In order to identify reliable markers of corneal epithelial stem cells, we employed an inducible transgenic “pulse-chase” murine model (K5Tta × TRE-H2BGFP) to localize, purify, and characterize slow cycling cells in the cornea. The retention of GFP labeling in slowly dividing cells allowed for localization of these cells to the corneal limbus and their subsequent purification by FACS. Transcriptome analysis from slow cycling cells identified differentially expressed genes when comparing to GFP- faster-dividing cells. RNA-Seq data from corneal epithelium were compared to epidermal hair follicle stem cell RNA-Seq to identify genes representing common putative stem cell markers or determinants, which included Sox9, Fzd7, Actn1, Anxa3 and Krt17. Overlapping retention of GFP and immunohistochemical expression of Krt15, ΔNp63, Sox9, Actn1, Fzd7 and Krt17 were observed in our transgenic model. Our analysis presents an array of novel genes as putative corneal stem cell markers.
Loss of the regenerative capacity of the ocular surface through the absence of corneal epithelial stem cells is a potentially blinding condition. Lack of definitive molecular markers to reproducibility locate, purify and expand corneal epithelial stem cells has hampered the ability to understand their biology and to use these cells for therapeutic transplantation.
Stem cells from the cornea reside between the corneal periphery and the conjunctiva, known as the limbus. Limbal stem cells (LSCs) are clonogenic, regenerating new tissue in vivo and in vitro1 exhibiting slow cycling phenotypic characteristics2. Classically, these cells have been characterized by the ability to retain tritiated thymidine or bromodeoxyurdine (BrdU) for long periods, yet have high proliferative potential3,4,5,6,7. More recently, a transgenic system that can genetically label slow cycling cells with GFP has been used to identify label retaining cells (LRCs) in skin8,9, sweat glands10, salivary glands11 and the cornea12. In this model, one parental strain harbors the H2B-GFP transgene under the control of a tetracycline (doxycycline; dox) regulatory element (TRE), creating a tet-off system. The second strain expresses a transcription factor regulated by tetracycline (tTA) under the control of a cell-type-specific Keratin 5 (K5) promoter. Thus, K5 expressing cells will have nuclear GFP labeling in the “pulse” period, which is then turned off with dox administration, beginning the “chase” period.
This approach allowed for the purification of cells and their subsequent molecular characterization of LRCs using next generation sequencing (NGS), yielding genes marking (and in some cases determining) “stemness”. Thus, the molecular markers are identified without a pre-conceived notion as to which genes may be related to stemness. Comparison of these data from corneal epithelium with prior similar characterization of hair follicle stem cells (HFSCs)13 were performed to identify common stem cell markers in these developmentally related tissues.
All animal experiments were approved by the Institutional Animal Care and Use Committee (IACUC) from Weill Cornell Medical College, in accordance with the US National Institutes of Heath Guide for the Care and Use of Laboratory Animals and guidelines of the Association for Research in Vision and Ophthalmology Statement for the use of Animals in Ophthalmic and Vision Research. Wildtype (WT) CD1 mice were obtained from Jackson Laboratories (Bar Harbor, ME). The double transgenic mice were obtained by crossing heterozygous K5Tta (FVB) × TRE-H2BGFP (CD1) from E. Fuchs laboratory at the Rockefeller University8.
Wholemount Corneal Imaging and K5Tta × TRE-H2BGFP Slit lamp Imaging
In our double transgenic K5Tta × TRE-H2BGFP+ mouse model, nuclear GFP label is diluted in fast-dividing differentiated cells following administration of 2 g/Kg (Bio-Serv, Flemington, NJ, USA) dox in the mouse chow from 21 days (d) of age. In slow cycling cells (a characteristic of stem cells) GFP is retained allowing the tracing of these cells in the adult cornea. GFP+ mice corneas (n = 49) were examined under the slit lamp microscope at eye-lid opening stage and followed to adult hood (>6–8 weeks old) to ensure only mice with normal clear corneas were selected for our study. K5Tta × TRE-H2BGFP− mice were also examined as controls (n = 20). Mice were administered dox at 21d old and sacrificed after 0, 10, 28, 53 & 91 d chase by CO2 asphyxiation. A subset of mice with ocular abnormalities (n = 22) exhibiting signs of neovascularization and conjunctivalization as a result of the genetic cross were sacrificed after 35, 42 and 49 d chase. Eyes were enucleated and the expression of GFP in corneal flatmounts was analyzed using a Zeiss Axiovision Observer fluorescence microscope.
Corneal Epithelial Cell Isolation and Fluorescence Activated Cell Sorting (FACS)
The corneal epithelia from adult K5Tta × TRE-H2BGFP mice (with prior slit lamp screening for clear corneas) chased as described above at 28, 42 and 91 d were separated from the stroma by incubating entire globes at 4 °C overnight in CnT50 media (CELLnTEC, Bern, Switzerland) containing 12.6 units dispase (Roche Diagnostics, Basel, Switzerland) and 100 mM D-sorbitol (Sigma Aldrich, St. Louis, MO). The detached epithelial sheets were collected and incubated with 0.05% trypsin/0.03% EDTA (Life Technologies, NY) at 37 °C for 10 mins to isolate single cells using a spatula to detach corneal epithelium from the underlying corneal stroma. Enzymatic reactions stopped by adding media supplemented with fetal calf serum (FCS) (Sigma-Aldrich, St. Louis, MO) and washed by centrifuging several times. Cells were then washed with PBS twice and suspended in 1 ml of DAPI solution and strained through a 70 μm cell strainer. GFP+ and GFP− cell populations were sorted using a FACSAria II (BD Biosciences, San Jose, CA) directly into tubes containing RNA lysis buffer (Qiagen, GmbH, Hilden, Germany) with 2-mercaptoethanol. 6–10 globes were used for each FACS procedure from clear and normal corneas at 28, 42 and 91 d chase and 14 globes for the abnormal corneas at 84 d chase.
Total RNA from FACS cells (GFP+ and GFP− cell populations) was extracted using Qiagen RNeasy Plus Mini Kit (Qiagen, GmbH, Hilden, Germany), and RNA integrity and quantity were recorded using Agilent Technologies 2100 Bioanalyzer and Nanodrop Spectrophotometer at the Genomics Resources Core Facility of Weill Cornell Medical College.
Next generation sequencing library preparation and Illumina sequencing
Total RNA from GFP− and GFP+ corneal epithelial cells (minimum concentration of 100 ng) was provided to the Genomics Core Facility at Weill Cornell Medical College to create cDNA libraries (Illumina, San Diego, CA). Samples were multiplexed with 3 samples per lane and loaded onto flow cell lanes. Sequencing-by-synthesis of 58-nucleotide length, single-end reads were performed on Illumina Hiseq 2000/1000 sequencing system.
Comparative RNA-Seq analysis from corneal epithelial GFP+ LRCs (slow cycling labeling retaining cells) and GFP− (fast-dividing cells) from 28, 42, 84 and 91 days chase
Comparative analysis from clear corneas at 28, 42 and 91 d chase reads were aligned to the mm9 mouse transcripts using STAR (version 2.3.0e)14. Then HTSeq15 was applied to obtain gene counts, and multi-mapping reads were discarded according to suggested HTSeq practice. A total of 12597 genes were used for subsequent analysis after filtering genes with less than 20 average read counts of all samples. Gene count data was rescaled using DESeq2 (version 1.2.10) R package16. Samples were separated into “GFP+” and “GFP−” groups for each chase period, and then differentially expressed genes (DEG) were detected between the groups with a false discovery rate (FDR) < 0.05 and >2 fold change by using DESeq2. Venn diagrams summarizing the overlap of DEG among different chase periods were generated in R. Gene ontology (GO) and functional annotation was used for the enrichment analysis. The GO biological process terms were assigned to each gene in the list with MOSAIC (version 1.1)17, and then the gene lists for functional enrichment were analyzed by NOA (version 1.1)18. In order to control the type I error rate of multiple hypotheses testing, Benjianmini & Hochberg method was employed to adjust P-values, so GO terms were considered as statistically significant overrepresented functions with adjusted-P < 0.05. Besides the regular differential expression analysis for each individual chase period, we also evaluated the trend of gene expression changes between GFP+ and GFP− over the chase time. A list of 3277 genes, differentially expressed in at least one chase period was obtained. From this list we picked 786 genes with monotonic fold changes over time (i.e. going from lower fold changes at 28 d chase to higher fold changes over chase periods in GFP+ and GFP− cell populations). Sequence reads from GFP+ and GFP− abnormal corneas were normalized with normal samples using DESeq2.
Comparative analysis between corneal epithelial GFP+ cells and hair follicle stem cells
In order to obtain putative markers of corneal stem cells, we compared our data in the cornea from 42 and 91 d chase GFP+ LRCs to Cluster of Differentiation 34 (CD34+) HFSCs from WT back skin13 (GSE54424) and the data was analyzed in the same manner as above. A total number of 13150 genes were used for the comparison of corneal GFP+ cells from 42 and 91 d chase corneas versus HFSCs.
Histological staining of adult cornea and conjunctival tissues
Adult 9 week old WT CD1 cornea and conjunctiva tissues were dissected in PBS, fixed in 4% paraformaldehyde (PFA) for 30 mins and embedded in Tissue Tek Optical Cutting Temperature compound (Sakura Finetek Japan Co., Tokyo, Japan) and snap frozen in liquid nitrogen. Cornea sections of 8μm were mounted onto Superfrost Plus Gold slides (Fisherscientific, MA) and stained with haemotoxylin and eosin.
Immunofluorescence detection of RNA-Seq derived candidate genes
Adult WT CD1 6–10 week old globes were fixed in 4% paraformaldehyde (PFA) for 20 mins, corneas were dissected in PBS, embedded in Tissue Tek and snap frozen in liquid nitrogen. Cornea sections of 8 μm were mounted as above, washed in 0.1% PBST, blocked (10% normal goat serum (NGS), 1% Bovine Serum Albumin + 0.1% Triton × 100 in PBS (PBST)) for 1 hr at room temperature and primary antibodies were incubated overnight with rabbit polyclonal antibodies (in blocking buffer as above containing 5% NGS) Sry-Box 9 (Sox9) (Millipore, AB5535, 1:1000), Annexin A3 (Anxa3) (Proteintech, 11804-1-AP, 1:100), Frizzled 7 (Fzd7) (Millipore, 06–1063, 1:300), Actinin1 (Actn1) (Sigma, HPA006035 1:750), Keratin 17 (Krt17) (Santa Cruz, 101931, 1:250). The following day slides were washed twice in 0.1% PBST for 15 mins and an anti-rabbit Cy3 (Jackson Immunoresearch: 711-165-152, 1:500) was used as secondary antibody and incubated for 1 hr at room temperature in blocking buffer containing 5% NGS. Slides were mounted in Vectashield containing DAPI (Vector Laboratories, Inc., CA) for nuclear staining.
Immuno co-localization of GFP+ cells with putative stem cell markers
Adult K5Tta × TRE-H2BGFP+ globes were fixed in 4% PFA for 4 mins prior to dissecting out the cornea in PBS to process for OCT embedding as described above. Corneal sections from chased corneas (at 35 and 53 d) containing strong nuclear localized GFP signals were used for co-localization of slow cycling cells with putative stem cell markers of the cornea. Sections were fixed using 1% PFA for 2 mins, blocked as above and co-stained H2B-GFP+ cells with antibodies Tumor protein 63 (ΔNp63) (Santa Cruz, sc8609, 1:200), Keratin 15 (Krt15) (Proteintech, 10137-1-AP, 1:200), Sox9 (Millipore, AB5535, 1:1000), Fzd7 (Millipore MA, 06-1063), Krt17 (Santa Cruz, sc101931, 1:250) and Actn1 (Sigma-Aldrich, HPA006035, 1:750).
Periodic Acid Schiff (PAS) staining of corneal epithelium to confirm the absence of conjunctival goblet cells on the corneal surface
We required corneas devoid of vessels and goblet cells, as this is an indicator of conjunctivalization. The presence of blood vessels and goblet cells on the corneal surface was analyzed using slit-lamp images following PAS staining in WT and K5Tta × TRE-H2BGFP+ (0, 42, 56 and 91 d chase) mice. Frozen sections from corneas were cut at 8 μm and rehydrated prior to incubation in 0.5% periodic acid solution, followed by staining in Schiff (Electron Microscopy Sciences, PA) reagent. Slides were rinsed in tap water, immersed in Harris haemotoxylin, and further rinsed in water. Slides were dipped in 0.5% acid alcohol, rinsed in water, dipped in ammonium water and further rinsed in water. Sections were dehydrated in a graded series of alcohol, cleared in xylene and mounted with DePeX mounting medium.
Bromodeoxyuridine (BrdU) pulse-chase co-labeling of H2BGFP+ cells from K5Tta × TRE-H2BGFP mice in the cornea
For label retention studies, 21 days old K5Tta × TRE-H2BGFP+ mice (n = 4) were injected intraperitoneally with 50 μg/g BrdU twice a day (at 12 hr intervals) for three consecutive days and fed with 0.8 mg/ml BrdU (BrdU, Sigma-Aldrich, St. Louis, MO) in water for three days. Mice were simultaneously chased with dox for 19 d and sacrificed. Globes were enucleated and the corneas were processed for sectioning (as described above). Frozen sections were cut at 7 μm, fixed in 2% PFA for 2 mins, washed in PBS and the sections were incubated in blocking buffer (as described above) containing DAPI for 30 mins at room temperature. The sections were washed in PBS and incubated in primary chicken polyclonal anti-GFP antibody (Abcam, ab13970, 1:1000) at 4 °C overnight. The following day, sections were washed in PBS with 0.1% PBST and were incubated with anti-chicken secondary antibody (Life technologies, A11039, 1:500) for 1 hour at room temperature. The sections were washed in PBST, fixed in 4% PFA for 15 mins, and further washed in PBS. Sections were incubated in 2 N HCL 37 °C for 30 mins, washed in PBS, blocked for 30 mins and incubated in anti-BrdU Biotin conjugated antibody (Millipore, MAB3262B, 1:100) at 4 °C overnight. The following day, secondary mouse antibody (Jackson Immunoresearch, 200-072-211, 1:150) was added in blocking buffer containing DAPI for 1 hour at room temperature. The sections were washed in PBS with Triton X 100, then incubated in PBS-DAPI for 2 mins, washed twice in PBST and then mounted in Vectashield (Vector Laboratories, Inc., CA).
Carl Zeiss Axiovision Microscope (Carl Zeiss Microimaging GmbH, Jena, Germany) was used to observe corneal wholemounts. Images were taken with an Observer Z1 fluorescent microscope (Carl Zeiss, AG) at 10x and 20x objective lenses utilizing a 1.6 Optovar optic and mosaic tile images. AxioCam HRm digital camera (Zeiss) was used to capture phase contrast images. Immunofluorescence staining from corneal sections was captured using a Zeiss LSM-710 confocal microscope (Carl Zeiss, NY). Images were compiled in Photoshop CS5.1 and Illustrator CS5.1 (Adobe systems Incorporated, USA).
The histone H2B-GFP pulse-chase system identifies slow cycling cells of the cornea
The double transgenic murine system has been used to detect slow cycling cells in various epithelial tissues8,12,19,20. The mating of two parent transgenic strains (K5Tta and TRE-H2BGFP) produces progeny in which the expression of a transgene encoding histone H2B-green fluorescent protein (H2B-GFP) can be turned off (beginning the chase period) when dox is added to the animal’s diet. (Fig. 1A). A time course analyzing the pattern of H2B GFP+ cells from 0–91 d chase enabled us to follow the label retaining cells in the corneal epithelium (Fig. 1B). At 0 d chase, GFP+ cells populated the majority of corneal cells on the ocular surface. After 10 d chase, a clear separation between the limbus and central cornea was observed, indicating the dox had taken effect by suppressing H2B expression. At 28 d chase, GFP expression was restricted to the corneal periphery and limbus. At the 53 d chase time point, GFP+ cells were few and localized only at the limbus, with a further diminution of GFP+ cells seen at the limbus by the 91 d chase time. These data suggested that the label-retaining cells were slow-cycling.
Unexpectedly, we found that some K5Tta × TREH2B-GFP+ mice spontaneously exhibit corneal anomalies as early as P14, including neovascularization, inflammation, and conjunctivalization (Supplementary Fig. 1). The corneas from adult WT FVB (Supplementary Fig. 1Aa), parent strain corneas K5Tta (Supplementary Fig. 1Ab) and TRE-H2BGFP (Supplementary Fig. 1Ac) were clear and normal when observed under slit lamp. We found an approximate 1:1 ratio of normal (Supplementary Fig. 1Ad), and abnormal corneas (as described above) (Supplementary Fig. 1Ae) in K5Tta × TRE-H2BGFP progeny. In all cases, corneas selected for molecular and histological analyses were devoid of corneal anomalies by pre-screening with slit lamp microscopy as seen in Supplementary Fig. 1A. In order to determine if outwardly “normal” mice had phenotypes that were left undetected by slit lamp microscopy, such as the appearance of goblet cells over the surface, we further analyzed these mice for signs of ocular surface abnormalities. Sections of PAS stained corneas from WT FVB, 21 d pulse or 0 d chase (Supplementary Fig. 1B), and pre-screened slit lamp imaged corneas from double transgenic mice after 42 and 91 d chase were devoid of goblet cells (Supplementary Fig. 1). However, PAS stained sections from mice with corneal defects (Supplementary Fig. 1Ad) revealed goblet cells at the surface of the cornea at 56 d chase (Supplementary Fig. 1). Additionally, differences in the distribution of GFP signal was observed when normal versus abnormal corneas were analyzed. In clear normal corneas from double transgenic mice chased for 28 d, a clear GFP+ ring was observed around the limbal region. Abnormal corneas from mice chased at 35, 42 and 49 d, showed a scattered distribution of GFP+ cells in limbal and central corneas with cellular appearance, and other parts were non-cellular and GFP+ due to autofluorescence, when viewed under fluorescent light (Supplementary Fig. 1C). We also observed that abnormal corneas have a different degree of differentiation when comparing the GFP+ cell population to GFP− at 84 d to normal corneas from 91 d chase periods. In abnormal corneas, higher Krt12 (differentiation marker) expression was found in GFP+ cells (Supplementary Fig. 1D). As expected, 91 d chased GFP+ LRCs from normal corneas showed a significant decrease in Krt12 expression. Putative stem cell markers Tumor repressor protein (Trp63), Krt15, Fzd7, β-catenin (Ctnnb1), Sox9, Ifitm1 and candidate marker Actn1 all showed elevated expression in the abnormal GFP− cell populations compared to the normal GFP+ cell populations found at 42 d chase (data not shown) and 91 d chase (Supplementary Fig. 1D). In contrast, Abcg2 was up-regulated in abnormal GFP+ cells compared to the GFP− and was shown to have the opposite effect in our normal GFP+ LRCs (Supplementary Fig. 1D).
Stem-like genes are significantly up-regulated as chase period’s increase
To further characterize GFP+ LRCs in the cornea, we performed FACS analysis comparing them to GFP− fast-dividing cells. The optimal chase duration was not known for the corneal epithelium. We examined three chase periods to ascertain the length of time needed to enrich for GFP+ cells expressing “stem-like” genes. FACS analysis at the 28 d chase demonstrated that 51% of corneal epithelial cells remained GFP+. By 42 d chase this decreased to 41% and then further reduced to 6% at 91 d chase (Fig. 2A). Negative control data using WT corneal epithelial cells from entire globes for each experiment were less than 1% GFP+ likely due to autofluorescence (Supplementary Fig. 2).
Scatterplots generated for differentially expressed genes for each chase period shows greater differences in gene expression in GFP+ LRCs as compared to the GFP− population as chase periods increase (Fig. 2A). The heatmaps generated are visual representations of 12,597 genes, (red, high expression; blue, low expression) comparing the normalized read counts of each gene as a single line in GFP− to GFP+ at 28 d, 42 d and 91 d chase with average read counts of less than twenty.
At 28 d chase, 487 (3.86%) genes show a significant change (2 fold change and FDR < 0.05) between GFP+ and GFP− cells. At 42 d chase, this increased to 2341 (18.58%) genes, similar to the 2396 (18.80%) value obtained at 91 d chase. Of these genes, 247 were found to be significantly up-regulated in GFP+ cells at 28 d chase; 1207 at 42 d chase and 1515 at 91 d chase (Fig. 2). In contrast, 240, 934 and 881 genes were down regulated in chase period 28 d, 42 d and 91 d respectively.
The Venn diagram represents overlapping significant genes (2 fold change and FDR < 0.05) in 42 d and 91 d chase periods (Fig. 2B). The percentage difference of genes changed at 91 d chase to 42 d chase equates to 60%. The gene percentage shared between 42 d and 91 d is 61%. The data shows approximately 40% of genes unshared amongst longer time points of 42 d and 91 d chase (Fig. 2B).
Gene ontology (GO) and pathway analysis for enriched genes in GFP+ LRCs and GFP− differentiated cells
A total of 3277 genes demonstrated differential expression between GFP− and GFP+ LRCs. We performed further analysis to determine if the changes in expression levels resulted in functional enrichment (Fig. 3). Using GO and KEGG (Kyoto encyclopedia of genes and genomes) pathway analysis, we found 786 genes with significant expression changes along the chase time points of 28, 42 and 91 d by the generalized linear model of DESeq2. This was then categorized into 2 enriched gene sets, 1) 651 up-regulated in GFP+ LRCs ascending the chase periods (Fig. 3A) and 2) 135 down-regulated in GFP+ LRCs, descending expression across chase periods (Fig. 3B). The most common trend for regulation of genes in these enriched sets was low expression difference (blue) between GFP+ and GFP− LRCs at 28 d chase with subsequent high expression difference (red) at 91 d chase. In addition to genes identified by our statistical analysis, we also included a table of genes implicated in corneal epithelial maintenance (Fig. 3A). Here, we found an elevated expression of Krt15, Sox9, Actn1, Fzd7, Bone morphogenic protein 4 (Bmp4), Transcription factor 3 (Tcf3), Interferon Induced Transmembrane Protein 1 (Ifitm1) and C-X-C motif chemokine 10 (Cxcl10) in GFP+ LRCs. Genes enriched in GFP− cells included epithelial differentiation marker Krt12 and Ivl. We also show that these cells significantly include an enriched level of the histone gene Histone cluster 1 H1 family member c (Hist1h1c).
Hair follicle stem cell markers are shared by GFP+ LRCs of the cornea
We compared the gene expression of WT CD34+ HFSCs (data obtained from Kadaja et al.13) to LRCs from the corneal epithelium at 42 d and 91 d chase (Fig. 4). Later chase periods were selected since in post 42 d chase the molecular analysis shows increased regulation of several stem cell related genes (as seen in Fig. 2). As discussed above, many regulated genes were common to both chase periods, but each period had a set of distinctly regulated genes, as well. The heat map represents the differences in gene expression between CD34+ HFSCs and GFP+ LRCs at 42 and 91 d chase respectively. Similar trends are observed across the two panels since the colors displayed little variation (Fig. 4A). A comparison of genes expressed in HFSC markers to the GFP+ LRCs at 42 and 91 d chase are highlighted in a table (Fig. 4B). In this analysis we found that the same level of expression of HFSC markers Krt5, Sox9, Tcf3, Contraction of Sma and Mad (Mothers against decapentaplegic) (Smad) 1, 5, 6, Trl2 and Bmp4, was found in corneal GFP+ LRCs (42 and 91 d chase). CD34 was found to be specific to HFSCs due to negligible expression in corneal epithelium. In addition, we pooled novel corneal candidates from our comparison to HFSCs to test on corneal tissue that were 1) Not significantly different between HFSCs and LRCs of the cornea; 2) Significantly up-regulated in only the HFSCs; 3) Significantly up-regulated in corneal epithelial LRCs at post 42 d chase compared to HFSCs. Collectively, these genes are known to play a role in maintaining epithelial HFSCs (Fig. 4B).
The Venn diagram shows differential expression analysis between CD34+ HFSCs and GFP+ LRCs from 42 and 91 d chase respectively (Fig. 4C). There are approximately 1000 more differentially expressed genes between HFSCs and 91 d chase compared to 42 d chase. There are 5308 genes shared between HFSCs and cornea LRCs at 42 and 91 d chase from a total of 13150 genes (Fig. 4C).
GFP+ LRCs co-localize with putative stem cell markers
Protein expression of candidate genes identified from the differentially expressed GFP+ versus GFP− corneal epithelial cells from RNA-Seq analysis was first determined by immunolocalization on wild-type corneal sections (shown in Supplementary Fig. 3). Immunocharacterization of Sox9, Krt17, Anxa3, Fzd7 and Actn1 (red) merged with DAPI (nuclear staining) are shown on sections of WT corneas (Supplementary Fig. 3).
BrdU co-localization with H2B-GFP+ cells marked approximately 80% of cells at the limbus at 19 d chase (Fig. 5). A mixed population of bright, medium and low expressing H2B-GFP+ cells were detected, with greater numbers of GFP+ cells marking the basal layer and weaker H2B-GFP+ expression extended to a few cells in the suprabasal layers of the limbus (Fig. 5B,D). The data shows that after this chase period, the BrdU+ cells co-localized with H2B-GFP+ cells with high and medium expression at the limbus as cells were dividing towards the suprabasal layers (Fig. 5F).
To further implicate candidate genes in the maintenance of the LRC population, co-localization analysis was performed on K5Tta × TRE-H2BGFP corneal tissue for candidate and putative stem cell markers (red) with LRCs (green) at 35 d chase (Krt15, Krt17 and Fzd7) and 53 d chase (P63, Sox9 and Actn1) (Fig. 6). Histological staining of the entire globe without the lens tissue in low power included the central cornea, cornea-limbal and corneal-conjunctival tissue. Higher power images indicate the central (more differentiated) and the limbal (stem cell rich) regions of the cornea (Fig. 6A). At 35 d chase, H2BGFP+ cells were still expressed in a high (basal), medium (suprabasal) and low (suprabasal) manner, while at 53 d chase, H2BGFP+ cells were peripherally localized and mostly basal. GFP+ LRCs after 35 d chase, marked the basal cells at the peripheral cornea and limbus. Stem cell marker Krt15 was not found in the central cornea and only localized at the limbus. The co-localization of few GFP+ LRCs at the limbus with Krt15 was observed (Fig. 6A). GFP+ LRCs at 53 d chase were localized to few cells in basal limbus cells only co-localizing with the majority of ΔNp63+ limbal basal cells (Fig. 6B). Epithelial stem cell marker Sox9 co-localized with GFP+ cells at the limbus, and the expression extended throughout the basal cells of the cornea (Fig. 6C). Actn1 staining in the central cornea marked approximately half of the central corneal basal cells (see Supplementary Fig. 3C), with greater expression at the limbus, co-localizing with few GFP+ LRCs (Fig. 6D). At 35 d chase, Fzd7 extended the limbus and was devoid of expression in the central cornea. Fzd7 co-localized with GFP+ cells at the limbus that were basal including H2BGFP+ cells included some cells to a row above (Fig. 6F). Krt17 co-localized with GFP+ cells at the limbus, in particular the basal cells (Fig. 6G).
Limbal stem cell (LSC) isolation, and subsequent use of these purified stem cells for possible therapeutics has proven to be challenging. Strategies to purify LSCs could include the use of validated stem cells markers coupled with FACS. However, this strategy, largely effective for stem cells of other lineages including HFSCs21, hematopoietic and mesenchymal stem cells22,23 is not so straightforward for corneal LSCs given the paucity of bona fide LSC markers. A second strategy, using the underlying cell biological properties would not rely on prior knowledge of stem cell markers, but would instead be agnostic to previously defined proteins or molecular markers. An important characteristic of LSCs, and indeed stem cells in general is their slow cycling phenotype. Slow cycling stem cells reported in the salivary glands11 sebaceous glands10 and hair follicles7 reside in “niches”, dividing to produce daughter stem cells. Despite technical advances made to label slow cycling LSCs using tritiated thymidine or BrdU, they cannot be purified for molecular characterization, hence a mouse genetics approach labeled their slow cycling nature with GFP2.
Prior to dox administration in our model, GFP+ cells migrate centripetally over the ocular surface forming stripes and spiral patterns consistent with other studies when LacZ or fluorescently labeled transgenics are made12,24,25,26. Soon after dox administration and the chase begun, we observed that the extensive GFP labeling changed to specific regions of highly GFP positive cells, one at the limbus, and the other in the center of the cornea, forming a “doughnut-like” configuration. While both regions represent populations of non-dividing cells, the loss of this central labeled population as the chase periods were extended suggests that the labeled cells at the limbus represent a true slowly dividing stem cell compartment while the cells in the center merely represented terminally differentiated corneal epithelial cells which were sloughed from the surface over time. A clear stream of GFP+ dividing cells migrated towards the center suggesting that the source of cell renewal is from the limbus as previously reported2,27,28. In addition to the spatial localization in the X-Y plane to the limbus, we also saw localization in the Z plane as the chase periods lengthened. The observation seen in GFP+ dividing cells followed X, Y, Z hypotheses of Thoft, R. A. & Friend, J., in which stem cell mobility and migration derives from limbal cells at the periphery that divide, giving rise to transient amplifying cells, moving centripetally through the basal epithelium undergoing a limited number of divisions on the central cornea29.
After long-term dox administration >53 d chase, GFP+ cells were limbal specific, residing in a “niche”. GFP+ distribution throughout the corneal epithelial layers in early dox administration was prominently green and cells were sloughing off as part of the natural corneal renewal process. After long-term dox administration, GFP+ cells were switched off in (fast-dividing) supra-basal layers and LRCs were basally restricted at the limbus. This prompted us to further characterize these cells through FACS and high throughput sequencing.
The initial characterization of the transgenic mice demonstrated that approximately 50% presented corneal anomalies including signs of conjunctivilization and vascularization. We compared RNA-Seq data from abnormal and normal corneas and found that the tissues from abnormal corneas present a different subset of gene expression likely due to signs of vascularization, conjunctivilized overgrowth and other unknown anomalies compared to the normal clear corneas of the same transgenic mice. These side effects could be due to the deleterious effects of GFP, since several studies have shown that high levels of GFP can be toxic to cells in vivo in transgenic animals30,31. In half of the pups born, anomalies were detected at eyelid opening suggesting that GFP toxicity to cells may have occurred in the embryo. In our studies the phenotypes were observed in both eyes of an affected animal. However, we did note in rare cases that only a single eye has the abnormal phenotypes described at the time of eyelid opening, but that these mice ultimately are affected. This would favor an explanation of these abnormalities based on genetic background and not a stochastic effect. We are unsure of the exact molecular mechanisms that have resulted in the corneal phenotypes seen in these mice, however in our studies we excluded mice with abnormal corneal phenotype at eyelid opening and once again prior to obtaining their corneal tissue for the experimental procedures in this paper.
Dox administration commenced at 21 d old, prior to when the stem cells are suggested to fully reside limbally at around 4–5 weeks old26,32,33. Switching off GFP in actively dividing cells at this time period ensured GFP label retaining in slow cycling cells for long periods, over 100 d chase. Initially, we were not certain of an exact chase period in mice to obtain slow cycling cell populations. Therefore, we started chase at 21 d old ensuring the animals were not too old when chasing for extended periods. LESC holoclone production efficiency in human corneas have known to decrease with age26,34. In rat and mice corneas stem cells were localized throughout the ocular surface in basal cells up to two weeks post birth26,33,35. Then, preferential binding of the stem cell marker occurred at the limbus after two weeks of age for mice and after 4 weeks for rats35. Although the exact age at which LSC appear in mice is undetermined, studies have shown the postnatal loss of stem cells from the central cornea using analysis of mosaic mouse corneas show LSC maintenance occurs between 5–8 weeks32. Similarly, with increased age, the corrected number of radial stripes in the corneal epithelium declines from ~100 at 10 weeks age to ~50 at 39 weeks, with no further decline up to 52 weeks32,36. The number of active LESCs not necessarily decline with age, but there is a reduction in the number of LESC clones.
The first appearance of entirely peripheral GFP+ LRCs in the cornea was observed at 28 d chase, however, the appropriate chase period to isolate true LSCs by FACS may not coincide merely with limbal localization, but instead may also require the enriched expression of stem cell genes occurring at later chase periods. We combined our H2B-GFP localization with results from molecular characterization of cells purified from GFP+ cells at increasingly longer chase time points to define an appropriate chase period. Over time, GFP expression at the limbus became sparse, suggesting that further enrichment for the slowest cycling cells beyond 28 d chase was required to identify LSCs. Later, molecular changes in GFP+ cells at the limbus, isolated at 28 d, 42 d and 91 d chase were compared.
It was evident in our analysis that 42 d and 91 d chase shared a greater percentage of gene similarities than either did with 28 d chase. That being said, the significantly up-regulated genes at 42 d and 91 d chase expressed unique markers at each chase period, suggesting that GFP+ LRCs represent different subsets of cells with increased chase time. At 28 d chase, the heat map generated in GFP− and GFP+ populations did not produce as many differential genes as the genes expressed between the two populations at 42 d chase onwards. At 42 d chase we detected significantly up-regulated landmark genes in our LRC population such as P63, Krt15 and Sox9. Although the RNA-Seq expression of GFP+ LRCs presented at 42 d and 91 d chase shared approximately 60% of genes respectively, each cell group represented unique slow cycling cell populations with 40% of genes that were not shared. These differences were likely due to increased aging in animals as chase time progressed and the selection for slower cycling cells with increased chase periods.
In general, cell labeling protocols of the cornea have used a chase period of 56 days to decipher limbal localization of the slow cycling cells2,12,37,38. Previous reports have shown that there was between 0.92–3.6% of LRCs in mouse corneas labeled with BrdU at P3 and chased till adulthood (6–8 weeks), with a preference of slow cycling cells at the inferior and superior quadrants37. In our data, at the 42 d chase period, there were greater numbers of GFP+ cells compared to 91 d chase. We would expect a mixed population of actively dividing and quiescent cells to be expressed at 42 d chase and a likely increase in the proportion of cells that were slow cycling at 91 d chase. After BrDU and doxycycline administration after 19 d chase in our double transgenic mice, H2B-GFP+ cells co-localized to BrDU+ cells at the limbus. Corneal epithelial cell turnover time in mice (time taken for a basal cell to travel to the surface and slough off) is less than or equal to 14 days as tested by BrdU labeling39,40. The turnover time is shorter than the time required for LSCs to replace the entire corneal epithelium, which is estimated to last 7 weeks in mice39. Our double labeling (BrdU and H2B-GFP) of the limbal tissue at 19 d chase, demonstrated that limbal cells are co-labeled effectively at a period where corneal epithelial cells are both in mitotic and slow dividing states.
It has been shown that HFSCs retain GFP labeling at the bulge up until 10 weeks following chase, whereas LRCs in the epithelium from the anal to rectal transition zone showed almost no GFP+ cells after 5 weeks of chase41. Therefore, ideal chase periods identifying slow cycling cells vary with different tissues.
Stem cell populations are both actively proliferating and quiescent. Our model is designed to target LRCs at G0 (quiescent phase). Quantitative analysis from previous reports has shown no evidence of a decline in LRC numbers between 15 and 30 weeks old in WT mice39. Since our chase times varied, the mice ages from each chase period also varied from 49, 63 and 112 d old suggesting that our chase time of 91 d (16 week old), although prolonged, may not affect the number of LRCs over time.
Comparative microarray expression of genes in human central and limbal corneas identified four genes, namely Krt15, Krt14, Cdh3 and Wnt4 as limbal and basal rich, and significantly up-regulated in corneal stem cells42. These markers were then co-localized with BrdU labeling in human limbal explants showing that they are slow cycling in nature42. Our data in mice also showed that these four markers mentioned above were significantly up-regulated in GFP+ LRCs at 42 d chase and onwards.
To corroborate the RNA-Seq expression in this model with known molecular markers of stem cells in the literature, we looked at genes up-regulated in LRCs of the cornea including the Wnt signaling gene network. Products of these Wnt genes act as niche factors maintaining cell renewal43,44,45 by regulating cell proliferation and binding to Frizzled (Fzd) cell surface receptors. Fzd7 belonging to the Frizzled family of G-coupled receptors mark limbal basal cells46 and was significantly up-regulated at the limbus compared to the central cornea. ß-catenin controlling the stability of Fzd, (also up-regulated in GFP+ LRCs after 42 d chase) functions with the protein transcription factor 3 (Tcf3)47 not yet reported in the corneal epithelium regulating cell cycle progression. Fzd7 and Tcf3, known as epidermal stem cell markers were up-regulated at 42 d chase onwards, but not at 28 d. Similar increased expression of the stem cell related genes interferon induced transmembrane protein 1 (Ifitm1, a marker significantly up-regulated in LSCs48) and Keratin 15 (Krt15, an epithelial stem and progenitor marker49,50) were also observed with Ifitm1 expression and Krt15 expression up-regulated at in GFP+ LRCs.
Cell adhesion molecules (CAMs) known to specialize in cellular niches protecting and maintaining stem cells51 were observed in GFP+ LRCs. Actinin 1 or α-Actinin (Actn1) expression has previously been reported in the cornea (embryonic chick52 and rat53). In our experiments, Actn1 was significantly up-regulated throughout chase periods in GFP+ LRCs. Likewise, Sry box 9 (Sox9), a cell adhesion molecule and an epithelial stem cell marker13,54,55 was up-regulated in all chase periods in GFP+ LRCs. We examined cell cycle related genes changes between slow cycling cells and their faster dividing counterparts. Quiescent cells in the cell cycle exit at G0 stage, where they do not replicate. Our RNA-Seq analysis examined genes involved in cell division that included the Cyclin dependent kinases (Cdks). These genes act as key regulators of the cell division cycle and we found a significant elevation of Cdk1 in GFP+ cells at 42 d chase and thereafter suggesting a decrease in cell division. In contrast, the expression of known differentiation markers such as Keratin 12 (Krt12) and Involucrin (Ivl) were significantly increased in GFP− cells, as might be expected. The Histone gene, Hist1h1c1 was enriched in our GFP− populations after 42 d chase suggesting the presence of fast-dividing cells. No other histone complexes were significantly observed in our LRC populations after 42 d chase. Surprisingly, in our corneal RNA-Seq analysis we did not identify ATP binding cassette subfamily B member 5 (Abcb5), a more recent corneal stem cell marker33 expressed in either GFP+ or GFP− cell population.
The most promising limbal stem cell markers in humans such as, CCAAT enhancer-binding protein δ (C/EBPδ)56, BMI1 Proto-Oncogene, Polycomb Ring Finger (Bmi1)56, ΔNp63α57, ΔNp6357,58, ATP-binding cassette sub-family G member 2 (ABCG2)1,59, N-Cadherin60 (N-cad or Cdh2), and Integrin α9 (ITGA9)59 localized in basal cells. Our data in mice has corroborated the expression pattern of human ΔNp63 to being limbal and basal specific. However, neither Itga9 (detected) nor Cdh2 (undetected) were significantly up-regulated in GFP+ LRCs at any chase period. Abcg2 and C/ebpδ were only up-regulated at the 28 d chase period.
The cornea, like the epidermis, functions as a barrier, playing a critical role in maintaining the immune-privileged status of the cornea, its clarity, and wound healing properties. Our data comparing cornea versus skin (data obtained by Kadaja et al.13) showed similar expression of HFSC markers Krt15, Sox9, Tcf3, Smad1, 561, 6 and Fzd7 to corneal derived LRCs perhaps suggesting analogous functions in these cell types. Given the differences in distribution of stem cells (bulge niches across skin and specific limbal niches for the cornea) as well as differences in the proportion of these epithelia (keratinized skin vs non keratinized cornea) we would expect some possible differences in the gene expression of stem cells in these tissues. As expected we found the HFSC marker CD34 was unique to skin and barely expressed in the cornea, and we also found Nuclear factor of activated T-cells, cytoplasmic 1 (Nfatc1) expression, significantly expressed in HFSCs.
We tested our skin-cornea analysis by looking in WT cornea tissue for the presence of highly up-regulated stem cell markers using immunostaining. We found high expression of Krt15, Fzd7 and Krt17 in limbal basal cells, whilst Sox9, Actn1 (cytoskeletal protein) and Anxa3 (membrane and cytoplasmic), expression also extended to few basal epithelial progenitors, thus corroborating our RNA-Seq data.
Localizing GFP+ cells in our model after longer chase periods were difficult to obtain since fewer GFP+ cells exist through the sections. Therefore, we used chase periods under 56 d chase to co-localize GFP+ LRCs to candidate markers. We explored the expression of stem cell markers in the cornea Krt15, ΔNp63 and Sox9 by co-localizing this gene to GFP+ LRCs in the nuclei of our corneas from the double transgenic. These markers although significantly up-regulated at the limbus, were not specific to slow cycling cells. Similarly, Actn1 expression was not exclusive to GFP+ LRCs and was prominently expressed in basal limbal cells extending to 50% of the central basal cells. In other tissues, this gene regulates cytokinesis, cell adhesion, spreading, migration and signalling62. From our pathway analysis we showed that 28 d chase may not be sufficient time for slow cycling cells to exist, since many of the key regulators involved in stemness namely, Krt15, Bmp4, Fzd7, Ctnnb1, Carcinoembryonic antigen-related cell adhesion molecule 1 (Cecam1) and A Disintegrin and metalloproteinase domain-containing protein 8 (Adam8) were not significantly up-regulated in the earlier chase stage. Given the expression of putative stem-like genes presented in our RNA-Seq results from GFP+ LRCs and GFP− cells, slow cycling cells would be best obtained after 42 d chase, closer to 91 d chase periods.
Our model isolates slow cycling cell populations of the corneal epithelium at the limbus but in greater quantities than we expected. Label retaining cells using this model has proven useful in studying corneal epithelial cell turnover to monitor divisions over time. This system can label virtually all LSCs independent of their cell cyclic stage and the gene expression analysis has provided an array of molecular markers showcasing key differences between the “fast” and “slow” cycling cells.
de Paiva, C. S., Chen, Z., Corrales, R. M., Pflugfelder, S. C. & Li, D. Q. ABCG2 transporter identifies a population of clonogenic human limbal epithelial cells. Stem cells 23, 63–73, https://doi.org/10.1634/stemcells.2004-0093 (2005).
Cotsarelis, G., Cheng, S. Z., Dong, G., Sun, T. T. & Lavker, R. M. Existence of slow-cycling limbal epithelial basal cells that can be preferentially stimulated to proliferate: implications on epithelial stem cells. Cell 57, 201–209 (1989).
Haskjold, E., Bjerknes, R. & Bjerknes, E. Migration of cells in the rat corneal epithelium. Acta Ophthalmol (Copenh) 67, 91–96 (1989).
Alonso, L. & Fuchs, E. Stem cells of the skin epithelium. Proceedings of the National Academy of Sciences of the United States of America 100(Suppl 1), 11830–11835, https://doi.org/10.1073/pnas.17342031001734203100 (2003).
Almeida-Porada, G., Zanjani, E. D. & Porada, C. D. Bone marrow stem cells and liver regeneration. Exp Hematol 38, 574–580, https://doi.org/10.1016/j.exphem04.007 (2010).
Moore, J. E., McMullen, C. B., Mahon, G. & Adamis, A. P. The corneal epithelial stem cell. DNA and cell biology 21, 443–451, https://doi.org/10.1089/10445490260099737 (2002).
Oh, I. H. & Kwon, K. R. Concise review: multiple niches for hematopoietic stem cell regulations. Stem cells 28, 1243–1249, https://doi.org/10.1002/stem.453.
Tumbar, T. et al. Defining the epithelial stem cell niche in skin. Science 303, 359–363, https://doi.org/10.1126/science.10924361092436 (2004).
Fuchs, E. & Horsley, V. Ferreting out stem cells from their niches. Nature cell biology 13, 513–518, https://doi.org/10.1038/ncb0511-513 (2011).
Parfitt, G. J., Geyfman, M., Xie, Y. & Jester, J. V. Characterization of quiescent epithelial cells in mouse meibomian glands and hair follicle/sebaceous glands by immunofluorescence tomography. The Journal of investigative dermatology 135, 1175–1177, https://doi.org/10.1038/jid.2014.484 (2015).
Zhang, H. et al. Defining the localization and molecular characteristic of minor salivary gland label-retaining cells. Stem cells 32, 2267–2277, https://doi.org/10.1002/stem.1715 (2014).
Parfitt, G. J. et al. Immunofluorescence Tomography of Mouse Ocular Surface Epithelial Stem Cells and Their Niche Microenvironment. Investigative ophthalmology & visual science 56, 7338–7344, https://doi.org/10.1167/iovs.15-18038 (2015).
Kadaja, M. et al. SOX9: a stem cell transcriptional regulator of secreted niche signaling factors. Genes & development 28, 328–341, https://doi.org/10.1101/gad.233247.113 (2014).
Dobin, A. et al. STAR: ultrafast universal RNA-seq aligner. Bioinformatics 29, 15–21, https://doi.org/10.1093/bioinformatics/bts635 (2013).
Anders, S., Pyl, P. T. & Huber, W. HTSeq–a Python framework to work with high-throughput sequencing data. Bioinformatics 31, 166–169, https://doi.org/10.1093/bioinformatics/btu638 (2015).
Love, M. I., Huber, W. & Anders, S. Moderated estimation of fold change and dispersion for RNA-seq data with DESeq2. Genome Biol 15, 550, https://doi.org/10.1186/s13059-014-0550-8 (2014).
Zhang, C. et al. Mosaic: making biological sense of complex networks. Bioinformatics 28, 1943–1944, https://doi.org/10.1093/bioinformatics/bts278 (2012).
Zhang, C. et al. NOA: a cytoscape plugin for network ontology analysis. Bioinformatics 29, 2066–2067, https://doi.org/10.1093/bioinformatics/btt334 (2013).
Zhang, Y. V., Cheong, J., Ciapurin, N., McDermitt, D. J. & Tumbar, T. Distinct self-renewal and differentiation phases in the niche of infrequently dividing hair follicle stem cells. Cell stem cell 5, 267–278, https://doi.org/10.1016/j.stem.2009.06.004 (2009).
Lu, C. P. et al. Identification of stem cell populations in sweat glands and ducts reveals roles in homeostasis and wound repair. Cell 150, 136–150, https://doi.org/10.1016/j.cell.2012.04.045 (2012).
Woo, W. M. & Oro, A. E. SnapShot: hair follicle stem cells. Cell 146, 334–334 e332, https://doi.org/10.1016/j.cell.2011.07.001 (2011).
Lv, F. J., Tuan, R. S., Cheung, K. M. & Leung, V. Y. Concise review: the surface markers and identity of human mesenchymal stem cells. Stem cells 32, 1408–1419, https://doi.org/10.1002/stem.1681 (2014).
Shin, J. Y., Hu, W., Naramura, M. & Park, C. Y. High c-Kit expression identifies hematopoietic stem cells with impaired self-renewal and megakaryocytic bias. The Journal of experimental medicine 211, 217–231, https://doi.org/10.1084/jem.20131128 (2014).
Collinson, J. M., Chanas, S. A., Hill, R. E. & West, J. D. Corneal development, limbal stem cell function, and corneal epithelial cell migration in the Pax6(+/−) mouse. Investigative ophthalmology & visual science 45, 1101–1108 (2004).
Mort, R. L. et al. Effects of aberrant Pax6 gene dosage on mouse corneal pathophysiology and corneal epithelial homeostasis. PloS one 6, e28895, https://doi.org/10.1371/journal.pone.0028895 (2011).
Mort, R. L. et al. Stem cells and corneal epithelial maintenance: insights from the mouse and other animal models. Results and problems in cell differentiation 55, 357–394, https://doi.org/10.1007/978-3-642-30406-4_19 (2012).
Dua, H. S. & Azuara-Blanco, A. Limbal stem cells of the corneal epithelium. Survey of ophthalmology 44, 415–425 (2000).
Lavker, R. M., Tseng, S. C. & Sun, T. T. Corneal epithelial stem cells at the limbus: looking at some old problems from a new angle. Experimental eye research 78, 433–446 (2004).
Thoft, R. A. & Friend, J. The X, Y, Z hypothesis of corneal epithelial maintenance. Investigative ophthalmology & visual science 24, 1442–1443 (1983).
Progatzky, F., Dallman, M. J. & Lo Celso, C. From seeing to believing: labelling strategies for in vivo cell-tracking experiments. Interface focus 3, 20130001, https://doi.org/10.1098/rsfs.2013.0001 (2013).
Perl, A. K., Zhang, L. & Whitsett, J. A. Conditional expression of genes in the respiratory epithelium in transgenic mice: cautionary notes and toward building a better mouse trap. American journal of respiratory cell and molecular biology 40, 1–3, https://doi.org/10.1165/rcmb.2008-0011ED (2009).
Collinson, J. M. et al. Clonal analysis of patterns of growth, stem cell activity, and cell movement during the development and maintenance of the murine corneal epithelium. Developmental dynamics: an official publication of the American Association of Anatomists 224, 432–440, https://doi.org/10.1002/dvdy.10124 (2002).
Hayashi, Y., Watanabe, N. & Ohashi, Y. The “replacement hypothesis”: corneal stem cell origin epithelia are replaced by limbal stem cell origin epithelia in mouse cornea during maturation. Cornea 31(Suppl 1), S68–73, https://doi.org/10.1097/ICO.0b013e318269c83f (2012).
Notara, M., Shortt, A. J., O’Callaghan, A. R. & Daniels, J. T. The impact of age on the physical and cellular properties of the human limbal stem cell niche. Age (Dordr) 35, 289–300, https://doi.org/10.1007/s11357-011-9359-5 (2013).
Chung, E. H., Bukusoglu, G. & Zieske, J. D. Localization of corneal epithelial stem cells in the developing rat. Investigative ophthalmology & visual science 33, 2199–2206 (1992).
Mort, R. L., Ramaesh, T., Kleinjan, D. A., Morley, S. D. & West, J. D. Mosaic analysis of stem cell function and wound healing in the mouse corneal epithelium. BMC developmental biology 9, 4, https://doi.org/10.1186/1471-213X-9-4 (2009).
Pajoohesh-Ganji, A., Pal-Ghosh, S., Simmens, S. J. & Stepp, M. A. Integrins in slow-cycling corneal epithelial cells at the limbus in the mouse. Stem cells 24, 1075–1086, https://doi.org/10.1634/stemcells.2005-0382 (2006).
Pajoohesh-Ganji, A., Pal-Ghosh, S., Tadvalkar, G. & Stepp, M. A. Corneal goblet cells and their niche: implications for corneal stem cell deficiency. Stem cells 30, 2032–2043, https://doi.org/10.1002/stem.1176 (2012).
Douvaras, P. et al. Increased corneal epithelial turnover contributes to abnormal homeostasis in the Pax6(+/−) mouse model of aniridia. PloS one 8, e71117, https://doi.org/10.1371/journal.pone.0071117 (2013).
Hanna, C. & O’Brien, J. E. Cell production and migration in the epithelial layer of the cornea. Archives of ophthalmology 64, 536–539 (1960).
Runck, L. A., Kramer, M., Ciraolo, G., Lewis, A. G. & Guasch, G. Identification of epithelial label-retaining cells at the transition between the anal canal and the rectum in mice. Cell cycle 9, 3039–3045 (2010).
Figueira, E. C., Di Girolamo, N., Coroneo, M. T. & Wakefield, D. The phenotype of limbal epithelial stem cells. Investigative ophthalmology & visual science 48, 144–156, https://doi.org/10.1167/iovs.06-0346 (2007).
Nusse, R. et al. Wnt signaling and stem cell control. Cold Spring Harbor symposia on quantitative biology 73, 59–66, https://doi.org/10.1101/sqb.2008.73.035 (2008).
Fevr, T., Robine, S., Louvard, D. & Huelsken, J. Wnt/beta-catenin is essential for intestinal homeostasis and maintenance of intestinal stem cells. Molecular and cellular biology 27, 7551–7559, https://doi.org/10.1128/MCB.01034-07 (2007).
Hsu, Y. C., Li, L. & Fuchs, E. Emerging interactions between skin stem cells and their niches. Nature medicine 20, 847–856, https://doi.org/10.1038/nm.3643 (2014).
Mei, H., Nakatsu, M. N., Baclagon, E. R. & Deng, S. X. Frizzled 7 maintains the undifferentiated state of human limbal stem/progenitor cells. Stem cells 32, 938–945, https://doi.org/10.1002/stem.1582 (2014).
Yi, F. et al. Opposing effects of Tcf3 and Tcf1 control Wnt stimulation of embryonic stem cell self-renewal. Nature cell biology 13, 762–770, https://doi.org/10.1038/ncb2283 (2011).
Takacs, L. et al. Differentially expressed genes associated with human limbal epithelial phenotypes: new molecules that potentially facilitate selection of stem cell-enriched populations. Investigative ophthalmology & visual science 52, 1252–1260, https://doi.org/10.1167/iovs.10-5242 (2011).
Yoshida, S. et al. Cytokeratin 15 can be used to identify the limbal phenotype in normal and diseased ocular surfaces. Investigative ophthalmology & visual science 47, 4780–4786, https://doi.org/10.1167/iovs.06-0574 (2006).
Liu, Y., Lyle, S., Yang, Z. & Cotsarelis, G. Keratin 15 promoter targets putative epithelial stem cells in the hair follicle bulge. The Journal of investigative dermatology 121, 963–968, https://doi.org/10.1046/j.1523-1747.2003.12600.x (2003).
Marthiens, V., Kazanis, I., Moss, L., Long, K. & Ffrench-Constant, C. Adhesion molecules in the stem cell niche–more than just staying in shape? Journal of cell science 123, 1613–1622, https://doi.org/10.1242/jcs.054312 (2010).
Khoory, W., Wu, E. & Svoboda, K. K. H. Intracellular Relationship between Actin and Alpha-Actinin in a Whole Corneal Epithelial Tissue. Journal of cell science 106, 703–717 (1993).
Torrado, M., Senatorov, V. V., Trivedi, R., Fariss, R. N. & Tomarev, S. I. Pdlim2, a novel PDZ-LIM domain protein, interacts with alpha-actinins and filamin A. Investigative ophthalmology & visual science 45, 3955–3963, https://doi.org/10.1167/iovs.04-0721 (2004).
Huch, M. & Clevers, H. Sox9 marks adult organ progenitors. Nature genetics 43, 9–10, https://doi.org/10.1038/ng0111-9 (2011).
Scott, C. E. et al. SOX9 induces and maintains neural stem cells. Nature neuroscience 13, 1181–1189, https://doi.org/10.1038/nn.2646 (2010).
Barbaro, V. et al. C/EBPdelta regulates cell cycle and self-renewal of human limbal stem cells. The Journal of cell biology 177, 1037–1049, https://doi.org/10.1083/jcb.200703003 (2007).
Di Iorio, E. et al. Isoforms of DeltaNp63 and the migration of ocular limbal cells in human corneal regeneration. Proceedings of the National Academy of Sciences of the United States of America 102, 9523–9528, https://doi.org/10.1073/pnas.0503437102 (2005).
Pellegrini, G. et al. p63 identifies keratinocyte stem cells. Proceedings of the National Academy of Sciences of the United States of America 98, 3156–3161, https://doi.org/10.1073/pnas.061032098 (2001).
Chen, Z. et al. Characterization of putative stem cell phenotype in human limbal epithelia. Stem cells 22, 355–366, https://doi.org/10.1634/stemcells.22-3-355 (2004).
Higa, K. et al. N-cadherin in the maintenance of human corneal limbal epithelial progenitor cells in vitro. Investigative ophthalmology & visual science 50, 4640–4645, https://doi.org/10.1167/iovs.09-3503 (2009).
Kandyba, E., Hazen, V. M., Kobielak, A., Butler, S. J. & Kobielak, K. Smad1 and 5 but not Smad8 establish stem cell quiescence which is critical to transform the premature hair follicle during morphogenesis toward the postnatal state. Stem cells 32, 534–547, https://doi.org/10.1002/stem.1548 (2014).
Kao, H. Y. The actinin family proteins: biological function and clinical implications. Cell & bioscience 5, 48, https://doi.org/10.1186/s13578-015-0039-5 (2015).
We thank Ya-Chieh Hsu, Meelis Kadaja and Nicole Stokes for technical advice and support with our transgenic murine model. Publication for this article was supported by grants from New York State Stem Cell Science and Tri-Institutional Stem Cell Initiative (M.I.R. and E.F.), Natural Sciences Foundation of China 81200656 (P.W.), National Institutes of Health R21EY025062 (M.I.R.), EY001792 an unrestricted grant from Research to Prevent Blindness, and National Institutes of Health AR050452 (E.F.).
The authors declare that they have no competing interests.
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Sartaj, R., Zhang, C., Wan, P. et al. Characterization of slow cycling corneal limbal epithelial cells identifies putative stem cell markers. Sci Rep 7, 3793 (2017). https://doi.org/10.1038/s41598-017-04006-y
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