FGF2-induced effects on transcriptome associated with regeneration competence in adult human fibroblasts
© Kashpur et al.; licensee BioMed Central Ltd. 2013
Received: 20 March 2013
Accepted: 24 September 2013
Published: 26 September 2013
Adult human fibroblasts grown in low oxygen and with FGF2 supplementation have the capacity to tip the healing outcome of skeletal muscle injury – by favoring regeneration response in vivo over scar formation. Here, we compare the transcriptomes of control adult human dermal fibroblasts and induced regeneration-competent (iRC) fibroblasts to identify transcriptional changes that may be related to their regeneration competence.
We identified a unique gene-expression profile that characterizes FGF2-induced iRC fibroblast phenotype. Significantly differentially expressed genes due to FGF2 treatment were identified and analyzed to determine overrepresented Gene Ontology terms. Genes belonging to extracellular matrix components, adhesion molecules, matrix remodelling, cytoskeleton, and cytokines were determined to be affected by FGF2 treatment.
Transcriptome analysis comparing control adult human fibroblasts with FGF2-treated fibroblasts identified functional groups of genes that reflect transcriptional changes potentially contributing to their regeneration competence. This comparative transcriptome analysis should contribute new insights into genes that characterize cells with greater regenerative potential.
KeywordsTranscriptome Human fibroblasts Fibroblast growth factor (FGF2) Wound healing Regeneration
During development, distinct cell phenotype differentiation is guided by finely tuned and orchestrated changes in transcriptional activity of specific groups of genes that become gradually activated (lineage-specific), gradually repressed (stem cell and progenitor cell genes), or whose activity does not change substantially (housekeeping genes). Ultimately, analyzing the transcriptome of a cell type offers an opportunity to broadly identify transcripts that define it. In addition to these either developmentally regulated or artificially induced phenotype changes that are accompanied by distinct transcriptional changes, a transcriptome of any given cell type can vary substantially depending on cell cycle [1–3], passage number, and environmental factors such as oxygen concentration , temperature, and presence of serum .
Another important factor that causes transcriptional changes and is crucial for maintaining a cell phenotype is growth substrate. For example, maintenance of undifferentiated state of embryonic stem cells is dependent on favorable substrate, composed of laminin [6–9], vitronectin [9–12], fibronectin , and collagen IV . In addition to chemical composition, physical properties of substrate also determine cell fate. Roughness and stiffness of the surfaces have also been shown to affect developmental plasticity of cells. Smooth and rigid glass surface supports undifferentiated phenotype, while rough and soft substrates promote differentiation [13, 14].
Lastly, presence of various growth factors in culture media can have a significant effect on a cell transcriptional activity and consequently its phenotype. FGF2 is a mesenchyme-derived growth factor that displays mitogenic, migratory, and morphogenic functions and is also known to play role in angiogenesis, organ development, organ regeneration, and wound healing . Contrary to its predominantly mitogenic effects on differentiated cell types, FGF2 is absolutely required for maintenance of expression of stemness-related genes. With respect to wound healing, FGF2 has been studied as a potential therapeutic anti-scarring agent [15–17].
We have previously investigated the effects of the aforementioned important cell culture conditions, FGF2 and culture surface, on adult human fibroblasts. We have observed that adult human fibroblasts demonstrated FGF2- and surface-mediated induction of some endogenous stem cell genes and a capacity to acquire a more developmentally plastic phenotype. This low level of activation of stem cell genes was not sufficient for induction of a phenotypic conversion into a pluripotent cell phenotype . However, when transplanted into skeletal muscle injury, adult human fibroblasts grown in low oxygen and with supplementation of FGF2 had the capacity to tip the healing outcome of skeletal muscle injury – by favoring regeneration response in vivo over scar formation . The wound repair process consists of several phases, including immediate response to injury, inflammatory response, cell proliferation and migration, ECM contraction, and ECM remodeling. The roles of dermal fibroblasts in wound healing have been described  and in mammals fibroblasts facilitate collagen deposition and formation of a scar. The cascade of molecular events leading to scar formation involves increased proliferation and migration of fibroblasts in response to growth factors , production and organization of specific ECM components [22, 23], and acquisition of an actin-dependent contractile phenotype . The wound repair process is complete by formation of a scar (disorganized extracellular matrix, mainly collagen) .
In this study, we compared transcriptomes of control fibroblasts and regeneration- competent fibroblasts to determine whether transcriptional profile that characterizes regeneration-competent cells reflects disregulation of genes involved in the default wound healing pathway leading to scar formation – turning the cells into a more pro-regenerative phenotype.
The effect of cell growth surface and FGF2 on fibroblast transcriptome
To obtain a sense of the effects of surface and FGF2 treatment on global transcription, two independent samples (in three technical replicates each) of human dermal fibroblasts grown on glass, glass with FGF2, plastic, and plastic with FGF2 were hybridized to the Human Whole Genome OneArray® microarray, which contains 29,187 human oligonucleotide probes. Background-corrected intensity data was normalized and filtered, which identified 11,124 probes of detectable level of intensity (Additional file 1). The gene expression dataset is of excellent quality as indicated by Pearson’s correlation coefficients for biological replicates: 0.987 for glass, 0.973 for glass with FGF2, 0.960 for plastic, and 0.971 for plastic with FGF2 (Additional file 2). To investigate cell culture effects, we examined significantly differentially expressed gene probes using moderated t-statistic and based on the false discovery rate (FDR) cutoff value of 0.05. Comparison of transcriptomes between cells grown on glass and plastic in the absence of FGF2 did not identify any differentially expressed genes. However, FGF2-induced changes in gene expression depended on surface.
Gene ontology analysis
Expression of genes associated with wound healing
As FGF2-treated human dermal fibroblasts were previously shown to participate in wound healing of volumetric skeletal muscle by contributing directly to the pool of satellite PAX7 positive cells and by stimulating regeneration of endogenous skeletal muscle tissue , we focused further analysis of differentially expressed genes to those that play a role in wound healing and could be uniquely identifying regeneration-competent fibroblasts.
Overall, select genes belonging to extracellular matrix and its remodeling, inflammation, cytoskeleton and migration, and growth factor signaling were found to be affected by FGF2.
Extracellular matrix, matrix remodeling enzymes, and adhesion molecules
ECM, adhesion, and matrix remodeling genes affected by FGF2 treatment
Log2 fold change
Collagen, type XXI, alpha 1
Collagen, type XIV, alpha 1
Collagen, type XIII, alpha 1
Collagen, type XVIII, alpha 1
Collagen, type VI, alpha 3
Collagen, type X, alpha 1
Collagen, type XXVII, alpha 1
Collagen, type XVI, alpha 1
Collagen, type I, alpha 2
Collagen, type XII, alpha 1
Collagen, type V, alpha 1
Collagen, type I, alpha 1
Collagen, type XV, alpha 1
Collagen, type VIII, alpha 1
Collagen, type V, alpha 2
Collagen, type V, alpha 3
Collagen, type IV, alpha 4
Collagen, type IV, alpha 2
Collagen, type XI, alpha 1
Collagen, type IV, alpha 1
Laminin, alpha 5
Laminin, beta 1
Laminin, alpha 4
Laminin, alpha 3
Laminin, gamma 2
Laminin, alpha 2
Laminin, beta 2 (laminin S)
Laminin, gamma 1 (formerly LAMB2)
Fibronectin type III domain containing 4
Fibronectin type III domain containing 3A
Fibronectin type III domain containing 3B
Fibronectin type III domain containing 1
Integrin, alpha 2 (CD49B, alpha 2 subunit of VLA-2 receptor)
Integrin, alpha 10
Integrin, beta 3 (platelet glycoprotein IIIa, antigen CD61)
Integrin, beta 1 (fibronectin receptor, beta polypeptide, antigen CD29 includes MDF2, MSK12)
Integrin, beta-like 1 (with EGF-like repeat domains)
Integrin, beta 2 (complement component 3 receptor 3 and 4 subunit)
Cadherin-related family member 3
Protocadherin gamma subfamily C, 3
Cadherin 11, type 2, OB-cadherin (osteoblast)
Protocadherin beta 2
Cadherin 2, type 1, N-cadherin (neuronal)
Matrix metallopeptidase 1 (interstitial collagenase)
ADAM metallopeptidase with thrombospondin type 1 motif, 8
Matrix metallopeptidase 27
Matrix metallopeptidase 10 (stromelysin 2)
Matrix metallopeptidase 3 (stromelysin 1, progelatinase)
TIMP metallopeptidase inhibitor 4
ADAM metallopeptidase domain 15
Matrix metallopeptidase 11 (stromelysin 3)
ADAM metallopeptidase domain 19
TIMP metallopeptidase inhibitor 3
ADAM metallopeptidase domain 12
ADAM metallopeptidase with thrombospondin type 1 motif, 1
ADAM metallopeptidase with thrombospondin type 1 motif, 5
Cytoskeleton genes regulated by FGF2 treatment
Log2 fold change
Tubulin, alpha 4a
Tubulin, beta 3 class III
Tubulin, alpha 1c
Tubulin, beta 2c
Actin, alpha 2, smooth muscle, aorta
Tubulin, epsilon 1
Tubulin, gamma 2
Actin, alpha, cardiac muscle 1
Actin, gamma 2, smooth muscle, enteric
Cytokines, their receptors, and downstream signaling molecules
Representative cytokines regulated by FGF2
Log2 fold change
Chemokine (C-X-C motif) ligand 5
Chemokine (C-X-C motif) ligand 6 (granulocyte chemotactic protein 2)
Chemokine (C-X-C motif) ligand 1 (melanoma growth stimulating activity, alpha)
Chemokine (C-C motif) ligand 22
Complement component 5
Chemokine (C-C motif) ligand 26
Chemokine (C-C motif) ligand 14
Chemokine (C-C motif) ligand 25
Chemokine (C-C motif) ligand 2
Chemokine (C-C motif) receptor-like 1
Chemokine (C-C motif) receptor 10
Chemokine (C-C motif) receptor 8
Chemokine (C-X-C motif) receptor 7
Interleukin 1 receptor antagonist
Interleukin 1, beta
Interleukin 1 receptor accessory protein
Interleukin 6 (interferon, beta 2)
Interleukin 17 receptor D
Interleukin 13 receptor, alpha 2
Interleukin 15 receptor, alpha
Interleukin 21 receptor
Interleukin 20 receptor beta
Interleukin 1 receptor-like 1
Signal transducer and activator of transcription 4
Signal transducer and activator of transcription 1
Signal transducer and activator of transcription 3 (acute-phase response factor)
Tumor necrosis factor family
Tumor necrosis factor, alpha-induced protein 8-like 1
Tumor necrosis factor receptor superfamily, member 25
Tumor necrosis factor (ligand) superfamily, member 10
Tumor necrosis factor, alpha-induced protein 8-like 3
Tumor necrosis factor receptor superfamily, member 1B
Tumor necrosis factor receptor superfamily, member 21
C1q and tumor necrosis factor related protein 6
Tumor necrosis factor receptor superfamily, member 10b
C1q and tumor necrosis factor related protein 3
Tumor necrosis factor, alpha-induced protein 6
Tumor necrosis factor, alpha-induced protein 1 (endothelial)
Tumor necrosis factor receptor superfamily, member 10d, decoy with truncated death domain
Tumor necrosis factor receptor superfamily, member 11b
Membrane frizzled-related protein, C1q and tumor necrosis factor related protein 5 transcription unit
Tumor necrosis factor (ligand) superfamily, member 4
Transforming growth factor, beta receptor 3
Transforming growth factor, beta-induced, 68kDa
Transforming growth factor, beta receptor 1
The comparative transcriptome analysis described here demonstrates a unique molecular signature for induced regeneration-competent (iRC) fibroblasts compared with control fibroblasts. Consistent with the notion that these two cell types are distinctly different, we have used both cell types in in vivo regeneration experiments and demonstrated that the induced regeneration-competent fibroblasts participate in regenerative response of skeletal muscle (concomitant with decreased scar formation), contribute to the pool of newly established satellite cells (PAX7+ cells) in a mouse injury model, as well as form mature myotubes .
Identification of significantly differentially expressed genes and subsequent Gene Ontology analysis determined that a large number of genes important for the outcome of wound healing such as extracellular matrix genes, adhesion molecules, matrix remodeling genes, and genes involved in inflammation were regulated by FGF2 (Figure 3).
During dermal wound healing, fibroblasts are responsible for ECM production  and, here, we show that FGF2 treatment affects a number of genes involved in production and remodeling of ECM. FGF2 caused downregulation of a number of collagens such as collagen IV, collagen XI, collagen V, and collagen I, as well as caused upregulation of collagen XXI and collagen XIV (Table 1). qRT-PCR analysis confirmed downregulation of COL1A1, COL4A1, COL4A2, COL4A4, COL8A1, and COL11A1 (Figure 4B). FGF2 was previously shown to downregulate expression of interstitial collagen I and III . Collagen I is a major component of ECM in skin, and during wound healing is the main scar forming collagen. Collagen IV is a major constituent of basement membrane (other components include laminin, nidogen, and heparan sulfate proteoglycan perlecan) and is a predominant type of collagen found in skeletal muscle. Other ECM genes affected by FGF2 treatment included laminins and fibronectins (Table 1). Most profoundly affected by FGF2 treatment were laminin gamma 1 (LAMC1) and laminin alpha 5 (LAMA5). qRT-PCR confirmed increased expression levels of these two laminins (Figure 4B). Fibronectin 1 was downregulated by FGF2 treatment (Figure 4B). FGF2 treatment of human fibroblasts modulates production of the ECM. The ECM composition of the FGF2-treated fibroblasts favors the pro-regenerative outcome in the wound site directly by affecting the balance between scar formation and tissue regeneration and potentially thorough changes in cell attachment to ECM, cell migration, and cell proliferation.
Cell attachment to the ECM is regulated through integrins, heterodimers that recognize specific substrates. Adhesion and migration on collagen substrate is performed through α1β1 and α2β1 and formation of collagen type I and type III network is dependent on fibronectin and α2β1 [25–27]. We show FGF2-induced upregulation of β1 and α2 (Figure 4B). Integrins α5β1, αVβ3, and α4β1 pairs are utilized to bind fibronectin matrix [28, 29], αVβ5 is used to adhere to vitronectin, and α6β1, α2β1, α3β1 to adhere to laminin and entactin [10, 12, 30]. FGF2 treatment downregulated ITGB2 and upregulated ITGB3 and ITGA10 (Figure 4B). Integrins connect ECM to actin cytoskeleton via focal adhesions rich in talin, which is recruited to F-actin, and binds integrin pairs, which in turn leads to transmission of F-actin movements to ECM . Change in the composition of integrins, as well as in the components of focal adhesions leads to change in migration, as well as preferential binding to specific substrate, production of which is regulated by FGF2 treatment, and may benefit a pro-regenerative response.
During wound healing, fibroblasts acquire a highly migratory phenotype. The process is driven by actin polymerization and resulting microfilaments of the cell’s leading edge link to ECM via integrins. Actomyosin contraction then allows for the disassembly of adhesions in the rear and movement forward . Thus, movement of the fibroblasts in the wound site is regulated not only by the ECM and adhesion molecules, but also by the actin cytoskeleton. Actin cytoskeleton is also involved in fibroblast contractile phenotype. During dermis healing, fibroblasts generate stress fibers (weakly contractile actin bundles) to enable contraction . Fibroblasts’ shape is regulated by the environment and cell-matrix adhesion determines the cell shape, such as strong cell-ECM adhesion promotes spindle-shaped fibroblast . In vitro fibroblasts were shown to have different morphology depending on the substrate they are grown on; in 3D cultures resembling an in vivo environment, fibroblasts display elongated shape, well-developed actin cortex, and filopodia at the leading edge . Alpha actin ACTC1, which is a constituent of the contractile apparatus, was downregulated in human dermal fibroblasts treated with FGF2 (Table 2; Figure 5B). Gamma actin ACTG2, which is involved in cellular motility and adhesion, was 64-fold downregulated (Table 2), though qRT-PCR did not confirm its expression. By regulating cytoskeleton gene expression, FGF2 potentially promotes cell migration in the wound site, and reduces contraction that leads to the favorable pro-regenerative outcome.
Previously, it was shown that administration of FGF2 alone into a dermal wound shows reduced scar formation , which can be attributed to upregulation of matrix metalloproteinase MMP1 . Our data shows strong upregulation of MMP1 (Figure 4B), the metalloproteinase responsible for cleaving collagen type I, II, and III . FGF2 signaling was shown to activate the MMP1 promoter . MMP1 was able to improve the skeletal muscle regeneration process by reducing scar tissue formation [36–38] and by promoting migration of myoblasts involved in regeneration of skeletal muscle [39, 40]. Interestingly, integrin α2β1 was shown to increase MMP1 expression [41, 42]. By transplanting FGF2 treated human dermal fibroblasts, continuous increase in production of MMP1 among other factors, may be allowed, indicating that MMP1 is present not only at the time of the resolution phase of wound healing leading to decreased collagen production, but also at earlier stages of wound healing, for example during the inflammation stage. Other MMP molecules, such as stromelysins MMP3, MMP10, MMP11, were upregulated as well (Table 1 and Figure 4). MMP3 was previously shown to be responsible for contraction of fibroblasts during wound healing  and was regulated by FGF2 in a mouse model . MMPs, mostly MMP2, 3, 9 and 10, are highly upregulated during amphibian limb regeneration [45–47]. All of these observations point toward a favorable role of MMPs in the regeneration process. Thus, FGF2-stimulated change in transcriptional profile of various MMPs is an important factor contributing to the regeneration-competence of fibroblasts.
FGF2 treatment also led to a favorable ratio between MMPs and tissue inhibitors of metalloproteinases (TIMPs), as an imbalance between MMPs and TIMPs has been shown to increase scar formation. FGF2 upregulated TIMP4 and downregulated TIMP3 expression (Figure 4B). ADAM and ADAMTS proteinases that were shown to be differentially regulated by FGF2 (Table 1) are regulators of ECM and adhesion molecules and affect cell motility, adhesion, and signaling during wound healing processes. ADAMTS1 and ADAMTS5 were downregulated by FGF2 treatment (Figure 4B). ADAM transmembrane proteinases are involved in cleaving and activating various cell surface molecules, whereas ADAMTS are secreted proteinases that can bind ECM. ADMATS8 that was upregulated by FGF2 treatment (Figure 4B) has anti-angiogenic properties .
The ratio of TGFB1/TGFB3 is a factor that predicts scar formation, the decrease in this ratio being indicative of reduced scar formation . Fetal wounds that are known to heal without scar formation exhibit decreased TGFB1 levels . Administration of TGFB3 has also been shown to reduce scar formation . TGFB pathway was previously shown to be induced by FGF2 treatment in mouse embryonic fibroblasts (MEFs) . We observed no change in the levels of TGFB1 due to FGF2 treatment by microarray analysis whereas qRT-PCR showed downregulation of TGFB1 levels (Figure 5B). We observed upregulation of TGFBR3 due to FGF2 treatment by the array, but qRT-PCR showed no change in expression levels (Figure 5B). qRT-PCR confirmed downregulation of TGFBR1 (Figure 5B). These observations may be due to differences between mouse embryonic fibroblasts and adult human dermal fibroblasts, indicating that FGF2 response in these cells may be unique.
Decreasing inflammation has been shown to decrease scar formation. For example, when wounds of skin and oral mucosa were compared, there was less inflammation and scarring in oral mucosa . Non-scar wound healing in fetal wounds is also characterized by absence of inflammation [52–56]. Inflammatory events are integrated by chemokines. Chemokines are chemotactic cytokines that regulate migration of cells during inflammatory process. ELR(+) CXC chemokines are neutrophil attractants and activators. CXCL6 or granulocyte chemotactic protein-2 (GCP-2) is a ELR(+) CXC chemokine. FGF2 treatment led to increase in CXCL6 chemokine expression (Figure 5B). CXCL5, a chemokine that attracts and activates neutrophils, amplifies inflammatory cascade, and stimulates local production of cytokines was shown to be upregulated by FGF2 treatment (Figure 5B). Interestingly, when CXCL5 is cleaved by MMP1, 2, 8, 9, and 13, increased inflammation is observed and cell recruitment to the wound site is activated . CCL2 (monocyte chemoattractant protein-1, MCP-1), which is involved in inflammatory cell recruitment, can be induced through focal adhesion kinase (FAK) leading to inflammation and scar production in a cutaneous injury, and CCL2 knock-out mice showed decreased scarring . Here, we observed downregulation of CCL2 due to FGF2 treatment (Figure 5B). In agreement with previous publications, implantation of FGF2 treated fibroblasts, which show CCL2 downregulation, into a mouse wound sight leads to reduced scar formation . We also show in this transcriptome analysis that IL6/STAT3 signaling pathway is regulated by FGF2 (Figure 5B). Interleukin 6 (IL6) is a pleiotropic cytokine that is produced by a variety of cells such as epidermal cells, endothelial cells, and fibroblasts . IL6 is known to increase production of collagen , thus the decrease in collagen synthesis that we observe in skeletal muscle injury, can be partially explained by decrease in IL6. CCL2 was shown to induce IL6 secretion in human lung fibroblasts, and has a role in regulating fibrosis  and was shown previously to be regulated by FGF2 . Scarless, fetal wounds are characterized by diminished expression of pro-inflammatory IL6 and IL8 [52, 53]. Here, we show that FGF2 treatment significantly reduces IL6 levels (Figure 5B), whereas levels of IL8 are upregulated with FGF2 treatment (Table 3). FGF2-induced decrease in IL6 level could be contributing to pro-regenerative phenotype of adult human fibroblasts. Signal transducer and activator of transcription (STAT3) conveys signals from IL6. Loss of IL6 was shown to result in deficiency of proliferation and migration of myoblasts [63–65]. IL6/STAT3 was shown recently to be involved in excessive ECM production and increased cellular proliferation in hypertrophic scars compared to normal human fibroblasts .
Comparison of transcriptomes between control and regeneration-competent fibroblasts indicates significant differences in expression of genes involved in several biological processes during wound healing. Downregulation of collagens, upregulation of ECM remodeling enzymes, and downregulation of pro-inflammatory cytokines may be in part responsible for the cells’ pro-regenerative phenotype. A choice between scar-forming and pro-regenerative wound healing responses may depend on a balance between ECM production, degradation, consequent ECM contractility, and decreased inflammatory response. Further studies are needed to elucidate functional significance of specific disregulated genes.
Adult human dermal fibroblasts were obtained from ATCC (CRL-2352) at passage number 1 (p1). Cells were expanded using culture conditions recommended by the supplier, namely ambient oxygen, 5% CO2 in air, 37°C in DMEM/F12 and 10% FBS. Expansion was done by trypsinizing (0.05% trypsin, Cellgro) the cells at 80% confluence and replating them at a density of 14,000 cells/cm2. Cells were cryopreserved with DMSO and the same passage used for all the experimental groups. Cells from the same passage number 7 were grown for seven days at 5% O2, 5% CO2, 37°C in DMEM/F12 and 10% FCIII in one of the following culture conditions: 1. with 4 ng/ml human recombinant FGF2 (PeproTech) on tissue culture plastic; 2. with 4 ng/ml human recombinant FGF2 on glass culture surface; 3. on tissue culture plastic; and 4. on glass culture surface. After 7 days, cells were used for three RNA collections for transcriptome arrays and qRT-PCR.
Total RNA was isolated from all treatment groups using TRIZOL reagent (Invitrogen) following manufacturer’s protocol.
OneArray microarray sample and data processing
To obtain a sense of global effects of surface and FGF2, two independent samples (in three technical replicates each) of cells grown on glass, glass with FGF2, plastic, and plastic with FGF2 were hybridized to the Human Whole Genome OneArray® v5 (Phalanx Biotech, Palo Alto, CA). RNA quality and integrity were determined utilizing an Agilent 2100 Bioanalyzer (Agilent Technologies, Palo Alto, CA, USA) and absorbance at A260/A280. Only high quality RNA, having a RIN of >7.0, and an A260/280 absorbance ratio of >1.8, was utilized for further experimentation. RNA was converted to double-stranded cDNA and amplified using in vitro transcription that included amino-allyl UTP, and the aRNA product was subsequently conjugated with Cy5™ NHS ester (GEH Lifesciences). Fragmented aRNA was hybridized at 50°C overnight using the HybBag mixing system with 1X OneArray Hybridization Buffer (Phalanx Biotech), 0.01 mg/ml sheared salmon sperm DNA (Promega, Madison, WI, USA), at a concentration of 0.025 mg/ml labeled target. After hybridization, the arrays were washed according to the OneArray protocol. Raw intensity signals for each microarray were captured using a Molecular Dynamics™ Axon 4100A scanner, measured using GenePixPro™ Software, and stored in GPR format.
The data was analyzed with R/bioconductor using standard statistical functions and analysis modules for the ANOVA, T test, FDR, and functional analysis [67, 68]. Analysis was performed in the following order. First, data was background corrected, normalized, and filtered to remove probes with very low expression or low variance (expression but no variation) across conditions. Next, 2-way ANOVA was performed to determine significant gene probes for the two factors and possible interactions between cell culture surface and FGF2. LIMMA package was used to determine significantly differentially expressed genes (DEG) with moderate t-statistic as main statistic of significance and standard errors moderated using Bayesian model [69–71]. P-values were adjusted for multiple comparisons using Benjamini and Hochberg method to control the false discovery rate (FDR) . FDR cutoff value of 0.05 was used.
Gene Ontology (GO) analysis was performed to analyze functional enrichment within DEG due to FGF2 treatment in human dermal fibroblasts cultured on plastic. DEG due to FGF2 treatment were profiled for GO slim using geneListPie package . In order to perform GO analysis, GOstats package was used . Hypergeometric conditional testing was performed to obtain overrepresented GO terms that belong to three groups: biological process, molecular function, and cellular component.
cDNA was prepared from total RNA using QuantiTect Reverse Transcription kit (Qiagen) using mixture of oligo-dT and random primers method. The kit also includes elimination of genomic DNA step prior to reverse transcription. 1 μg of total RNA was used for cDNA preparation. For each qPCR reaction 20 ng of cDNA were used. qPCR was performed using SYBR SELECT master mix (Invitrogen). The list of primers can be found in Additional file 7. Quantification of qPCR results was performed by the ΔΔCT method.
Availability of supporting data
The data sets supporting the results of this article are available in Gene Expression Omnibus (GEO) repository (GSE48967) and at http://users.wpi.edu/~tdominko/iRC_transcriptome/.
This work was supported by the grant from the NIH (#R01GM85456) to Tanja Dominko.
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