G, H). Cells were colabeled for GFAP (red, A, C, E, G) and either S100β (B, D, green) or RC2 (F, H) or nestin. Cell nuclei were labeled with DAPI (blue). Scale bars: 20 μm. Please note the differences in cell size in 2D (A, B, E, F) and 3D (C, D, G, H). (I) Analysis of immunoreactivity patterns shows that the majority of the round cells express S100β, with only a few that were grown in 3D-expressing RC2 or nestin. Bars represent mean ± SEM from at least n = 3 samples; in each sample, n > 50 astrocytes were counted. An asterisk denotes a significant difference at the p < 0.05 level. Color images available online at www.liebertpub.com/tea

FIG. 7.

Bipolar cells express phenotypic markers of radial glia. Representative images of bipolar cells cultured on 2D (A, B, E, F, I, J) or 3D substrates (C, D, G, H, K, M). On 2D, the GFAP⁺ (red) bipolar cells colabeled with the mature astrocyte marker, S100β (B, green), as well as the radial glial markers, RC2 (F, green) and nestin (J, green). By contrast, in 3D, very few bipolar cells expressed S100β (D), but nearly all expressed RC2 (H) and nestin (M). Scale bar: 20 μm. (N) Expression of markers in bipolar cells. Bars represent mean ± SEM from at least n = 3 samples; in each sample, n > 50 astrocytes were counted. An asterisk denotes a significant difference at the p < 0.05 level. Color images available online at www.liebertpub.com/tea

In 2D cultures, round astrocytes expressed GFAP and S100β in the same cells (99% ± 1%, Fig. 6A, B), with almost no coexpression of GFAP and RC2 (Fig. 6E, F) or GFAP and nestin. In 3D cultures, the coexpression of GFAP and S100β (Fig. 6C, D) was less, at 79% ± 3%, with 3% ± 1% of the GFAP⁺ cells also expressing RC2 (Fig. 6G, H) and 12% ± 1% of the GFAP⁺ cells coexpressing nestin. We analyzed the differences in biochemical marker expression (Fig. 6I) and found an overall effect of marker type (F = 4535.912, p < 0.001) and a significant dimension x marker interaction (F = 82.573, p < 0.001), but no overall effect of dimension (F = 0.334, p = 0.566). Post hoc analysis revealed that for S100β (p < 0.001) and nestin expression (p < 0.001), the percentages of GFAP⁺ cells that coexpressed each marker in 3D were significantly different than 2D. No difference was observed for the RC2 marker (p = 0.087). Therefore, dimensionality of the substrate altered the S100β and nestin biochemical marker expression of the round astrocyte subpopulation.

Our initial observations of the bipolar astrocytes led us to propose that they may be radial glial cells, which express RC2 and nestin. Double immunocytochemistry for GFAP and S100β showed that while 85.1% ± 4.5% of the GFAP⁺ astrocytes grown on 2D also express S100β, only 4.5% ± 1.2% of the GFAP⁺ cells in 3D also expressed S100β (Fig. 7A–D). In contrast to the round cells, coexpression with RC2 (2D: 89.2% ± 3.0% and 3D: 96.2% ± 1.6%, Fig. 7E–H) and nestin (2D: 94.1% ± 3.0% and 3D: 94.5% ± 2.7%, Fig. 7I–M) was very high in the bipolar cells. Quantification of the percentages of the GFAP⁺ astrocytes that expressed each marker shows the marked differences in S100β expression (Fig. 7N). We found main effects of dimension (F = 109.349, p < 0.001) and biochemical marker (F = 193.847, p < 0.001) and a dimension x marker interaction (F = 145.761, p < 0.001). Post hoc analysis revealed a significant difference between 2D and 3D substrates in S100β expression (p < 0.001), but not RC2 (p = 0.087) or nestin expression (p = 0.931). In summary, the bipolar cells on 2D coexpressed S100β, while those cultured in 3D expressed RC2 and nestin, markers found in radial glia.

Discussion

One of the major challenges in neural tissue engineering is defining the in vivo environment of the brain and the essential components for achieving the repair or regenerative environment.^2,28,78 For decades, neurons have been grown alone in/on biomaterials or devices, with some success, while the roles of astrocytes in normal development and disease and injury were being discovered. The current understanding of the astrocyte role in healthy neural function encompasses guidance of neurons and axons, synaptogenesis, formation of the blood–brain barrier, and inflammatory responses to injury and disease. Integrating the neuronal and astrocytic components for neural tissue engineering applications is stymied by our incomplete understanding of neurobiology and limited engineering tools and approaches.^79–82 Our approach has focused on a carefully defined astrocyte population and its response to several controlled parameters within the engineered environment. Our data suggest that perinatal cerebral cortical gray matter astrocytes are capable of progressing through normal ontogeny in an engineered 3D environment, providing a critical step to re-creating a receptive environment for normal neural function.^83,84

In the brain, astrocytes are heterogeneous populations that differ in morphology, functional, and biochemical profiles, dependent upon their origin and developmental stage.^18,61 The most recent ideas suggest that astrocyte heterogeneity may direct brain regionality or NSC lineage.⁸⁵ Due to their heterogeneity, using astrocytes harvested from whole brains to evaluate biomaterials may obscure the different capacities of the substrates to support proliferation or specific functions. Therefore, we chose the well-studied perinatal cerebral cortical gray matter astrocytes.^16,39 While astrocytes have been successfully cultured, biochemical and morphological analyses indicate that cultured glia represent the reactive stages of ontogeny^40,61 and not the normal developmental trajectory.^18,34 Reactive astrocytes are commonly found in vivo after injury, in which the cells hypertrophy and release inflammatory cytokines and chemokines and generate extracellular matrix molecules that are hypothesized to inhibit nerve regeneration.^86–89

Using standard techniques, astrocytes are often harvested, grown, and then expanded on 2D substrates.^39,90 Although 2D cultures have provided valuable biological insights, cells cultured in 3D culture may better represent the in vivo response in the healthy brain^91–95 because cells in 2D do not appear to achieve normal maturation. One of the fundamental differences of 2D versus 3D culture is the distribution of cell–cell and cell–matrix interactions, which can alter signaling mechanisms regulating cell response.⁹⁶ We therefore hypothesized that a 3D culture may better maintain a heterogeneous astrocyte population characteristic of postnatal development in comparison with the 2D counterpart.

Astrocytes have been previously cultured in 3D electrospun scaffolds and in the Bioactive3D cell culture system, where astrocytes were treated as a single homogeneous population.^93,95 However, it is unclear whether these 3D culture systems support astrocyte heterogeneity and development in vitro. These reports used mixed cultures of gray and white matter astrocytes and did not follow the ontogeny and maturation processes. To characterize the populations of astrocytes that appear in 3D culture, we quantified astrocytes based on their morphology, marker expression, and proliferation to reflect reported differences in ontogeny. Focusing first on quantifying the heterogeneous astrocyte populations based on morphology (Fig. 2), we found that a 3D culture environment allows astrocytes to transition from a population of round and bipolar cells at 4 days toward a population with greater numbers of stellate and perivascular-like cells at 10 days. However, in 2D cultures, this population shift from round to bipolar involved a smaller fraction of the GFAP⁺ population compared with 3D and yielded no stellate or perivascular cells (Fig. 5). Our results suggest that the dimensionality of the cellular microenvironment influences astrocyte ontogeny with 3D culture providing an aspect of the in vivo environment that allows early postnatal astrocytes to transition to the fully differentiated stellate morphology.

Next, we characterized astrocyte heterogeneity as influenced by various properties of the culture system, including the presence of serum, cell density, and location in the gel (edge vs. center). Previous reports have not investigated the effects of varying culture parameters on cell growth and maturation, including morphology and expression of biochemical markers. In comparison with 2D cultures, cells cultured in 3D may be more affected by restricted mass transfer of solutes throughout the gel and altered spatial distributions of cell and matrix ligands in the gel, thus leading to subpopulations dependent upon location. We observed that there is little influence on astrocyte heterogeneity with respect to location in the 3D substrates (Supplementary Fig. S2), likely due to the large pore size of collagen, which provides for a minimal barrier to solute transport.⁹⁷ These results suggest that macroporous gels such as collagen possess the architecture suitable to allow adequate solute transport.

The serum content of the media had the greatest effect on distribution of cell morphologies. We observed an interaction between dimensionality and serum content in the representation of bipolar and stellate groups (Fig. 3). These data imply that cell fate may be directed by a combination of serum-containing factors and microenvironment dimensionality and to a lesser extent cell density. Future studies will explore how the gels provide a 3D structure for ECM deposition and cell–matrix interactions that can drive cell maturation as these data are critical for scale-up to larger applications such as transplantation.

The different populations of astrocytes observed on 2D versus 3D culture could have resulted from differential rates of survival or proliferation between the morphological groups. We did observe a 6% difference in cell survival, with more dead cells being counted in 3D. This difference may be due to an underestimate of cell death in 2D as many cells lift from the substrate and are washed away in the media. A similar apparent increase in cell death was observed for rat astrocytes in 3D.⁹⁵ However, we do acknowledge that dead trapped cells may degrade over time, and the estimates of cell death in 3D may also be underestimated.

To address the issue of altered proliferation, we performed EdU incorporation assays (Fig. 4). Independent of dimensionality, round cells constituted the majority of proliferating cells, followed by bipolar cells, with negligible numbers of stellate cells dividing in culture. Yet, the 3D astrocyte cultures had fewer EdU⁺ cells (8–13%), similar to that observed in healthy cortex (9%).² On the contrary, 2D astrocyte cultures had more EdU⁺ cells (19%) with higher proliferation similar to that observed in an injured cortex (20%) or suggesting an earlier maturation phase of the astrocytes that is observed during the first postnatal weeks.^98,99 Our proliferation results corroborate previous genomic studies that suggest that astrocytes isolated by the same methods³⁹ and cultured on 2D substrates are highly proliferative compared with healthy mature astrocytes and may represent reactive astroglial cells.⁴⁰ Furthermore, previous studies suggest that astrocytes proliferate faster in injured versus healthy adult brain,^100,101 and it is possible that the astrocytes sense the 3D environment as more akin to in vivo and proceed along a maturation pathway congruent with their biological age rather than continuing proliferation.

We note that while there was a marked increase in the populations of stellate and perivascular astrocytes in 3D culture, small round GFAP⁺ cells are yet the predominate cell morphology. Previous literature from other cell types have also reported that cells cultured within 3D are smaller in apparent diameter than those cultured on 2D surfaces.^92,102 Furthermore, we speculate that the round phenotype of the majority of postnatal astrocytes in 3D is possibly because of lack of other essential growth factors that would otherwise allow them to transform into their mature form. This hypothesis is supported by the stable fraction of stellate astrocytes after 4 days of culture in 3D. Furthermore, in vivo, various growth factors, such as leukemia inhibitory factor and ciliary neurotrophic factor, are secreted by endothelial cells and early differentiated neurons and are known to promote astrocyte maturation.^{11,22,103,104} Previous tissue engineering constructs have not evaluated the progression of glial maturation and therefore our study provides the first characterizations of the potential of 3D substrates to direct glial progenitors along specific cell lineages.

We then asked whether the morphological heterogeneity observed in culture corresponds to the in vivo astrocyte phenotypes that exist during development and in the adult. Recently human astrocytes were observed to have differential expression of GFAP and a range of shapes.¹⁰⁵ The relative expression of glial markers by astrocytes changes during development, varies between areas within the brain, and is influenced by cues in the extracellular environment.^7,34,61 Round astrocytes lacked a corresponding in vivo-like morphology, but expressed GFAP and S100β, which are markers for more mature astrocytic populations (Figs. 6 and 7). This result reinforces our hypothesis that additional factors may be required for the elaboration of a mature resting-state phenotype.

Radial glial cells are progenitors that can transform into neurons or astrocytes, depending on the stage of corticogenesis.^106,107 In vivo, astrocytes mature about 2 weeks after birth,¹⁰⁸ while radial glial cells that were present in the developing embryo disappear during this time.¹⁰⁹ In fact, after birth, the glial cells in the rodent brain expand six- to eightfold, with local sources, presumably radial glia, providing the initial glial pool.^110,111 During astrogliogenesis in vivo, radial glial cells progressively lose nestin and RC2 immunoreactivities and acquire a more ramified appearance and a stronger GFAP immunostaining.^112,113 Bipolar GFAP⁺ cells present in 3D culture appear to be radial glial cells as characterized by morphology (Fig. 5C) and expression of both RC2 and nestin (Fig. 7).^51,71 We observed that in 3D culture, with an increase in culture time from 4 to 10 days, there was a reduction in the percentage of bipolar RC2⁺ cells and an increase in stellate and perivascular astrocytes that do not express RC2 (Fig. 5B). Furthermore, the stellate and perivascular cells also do not express nestin, indicating that these GFAP⁺ astrocytes have lost their progenitor potential and acquired a more mature developmental stage.^74,114 It is noteworthy that the bipolar astrocytes express S100β in 2D culture, but not in 3D culture. The molecule, S100β, is generally not expressed by radial glia in vivo.¹¹² Thus, the abnormal expression of S100β by radial glial cells could possibly be attributed to a stress response imposed by the artificial nature of 2D culture.⁹³

In summary, we report that a 3D culture environment can sustain the morphology and heterogeneity of astrocytes observed in vivo. These findings suggest new ways of studying astrocyte development, behavior, and function in vitro. These studies also have significance in culturing populations of radial glial as well as mature nonreactive astrocytes in hydrogels for use in transplantation. Our ongoing work focuses on developing strategies to shift the astrocyte population toward specific phenotypes (e.g., radial glial progenitor cells) and defining the signaling mechanisms responsible for differences in astrocyte morphology observed in 2D versus 3D environments. By tailoring in vitro systems along specific trajectories, we can devise strategies to generate targeted cell populations from patient-derived progenitor or stem cells and also explore new mechanisms to altering in vivo milieu away from injury outcomes back to normal states and function.

Footnotes

Acknowledgments

The authors thank C. Petty for assistance with confocal microscopy and Dr. J. Loehe and Dr. C. Rakes for advice on statistical analysis. This work was supported by NIH-NINDS R01NS065205 (JBL and EMP) and a UMBC Undergraduate Research Award (JAP).

Disclosure Statement

The authors have no conflicts of interest to disclose.

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