New Results

The Lineage-Specific Transcription Factor CDX2 Navigates Dynamic Chromatin to Control Distinct Stages of Intestine Development

Namit Kumar, Yu-Hwai Tsai, Lei Chen, Anbo Zhou, Kushal K. Banerjee, Madhurima Saxena, Sha Huang, Jinchuan Xing, Ramesh A. Shivdasani, Jason R. Spence, Michael P. Verzi
doi: https://doi.org/10.1101/425827

Abstract

Lineage-restricted transcription factors, such as the intestine-specifying factor CDX2, often have dual requirements across developmental time. Embryonic-loss of CDX2 triggers homeotic transformation of intestinal fate, while adult-onset Cdx2-loss compromises critical physiological functions but preserves intestinal identity. It is unclear how such diverse requirements are executed across the developmental continuum. Using primary and engineered human tissues, mouse genetics, and a multi-omics approach, we demonstrate that divergent CDX2 loss-of-function phenotypes in embryonic versus adult intestines correspond to divergent CDX2 chromatin-binding profiles in embryonic versus adult stages. CDX2 binds and activates distinct target genes in developing versus adult mouse and human intestinal cells. We find that temporal shifts in chromatin accessibility correspond to these context-specific CDX2 activities. Thus, CDX2 is not sufficient to activate a mature intestinal program, but rather, CDX2 responds to its environment, targeting stage-specific genes to contribute to either intestinal patterning or maturity. This study provides insights into the mechanisms through which lineage-specific regulatory factors achieve divergent functions over developmental time.

Introduction

Lineage-specifying transcription factors, sometimes called “master regulators”, are required for a cellular lineage to develop in embryos and their loss leads to a selective failure to develop that lineage. Examples include MYOD, which establishes muscle development and induces muscle trans-differentiation in fibroblasts (Davis et al., 1987; Tapscott et al., 1988), or PDX1, which is essential for pancreas development (Jonsson et al., 1994; Offield et al., 1996). Study of lineage-specifying transcription factors is informative during early development, when tissues are specified; however, the same factors often have additional roles in subsequent tissue maturation, organogenesis, and adult homeostasis.

The homeodomain transcription factor, CDX2, is expressed from the onset of intestinal development through adult life. In mice, early deletion of Cdx2 in the visceral endoderm precludes formation of the intestinal epithelium, which is replaced by an esophagus-like homeotic conversion (Gao et al., 2009). When CDX2 is lost early in the developing mouse endoderm, a striking patterning deficit follows, best illustrated by homeotic conversion of intestinal to esophageal epithelium (Gao, 2009), but also observed upon spontaneous loss of heterozygousity of CDX2 leading to harmatomas in the colon with features of esophageal squamous epithelium (Chawengsaksophak et al., 1997; Tamai et al., 1999), and expression of certain gastric markers in the intestinal epithelium upon early embryonic CDX2 inactivation using the Villin-Cre model (Grainger et al., 2010). In striking contrast to these findings, deletion of CDX2 at later stages in fetal and adult life compromises intestinal function, but not tissue identity (Verzi et al., 2010; Verzi et al., 2011), although tissue identity can become permissive when intestinal stem cells lacking CDX2 are isolated and subsequently cultured in a cocktail of factors conducive to gastric cell culture (Simmini et al., 2014), or upon prolonged loss of CDX2 in a subset of tissues (Hryniuk et al., 2012; Stringer et al., 2012).

The distinct consequences of CDX2 loss at different developmental stages prompts questions about the mechanistic basis of lineage-specifying transcription factor activities: Do these factors bind their chromatin targets from the outset or do their transcriptional targets differ along the developmental continuum? How do they interact with chromatin across developmental time? Is expression of a lineage-specific transcription factor sufficient to activate appropriate target genes, even in the absence of extracellular signals? Additionally, while many insights have been garnered from studies in mice, CDX2 function in human tissue specification remains untested.

Here, we employ mouse models and human pluripotent stem cell-derived models, coupled with investigation of chromatin accessibility, to show that CDX2 binds distinct chromatin sites in embryonic and adult intestines; this distinction is conserved in mice and humans. We find that CDX2 is incapable of instructing major shifts in the chromatin to direct its own binding. Rather, it follows the transitions in chromatin landscape that occur in the course of intestine development, and importantly, sustains that evolution. Our identification of distinct binding sites and regulatory functions during tissue specification and in adults provides one explanation for why intestinal identity in the absence of CDX2 is compromised only during a defined developmental window. These findings support a model in which lineage-specifying transcription factors operate in context-dependent roles, shaped by a dynamic developmental chromatin landscape.

Results

CDX2 is required for human intestinal development

In mouse embryos with conditional deletion of Cdx2 in the developing endoderm, the intestinal epithelium exhibits morphologic and molecular characteristics of foregut identity. Esophageal, gastric corpus, or gastric antral identities are observed, depending on the timing of CDX2 loss, with earlier onset of Cdx2 inactivation producing more anterior (rostral) identity shifts (Gao et al., 2009; Grainger et al., 2010). It is unknown whether CDX2 has a conserved role in human intestine development, and new methods to direct differentiation of human pluripotent stem cells (hPSCs) allow us to ask this question (D’Amour et al., 2005; Finkbeiner et al., 2015; McCracken et al., 2011; Spence et al., 2011).

CDX2 expression is first observed upon specification of the hindgut by WNT and FGF signaling (Wells and Melton, 2000). Immunoblotting confirmed absence of CDX2 in human embryonic stem cells (hESC) or definitive endoderm, but combined activation of WNT (using the GSK3β inhibitor, CHIR99021, to stabilize β-CATENIN) and FGF (using recombinant FGF4) signaling triggered robust CDX2 expression, which was sustained in 3-dimensional human intestinal organoid (HIO) cultures months later (Fig. 1A-C). To determine if CDX2 is required to induce the intestinal lineage, we used Cas9/CRISPR to engineer CDX2-null hESC in the H9 line and differentiated the cells into HIOs. Sequencing confirmed mutation of CDX2, and CDX2 immunoreactivity was lost in mutant cells directed toward intestine differentiation (Fig. 1D and S1). Whereas control hESC gave rise to tissues that expressed CDX2 (Fig. 1D) and the intestine-restricted markers AMY2B, MUC2, and DPP4 (Fig. 1E), CDX2-null hESCs failed to develop tissues with these characteristic markers. Instead, they gave rise to organoids expressing transcripts and proteins of CDX2-negative foregut lineages, including stomach, esophagus, pancreas, and gall bladder (Fig. 1D-E). These findings indicate a conserved role for CDX2 in initiating human intestine development and underscore the importance of defining the mechanisms through which CDX2 imparts intestinal fate.

Figure 1.
Figure 1. CDX2 is required for human intestinal development.

A) Differentiation schema used to differentiate hES cells into Human Intestinal Organoids (HIOs). B) Immunoblot and C) RNAseq (E-MTAB-4168, (Tsai et al., 2017)) show that CDX2 expression is only induced robustly after differentiation of ES cells into endoderm with Activin and then induction of hindgut specification via treatment with FGF4 (500ng/ml) and the WNT agonist CHIR99021 (2µM). HIOe = HIO early, pre-transplant; HIOl = HIO late, after transplant into mouse kidney capsule for further intestinal maturation. D-E) While Human Intestinal Organoids (HIO) result from this differentiation protocol, ES cells lacking CDX2 due to Crispr targeting (Fig. S1) do not give rise to HIOs, and instead give rise to organoids expressing genes characteristic of foregut lineages, as seen by immunofluorescent staining (D, representative of at least 3 independent experiments) and qRT-PCR (E) on organoids collected after 30 days in ENR (EGF, Noggin, RSPO) culture conditions. (Unpaired t-test). Scale bars = 200µm.

CDX2 regulates distinct transcriptional targets across human intestinal development

To determine these mechanisms, we performed ChIP-seq on biological replicates (Fig. S2A) of intestine-specified endoderm (herein referred to as ‘Hindgut’, as defined in Fig. 1A) and on primary adult human duodenal epithelium (herein referred to as ‘Adult’). We used MACS (Zhang et al., 2008) to identify ChIP-seq binding sites and k-means clustering to define genomic regions with differential CDX2 occupancy (Fig. 2A-B). Ontology analysis of genes linked to CDX2 binding sites revealed that Hindgut-enriched CDX2 binding occurred near genes that were enriched for functions in development, patterning, and morphogenesis, whereas genes near Adult-enriched CDX2 binding sites were associated with adult intestinal physiological functions (Fig. 2C). DNA sequence motifs enriched at Hindgut- and Adult-enriched regions were also distinct, suggesting that CDX2 works in different regulatory complexes in embryos and adults. The CDX2 motif was strongly enriched in both groups of binding regions, but whereas Hindgut-enriched sites were enriched in NANOG and SOX15 motifs, consistent with a role for SOX factors supporting endoderm development (Kanai-Azuma et al., 2002), Adult-enriched regions were most enriched in HNF4A motifs (Fig. 2D, Table S1), consistent with the function of HNF4 in the mature intestine (Babeu et al., 2009; Cattin et al., 2009; San Roman et al., 2015; Stegmann et al., 2006). Examples of Hindgut-enriched target genes included the HOXB cluster genes (Fig. 2E, S2B) known for their roles in tissue patterning and axial elongation (Young et al., 2009), whereas adult-enriched target genes included the enterocyte differentiation marker ALPI and the differentiation-promoting transcription factor gene HNF4A (Fig. 2E, S2C). These results reveal that human CDX2 binds distinct genomic regions in a stage-specific manner and regulates stage-specific genes.

Figure 2.
Figure 2. CDX2 has distinct transcriptional targets in the developing hindgut versus the adult intestine.

A-B) CDX2 ChIP-seq performed in in vitro differentiated hindgut (4 day FGF4+CHIR treated endoderm, Fig. 1A) and in primary adult human duodenum epithelium show distinct binding profiles, as defined by k-means clustering (A) and compared using composite signal traces (B). (2 biological replicates each, Figure S2A). C) Distinct binding sites correspond to different sets of nearby target genes (within 5 kb of binding sites), as indicated by GO analysis using DAVID. D) CDX2 binding motifs are present in both categories of binding regions, but other transcription factor binding motifs are differentially enriched in the hindgut-enriched or adult-enriched CDX2-binding regions, defined using HOMER. E) Examples of stage-specific CDX2 binding sites are shown using IGV. F) Ectopic expression of CDX2 in endoderm, using a Doxinducible hES cell line (Endoderm + 4 days DOX treatment), is not sufficient to recapitulate CDX2 binding to the majority of its normal hindgut target sites (Endoderm + 4 days CHIR + FGF). Approximately 52% of CDX2 hindgut sites (MACS p < 1e-10) were not detected by MACS in the Dox-inducible condition, even at a lower peak-calling stringency (p < 1e-3). Lack of binding cannot be attributed to differences in CDX2 binding motifs, which were robust in each category of binding site (HOMER). Also see Figure S2 and Table S2.

Both WNT and FGF signals are required to drive robust differentiation of human endoderm into hindgut (Spence et al., 2011) and activation of these signals induces CDX2 expression (Fig. 1A). It is unclear whether CDX2 expression is sufficient for its binding at hindgut regulatory regions or whether CDX2 also requires other sequelae of dual signaling pathway activation to arrive at its hindgut binding regions. To address this question, we engineered hESC for doxycyclineinducible CDX2 expression. ChIP-Seq after forced CDX2 expression in endoderm cells yielded more than twice as many binding sites as were present in CHIR- and FGF4-treated endoderm (135,194 sites compared to 58,981 sites, Fig. 2F), and both groups of regions were enriched in the CDX2 consensus motif (Fig. 2F, Table S2), consistent with bona fide CDX2 binding to these regions. Surprisingly, despite robust expression (Fig. S2E) and occupancy of significantly more genomic sites, ectopic CDX2 failed to bind more than half of the Hindgut-enriched targets occupied in the presence of CHIR and FGF4 (Fig. 2F), despite robust enrichment of consensus CDX2 binding sequences at these regions (HOMER, p = 1e-12760, Fig. 2F, Table S2). Thus, while CDX2 expression is necessary for specification of human intestine (Fig. 1C-D), CDX2 cannot reach its full complement of hindgut chromatin targets in the absence of WNT and FGF signaling cues.

Dynamic CDX2 activity across intestinal development is conserved in mice

To refine and corroborate this model of CDX2 binding and activity in vivo, we turned to mice. First we identified CDX2 binding sites in intestinal cells isolated at embryonic days (E) 13.5, 16.5 and 17.5, and from adult intestines. k -means clustering identified 4 major groups: 4,123 genomic regions were bound more robustly in embryos, 12,551 sites were more specific to the adult (Fig. 3A-B), and the remaining sites were bound similarly at all stages (1,791 sites with robust CDX2 binding and 15,368 sites with modest signals – clusters 1 and 4 in Fig. S3A and Table S3). CDX2 showed a notable transition late in gestation: binding at embryo-enriched sites declined by E16.5, as occupancy of adult-enriched regions became evident (Figure 3A). To test stage-specific binding functions in gene regulation, we purified control and CDX2-depleted epithelium after embryonic knockout (Shh-Cre;Cdx2f/f, collected at E12.5) or adult knockout (Villin-CreERT2;Cdx2f/f) and used RNA-seq to identify CDX2-dependent transcripts. Consistent with CDX2’s activity as a direct transcriptional activator, the genes nearby CDX2 binding sites showed reduced expression upon CDX2 loss at the corresponding developmental stages (Fig. S3B). Developmental stage-specific CDX2 binding regions also correlated with stage-specific gene expression, as genes linked to adult-enriched binding sites were expressed more robustly in adult than in the developing intestine, and the converse was true for embryo-enriched binding targets (Fig. 3C). Thus, stage-specific CDX2 binding predicts nearby gene expression in each context.

Figure 3.
Figure 3. Temporal-specific shifts in CDX2 binding is conserved between mice and humans, and corresponds to temporal shifts in intestinal gene expression.

A) CDX2 ChIP-seq performed at the indicated stages of intestinal development on isolated epithelium show distinct, stage-dependent binding profiles (2 biological replicates each, Figure S3). The heatmap depicts CDX2 ChIP-seq intensity at each of the regions defined as Embryo or Adult-enriched, and in (B) the average ChIP-seq signals at these binding regions is plotted. C) Embryo-enriched and Adult-enriched binding sites correspond to different sets of nearby target genes, which show stage-specific gene expression. RNA-seq was conducted on E12.5 or adult intestinal epithelium and genes linked to Embryo-enriched or Adult-enriched CDX2 binding (within 5kb) were analyzed for their distribution along the E12.5-to-adult expression continuum using GSEA analysis. CDX2-bound genes are also dependent upon CDX2 for expression, as revealed by RNA-seq analysis in Cdx2 knockout tissues (Figure S3B), and have distinct gene ontologies, corresponding to embryo-specific or adult-specific functions (D). Representative examples of Embryo-enriched (E) or Adult-enriched (F) CDX2 binding sites are shown using IGV. Also see Figure S3.

Transcription factor motifs enriched at stage-specific enhancers also suggest dynamic regulatory activity. While CDX2 binding motifs were enriched in both adult- and embryo-enriched binding sites, other motifs were selectively enriched. For example, embryo-enriched CDX2 binding was associated with HOX and FOXA motifs, whereas Adult-enriched binding sites were associated with HNF4, FRA1, and KLF5 motifs (Fig. S3C, Table S3). This divergence points to different transcriptional regulatory networks in the embryonic gut, where developmental competence and tissue patterning predominate (Wang et al., 2015) and in the adult intestine, where cell identity is fixed and CDX2 and partner factors control physiologic functions (Verzi et al., 2010; Verzi et al., 2011). Indeed, ontology analysis indicated that genes near embryo-enriched binding sites associate with developmental processes such as liver development and regulation of stem cell differentiation, whereas genes near Adult-enriched regions associate with mature intestinal functions, including lipid metabolism and brush border (Fig. 3D). Condition-specific binding at developmental genes (HoxB, Fzd10) or those expressed exclusively in the mature tissue (Alpi, Sis) illustrates these findings (Fig. 3E-F, S3D-E). Together, these results reveal that CDX2 has distinct genomic targets at different developmental stages, regulates target genes in a stage-dependent manner, and likely partners with different factors in each context to accomplish stage-dependent gene regulation.

Temporal dissection of Cdx2 requirements for intestinal identity

We next sought to correlate our observed changes in CDX2’s genomic occupancy with observations of homeotic conversion phenotypes upon CDX2 loss. CDX2 loss triggers profound homeotic transformation of the intestine to esophagus when it occurs at E8.5 (FoxA3-Cre, (Gao et al., 2009). When Cdx2 is deleted at E13.5, however certain stomach-specific genes are ectopically expressed without overt squamous cell differentiation (Grainger et al., 2010). We examined the timing of CDX2 dependency more closely, with additional time points of CDX2 inactivation. Mouse endoderm engineered to delete Cdx2 at ~E9.5 using the Shh-Cre driver (Harfe et al., 2004) exhibited stomach characteristics anteriorly in the jejunum (ATP4B and foveolar PAS staining) and stratified squamous esophageal features posteriorly (Fig. 4A, Fig. S4A). Thus loss of CDX2 ~E9.5 results in a homeotic change of intermediate phenotypic severity compared to when CDX2 is lost earlier E8.5 (Gao et al., 2009), or later E13.5 (Grainger et al., 2010). In contrast, we observed no evidence of transformation when we inactivated Cdx2 at later embryonic stages by tamoxifen treatment of dams carrying Villin-CreERT2; Cdx2f/f embryos at E13.5 or E15.5 (Fig. 4A). Thus these late stage embryos, like the adult epithelium upon CDX2-loss (Verzi et al., 2011), retain intestinal identity. A summary of our findings on the consequences of CDX2 inactivation in the developing intestine, along with those previously published, indicates a critical window prior to E13.5 in which intestinal identity is plastic; after this timepoint, intestinal identity is stabilized and less-susceptible to transformation to anterior structures (Fig. 4B). These temporal phenotypes roughly correspond to the dynamic CDX2 binding patterns we observed in ChIP-seq assays of early versus late embryonic intestinal epithelia (Figure 3A) and are consistent with observations that CDX2 target genes partition into functions associated more with developmental process (Embryo-enriched sites) versus mature intestinal physiological functions (Adult-enriched sites, Figure 3D).

Figure 4.
Figure 4. Developmental stage dictates the consequences of CDX2 loss.

A) Analysis of regional tissue identity on samples from control, Shh-Cre; CDX2f/f or Villin-CreERT2; CDX2f/f embryos, treated with tamoxifen to induce CDX2 loss as indicated, and collected at E18.5 from the indicated intestinal region. PAS stain marks mucosubstances, including intestinal Goblet cells, which are identified by a punctate staining and are characteristic in the intestinal epithelium (Control or Villin-CreERT2), whereas broad PAS staining at the apical cell surface is indicative of gastric foveolar cells, as observed in the jejunum of Shh-Cre; Cdx2f/f embryos. TRP63 marks esophageal cells and is not typically found in the intestine, but appears ectopically in the ileum of Shh-Cre; Cdx2f/f embryos, but not in control embryos, or embryos induced to delete Cdx2 in the later stages. The parietal cell marker, ATP4B, is typically expressed in the glandular stomach, but is ectopically expressed in the CDX2-negative jejunum of Shh-Cre; Cdx2f/f embryos, but not in embryos deficient in intestinal CDX2 at the later stages tested. B) Summary of CDX2 loss-of-function phenotypes from this (A) and previous studies. Temporal-specific CDX2 loss at stages early than E12.5 induces homeotic transformations, as observed by Gao and colleagues using the Foxa3-Cre driver (~E8.5), in this study using the Shh-Cre driver (~E9.5), or at ~E13.5 using the VIllin-Cre driver (Grainger et al., 2010). However, acute loss of CDX2 at later developmental stages (>E13.5) and in the adult compromises intestinal digestive functions but intestinal identity is preserved (Villin-CreERT2 with tamoxifen treatment at E13.5, E15.5, or adult), as documented in these studies in the embryo (Gao et al., 2009; Grainger et al., 2010), and previously in the adult (Verzi et al., 2011).

CDX2 follows, then stabilizes, a developmentally dynamic chromatin landscape

CDX2 expression is nearly constant from the onset of intestine development through adult life in both humans (Fig. 1A-B) and mice (Fig. 5A-B). To resolve why CDX2 could function in different capacities despite relatively consistent levels of expression (Figs. 2-3), we examined the possibility that a dynamic chromatin environment could underlie stage-specific CDX2 genomic binding. Chromatin accessibility was measured at all embryonic and adult binding sites using ATAC-seq at E11.5, E14.5, E16.5, E18.5, P1, and Adult. We observed a clear pattern at CDX2-bound regions, with embryo-enriched sites losing accessible chromatin after E14.5, while adult-enriched sites gained chromatin access thereafter (Fig. 5C-D). Four features are notable in this regard. First, 74% of genomic regions with strong adult-enriched CDX2 binding showed poor accessibility in early embryos, lacking ATAC signals at E11.5 (P <10-5; Fig. 5C). Second, open chromatin emerged at these sites in adults (Fig. 5C), where CDX2 binding was clearly absent in the embryo (Figure 3A); the converse was apparent for the embryo-enriched CDX2 binding sites. Third, chromatin dynamics were similar for the active histone mark H3K27ac (Kazakevych et al., 2017), with stage-specific enhancer marks corresponding to stage-specific CDX2 binding regions (Fig. S5A-B). Fourth, stage-specific binding in mouse endoderm resembled the profound shift in binding between human ESC-derived gut endoderm and adult human intestine (Fig. 2A). Thus, despite constant expression across time, CDX2 binding closely follows a temporal wave of accessible chromatin from embryo-enriched to adult-enriched sites. Examples of these findings are illustrated at genes selectively expressed in developing or adult intestine (Fig. 5E-F).

Figure 5.
Figure 5. CDX2 temporally-enriched binding patterns follow a temporally dynamic chromatin landscape that requires CDX2 for maintenance.

A) CDX2 transcripts (from RNA-seq on isolated epithelium) and B) protein levels (via immunostaining) are consistent across mouse developmental time, yet CDX2 occupies distinct sets of genomic regions at different developmental stages (Fig. 3). CDX2 binding chromatin binding shifts may be due to a shifting chromatin landscape across developmental time, as indicated by the ATAC-seq assay for accessible chromatin (C), shown at CDX2’s condition-enriched binding regions (defined in Fig. 3A). D) Average ATAC-seq signal is robust at embryo-enriched CDX2 binding sites prior to E16.5, after which chromatin accessibility at these regions diminishes. The converse is true for adult-enriched CDX2 binding sites. (E-F) Specific examples of condition-enriched chromatin accessibility at CDX2 binding sites. CDX2 binding regions are also dependent upon CDX2-binding to remain accessible to the ATAC-seq assay, as seen in CDX2 knockout epithelium (Figure S5).

The contemporaneous transitions we observed after E14.5 in chromatin accessibility (Fig. 5C-D), CDX2 binding (Figure 3A), and histone marks (Figure S5A-B) coincide roughly with the temporal restriction of Cdx2-null phenotypes (Fig. 4A-B). Importantly, although CDX2 cannot access adult-enriched target sites in the developmental context (Fig. 2A & 3A), ATAC-seq in Shh-Cre;CDX2f/f embryos at E16.5 revealed diminished chromatin accessibility at the vast majority of regions occupied by CDX2 at that developmental time point (Fig. S5C-D). Reduced chromatin access was specific to CDX2-bound regions, as chromatin accessibility at all annotated promoters was unchanged (Fig. S5D-E). Together, these data reveal that although chromatin accessibility directs CDX2 binding during endoderm development, CDX2 is required to sustain access at regions associated with adult intestinal genes, consistent with CDX2 control of enhancer chromatin structures in mature mice (Verzi et al., 2013). Thus, CDX2 acts in distinct developmental contexts, constrained in part by temporal chromatin landscapes, to promote tissue specification in embryos and essential digestive functions in adults.

Discussion

Pioneer factors help shape accessible chromatin (Iwafuchi-Doi and Zaret, 2016) and developmental signaling pathways and partner transcription factors prime chromatin structure to create a state of “developmental competence” (Wang et al., 2015). Our findings fit within this model, in that CDX2 is unable to bind condition-enriched binding sites (embryo or adult) outside of the proper developmental context. Our findings demonstrate that CDX2 is repurposed across the transitions in developmental competence: first CDX2 binds genes associated with developmental and specification functions, and subsequently CDX2 binds genes that promote the mature differentiated state in adults. The correlation between chromatin accessibility (Fig. 5), active histone modifications (Fig. S5), and CDX2 binding suggests that the chromatin environment is likely a critical factor in dictating condition-specific binding of CDX2. Our experiments with forced CDX2 expression in hESC-derived endoderm are similar to our findings in the mouse, with the observation CDX2 is not sufficient to access at many of its primary hindgut targets independently of the signaling environment. These findings are consistent with CDX2’s ability to pioneer certain binding sites in ES cells, while depending on accessible chromatin at others (Mahony et al., 2014). Alternatively, post-translational modifications, expression of transcriptional co-regulators, or other regulatory mechanisms likely function downstream of WNT and FGF signaling to create an environment in which CDX2 can access its hindgut target sites and impart intestinal identity. A similar set of regulatory mechanisms could govern the transition of CDX2 from Embryo-enriched binding sites to Adult-enriched binding sites (Figures 2-3) across critical developmental transitions (Figure 4B). CDX2 binding during intestinal specification is likely to rely upon pioneer factors, and motif analysis points to FoxA, a known pioneer factor (McPherson et al., 1993), as a likely candidate (Figure S3C). As yet unidentified chromatin regulators likely generate the corresponding competence for CDX2 occupancy and intestinal maturation as the intestinal chromatin landscape is altered in late gestation (Figure 5C). Our observations that CDX2 binding and chromatin access shift during development provide new insights into the molecular basis of intestinal maturation and indicate that mere expression of lineage regulators is insufficient to achieve desired tissue fates. Defining the factors that craft embryonic chromatin landscapes toward their mature forms will bolster efforts of regenerative medicine to accurately develop these tissues in vitro.

In models of Barrett’s esophagus, a predisposing condition of esophageal adenocarcinoma, CDX2 is unable to induce intestinal metaplasia simply by its lone ectopic expression in the foregut; pathologic changes are triggered only within the proper cellular context (Jiang et al., 2017; Silberg et al., 2002). This limitation is consistent with the mechanisms we report. CDX2 does not bind mouse adult-specific intestinal regions in early endoderm. Only after the epigenome is restructured late in gestation does CDX2 access adult-specific binding regions. Consistent with the observation that the intestinal chromatin landscape shifts late in development, loss of CDX2 in the adult mouse epithelium leads to a fetus-like transcriptome (Mustata et al., 2013), but not the early embryonic state permissive to homeotic transformation. CDX2 loss in early embryos permits such transformation in both mice and humans (Gao et al., 2009; Grainger et al., 2010), Figures 4A-B), likely because a distinct chromatin environment is present for a limited time. Defining whether and how chromatin accessibility is altered in instances of homeotic transformation upon prolonged loss of CDX2 in adult tissues (Simmini et al., 2014; Stringer et al., 2008) will be an important next step in understanding the mechanisms of lineage plasticity.

Materials and Methods

Mice

Shh-cre mice (Harfe et al., 2004) were purchased from Jackson Labs and male Shh-cre; Cdx2f/+ were bred to Cdx2 f/f female mice for inducing Cdx2 knockout (KO) in the developing intestine beginning at ~E9.5. Cre-negative embryos were used as littermate controls. Villin-CreERT2 (el Marjou et al., 2004) and CDX2f/f mice (Verzi et al., 2010) were previously described. Wild-type CD1 mice were obtained from Charles River Laboratories. All mouse protocols and experiments were approved by Rutgers Institutional Animal Care and Use Committee.

Key features of the methodologies are noted below and expanded upon in the supplemental methods.

Human pluripotent stem cell culture and differentiation

Human embryonic stem cells (line H9, WiCell Research Institute, NIH registration number 0062) were maintained and differentiated into endoderm, hindgut and intestinal organoids as published previously (Cruz-Acuna et al., 2017; Tsai et al., 2016; Tsai et al., 2017).

Histology, immunofluorescence and immunohistochemistry

Human organoids derived from stem cells (Spence et al., 2011) for 30 days were processed for immunofluorescence using antibodies (CDX2, Bio-Genex, MU392-UC, 1:500; MUC5AC, Abcam, ab79082, 1:500; NKX2.1, ThermoFisher, 8G7G3, 1:50; PDX1, Epitomics Inc, 3470-1 1:300; SOX2, Santa Cruz, sc-27603, 1:100). Mouse immunostaining was performed with following antibodies: CDX2 1:200, Cell Signaling, 12306; ATP4B 1:200, MBL International Corp., D032-3; TRP63 1:500, Santa Cruz Biotech, sc-8343.

Purification of Intestinal epithelial cells from mice

Single cells from dissected intestines were incubated with PE-conjugated anti-CD326 (EpCam clone G8.8, eBiosciences, 12-5791-81) and PE-stained cells were then incubated for ~30 minutes with magnetic conjugated anti-PE antibody (Miltenyi Biotec Anti-PE MicroBeads, 130-048-801) and isolated on a column (Miltenyi Biotec, MS Columns, 130-042-201) in a magnetic field to obtain magnetic antibody conjugated, EpCam positive epithelial cells.

ChIP-seq

For embryonic CDX2 ChIP-seq (E13.5, 12 embryos pooled per replicate; E16.5, 3 embryos pooled per replicate; and E17.5, 2 embryos pooled per replicate) midguts (caudal stomach to rostral caecum) were collected cells were isolated, fixed, and sonicated. Chromatin was incubated overnight with CDX2 antibody (6µl, Bethyl A300-691A) ChIP DNA was used to prepare ChIP-seq libraries using Rubicon Genomics ThruPLEX DNA-seq Kit (R400427/R400428/R40048), fragment size selected using Pippin Prep and sequenced on Illumina HiSeq.

ATAC-seq

25,000-50,000 isolated epithelial cells, from midguts (caudal stomach to rostral caecum, up to 2 embryos per sample) were used for ATAC-seq as described previously (Buenrostro et al., 2015).

RNA-seq

For E12.5 RNA-seq, total RNA was extracted from epcam-enriched epithelial cells (as described above) from gut tissue caudal to the stomach (2-5 embryos pooled per sample) in trizol using RNeasy micro kit (QIAGEN, 74004). RNA-seq libraries were prepared using the SMARTer-Seq v4 Low Input mRNA library kit (Clonetech SMARTer 634888). Adult RNA data were curated from GSE70766 and GSE98724 (San Roman et al., 2015; Saxena et al., 2017).

Computational analysis

Raw Sequencing reads (fastq) were quality checked using fastQC (v0.11.3), aligned to mouse (mm9) or human (hg19) genomes using Tophat2 (v2.1.0, RNA-seq) or bowtie2 (v2.2.6, ChIP- and ATAC-seq). For ChIP- and ATAC-seq, bam files were merged using samtools merge (0.1.19) for downstream analysis. Bigwigs were generated from bam files using deeptools bamCoverage v2.4.2, (Ramirez et al., 2014).

RNA-seq: Cxb files were generated using Cuffquant, normalized expression count tables were generated from cxb files using Cuffnorm (v2.2.1, library-norm-method quartile). Differential gene expression tables were computed using Cuffdiff (v2.2.1) and log2 fold change (FPKM+1) used for analysis.

For ChIP-seq and ATAC-seq: Peaks (bed file) were identified using MACS (1.4.1, Zhang et al., 2008). Two biological replicate ChIPs were performed for each condition, and replicates inspected by measuring Pearson correlation coefficients. Genes associated with ChIP peaks were identified using BETA minus and Enriched Motifs at ChIP peaks were identified using HOMER findMotifsGenome.pl (Heinz et al., 2010).

For comparing open chromatin regions (ATAC-seq) or differential CDX2 binding (ChIP-seq), bigwigs were generated (no normalization) and signal intensities were quantile normalized (v0.4.0, bin_size 50, log transformation) using Haystack (Pinello et al., 2018). k -means clustered heatmaps were generated from haystack normalized bigwigs using computeMatrix and plotHeatmap from deeptools package (v 2.4.2).

For ATAC-seq, two biological replicates from each developmental stage were performed, bam files were merged and bigwigs were quantile normalized to compare intensities of open chromatin signal. Embryonic and adult ChIP-seq data (Kazakevych et al., 2017) of the active chromatin marker (H3K27ac) was applied to Cdx2’s E13.5 and adult enriched genomic targets.

All RNA-seq, ATAC-seq, and ChIP-seq data generated in this study can be found at GEO with accession# GSE115314 (using reviewer code uvojyywmjnujtiz) and GSE115541 (reviewer code ozsryousxfexlqx).

Author Contributions

Conceptualization, MPV and JRS; Investigation, NK, YHT, LC, SH, KKB; Analysis, NK, LC, AZ, KKB, MS; Supervision, MPV, JRS, JX, RAS; Writing – Original Draft, NK and MPV; Writing – Reviewing and Editing, NK, MPV, JX, RAS, JRS.

Supplemental Tables

Table S1. Genome coordinates for CDX2-binding data from ChIP-seq performed in human hindgut (Hindgut-enriched sites) and Adult (Adult-enriched sites). Additionally, the results of HOMER motif-calling analysis on these sites enriched more specifically in the hindgut or adult are reported. Finally, the results of GO term enrichment using DAVID analysis for genes in proximity to these binding regions are reported. These data correspond to findings displayed in Figure 2.

Table S2. CDX2 binding data from ChIP-seq performed in Hindgut (Activin, WNT/FGF treatment protocol) versus Endoderm treated with Doxycycline (Activin, Doxycycline-CDX2). Binding coordinates of CDX2 sites found in both conditions (OverlapHindgutTetOn), sites more robustly bound by CDX2 in hindgut (HindgutEnriched), or sites more robustly bound by CDX2 when ectopically expressed in endoderm without the hindgut-inducing WNT/FGF-treatment (TetOnEnriched) are listed. Additionally, the results of motif-calling analysis of the sites enriched more specifically in the Tet-On or WNT/FGF treated condition are reported. These data correspond to findings displayed in Figure 2.

Table S3. Genome coordinates for CDX2-binding data from ChIP-seq performed in purified mouse intestinal epithelium at E13.5 (Embryo-enriched sites) and Adult (Adult-enriched sites). Additionally, the results of motif-calling analysis on these sites enriched more specifically in the mouse embryo or adult are reported. Finally, the results of GO term enrichment using GREAT analysis for genes in proximity to these binding regions are reported. These data correspond to the findings in Figure 3.

Acknowledgements

Research reported in this publication was supported by National Institute of Diabetes and Digestive and Kidney Disorders (NIDDK) and National Institute of Allergy and Infectious Diseases (NIAID) of the National Institutes of Health under grant number U01 DK103141 (MPV and JRS). The content is solely the responsibility of the authors and does not necessarily represent the official views of the National Institutes of Health. This work was also supported by the Human Genetics Institute of New Jersey; NIH grants R01 CA190558 (MPV), R01 DK082889 (RAS); the Biospecimen Repository Service Shared Resource and Sequencing Facility of the Rutgers Cancer Institute of New Jersey (P30CA072720); and the University of Michigan Center for Gastrointestinal Research (UMCGR) (NIDDK 5P30DK034933).

References

  1. ↵
    Babeu, J. P., Darsigny, M., Lussier, C. R. and Boudreau, F. (2009). Hepatocyte nuclear factor 4alpha contributes to an intestinal epithelial phenotype in vitro and plays a partial role in mouse intestinal epithelium differentiation. Am J Physiol Gastrointest Liver Physiol 297, G124–134.
    OpenUrlCrossRefPubMedWeb of Science
  2. Beck, F., Chawengsaksophak, K., Luckett, J., Giblett, S., Tucci, J., Brown, J., Poulsom, R., Jeffery, R. and Wright, N. A. (2003). A study of regional gut endoderm potency by analysis of Cdx2 null mutant chimaeric mice. Dev Biol 255, 399–406.
    OpenUrlCrossRefPubMed
  3. Beck, F., Chawengsaksophak, K., Waring, P., Playford, R. J. and Furness, J. B. (1999). Reprogramming of intestinal differentiation and intercalary regeneration in Cdx2 mutant mice. Proc Natl Acad Sci USA 96, 7318–7323.
    OpenUrlAbstract/FREE Full Text
  4. ↵
    Bell, S. M., Schreiner, C. M., Wert, S. E., Mucenski, M. L., Scott, W. J. and Whitsett, J. A. (2008). R-spondin 2 is required for normal laryngeal-tracheal, lung and limb morphogenesis. Development 135, 1049–1058.
    OpenUrlAbstract/FREE Full Text
  5. ↵
    Buenrostro, J. D., Wu, B., Chang, H. Y. and Greenleaf, W. J. (2015). ATAC-seq: A Method for Assaying Chromatin Accessibility Genome-Wide. Curr Protoc Mol Biol 109, 21 29 21–29.
    OpenUrlCrossRef
  6. ↵
    Cattin, A. L., Le Beyec, J., Barreau, F., Saint-Just, S., Houllier, A., Gonzalez, F. J., Robine, S., Pincon-Raymond, M., Cardot, P., Lacasa, M., et al. (2009). Hepatocyte nuclear factor 4alpha, a key factor for homeostasis, cell architecture, and barrier function of the adult intestinal epithelium. Mol Cell Biol 29, 6294–6308.
    OpenUrlAbstract/FREE Full Text
  7. ↵
    Chawengsaksophak, K., James, R., Hammond, V. E., Kontgen, F. and Beck, F. (1997). Homeosis and intestinal tumours in Cdx2 mutant mice. Nature 386, 84–87.
    OpenUrlCrossRefPubMed
  8. ↵
    Chen, Y. J., Finkbeiner, S. R., Weinblatt, D., Emmett, M. J., Tameire, F., Yousefi, M., Yang, C., Maehr, R., Zhou, Q., Shemer, R., et al. (2014). De novo formation of insulin-producing "neo-beta cell islets" from intestinal crypts. Cell reports 6, 1046–1058.
    OpenUrl
  9. ↵
    Cruz-Acuna, R., Quiros, M., Farkas, A. E., Dedhia, P. H., Huang, S., Siuda, D., Garcia-Hernandez, V., Miller, A. J., Spence, J. R., Nusrat, A., et al. (2017). Synthetic hydrogels for human intestinal organoid generation and colonic wound repair. Nat Cell Biol 19, 1326–1335.
    OpenUrlCrossRef
  10. ↵
    D’Amour, K. A., Agulnick, A. D., Eliazer, S., Kelly, O. G., Kroon, E. and Baetge, E. E. (2005). Efficient differentiation of human embryonic stem cells to definitive endoderm. Nat Biotechnol 23, 1534–1541.
    OpenUrlCrossRefPubMedWeb of Science
  11. ↵
    Davis, R. L., Weintraub, H. and Lassar, A. B. (1987). Expression of a single transfected cDNA converts fibroblasts to myoblasts. Cell 51, 987–1000.
    OpenUrlCrossRefPubMedWeb of Science
  12. ↵
    el Marjou, F., Janssen, K. P., Chang, B. H., Li, M., Hindie, V., Chan, L., Louvard, D., Chambon, P., Metzger, D. and Robine, S. (2004). Tissue-specific and inducible Cre-mediated recombination in the gut epithelium. Genesis 39, 186–193.
    OpenUrlCrossRefPubMedWeb of Science
  13. ↵
    Finkbeiner, S. R., Hill, D. R., Altheim, C. H., Dedhia, P. H., Taylor, M. J., Tsai, Y. H., Chin, A. M., Mahe, M. M., Watson, C. L., Freeman, J. J., et al. (2015). Transcriptome-wide Analysis Reveals Hallmarks of Human Intestine Development and Maturation In Vitro and In Vivo. Stem Cell Reports.
  14. ↵
    Gao, N., White, P. and Kaestner, K. H. (2009). Establishment of intestinal identity and epithelial-mesenchymal signaling by Cdx2. Dev Cell 16, 588–599.
    OpenUrlCrossRefPubMedWeb of Science
  15. ↵
    Grainger, S., Savory, J. G. and Lohnes, D. (2010). Cdx2 regulates patterning of the intestinal epithelium. Dev Biol In Press.
  16. ↵
    Harfe, B. D., Scherz, P. J., Nissim, S., Tian, H., McMahon, A. P. and Tabin, C. J. (2004). Evidence for an expansion-based temporal Shh gradient in specifying vertebrate digit identities. Cell 118, 517–528.
    OpenUrlCrossRefPubMedWeb of Science
  17. ↵
    Heijmans, J., van Lidth de Jeude, J. F., Koo, B. K., Rosekrans, S. L., Wielenga, M. C., van de Wetering, M., Ferrante, M., Lee, A. S., Onderwater, J. J., Paton, J. C., et al. (2013). ER stress causes rapid loss of intestinal epithelial stemness through activation of the unfolded protein response. Cell reports 3, 1128–1139.
    OpenUrl
  18. ↵
    Heinz, S., Benner, C., Spann, N., Bertolino, E., Lin, Y. C., Laslo, P., Cheng, J. X., Murre, C., Singh, H. and Glass, C. K. (2010). Simple combinations of lineage-determining transcription factors prime cis-regulatory elements required for macrophage and B cell identities. Mol Cell 38, 576–589.
    OpenUrlCrossRefPubMedWeb of Science
  19. ↵
    Hryniuk, A., Grainger, S., Savory, J. G. and Lohnes, D. (2012). Cdx function is required for maintenance of intestinal identity in the adult. Dev Biol 363, 426–437.
    OpenUrlCrossRefPubMed
  20. ↵
    Huang da, W., Sherman, B. T. and Lempicki, R. A. (2009). Systematic and integrative analysis of large gene lists using DAVID bioinformatics resources. Nature protocols 4, 44–57.
    OpenUrl
  21. ↵
    Iwafuchi-Doi, M. and Zaret, K. S. (2016). Cell fate control by pioneer transcription factors. Development 143, 1833–1837.
    OpenUrlAbstract/FREE Full Text
  22. ↵
    Jiang, M., Li, H., Zhang, Y., Yang, Y., Lu, R., Liu, K., Lin, S., Lan, X., Wang, H., Wu, H., et al. (2017). Transitional basal cells at the squamous-columnar junction generate Barrett’s oesophagus. Nature 550, 529–533.
    OpenUrlCrossRef
  23. ↵
    Jonsson, J., Carlsson, L., Edlund, T. and Edlund, H. (1994). Insulin-promoter-factor 1 is required for pancreas development in mice. Nature 371, 606–609.
    OpenUrlCrossRefPubMedWeb of Science
  24. ↵
    Kanai-Azuma, M., Kanai, Y., Gad, J. M., Tajima, Y., Taya, C., Kurohmaru, M., Sanai, Y., Yonekawa, H., Yazaki, K., Tam, P. P., et al. (2002). Depletion of definitive gut endoderm in Sox17-null mutant mice. Development 129, 2367–2379.
    OpenUrlPubMedWeb of Science
  25. ↵
    Kazakevych, J., Sayols, S., Messner, B., Krienke, C. and Soshnikova, N. (2017). Dynamic changes in chromatin states during specification and differentiation of adult intestinal stem cells. Nucleic Acids Res 45, 5770–5784.
    OpenUrlCrossRef
  26. ↵
    Leslie, J. L., Huang, S., Opp, J. S., Nagy, M. S., Kobayashi, M., Young, V. B. and Spence, J. R. (2015). Persistence and toxin production by Clostridium difficile within human intestinal organoids result in disruption of epithelial paracellular barrier function. Infect Immun 83, 138–145.
    OpenUrlAbstract/FREE Full Text
  27. ↵
    Mahony, S., Edwards, M. D., Mazzoni, E. O., Sherwood, R. I., Kakumanu, A., Morrison, C. A., Wichterle, H. and Gifford, D. K. (2014). An integrated model of multiple-condition ChIP-Seq data reveals predeterminants of Cdx2 binding. PLoS Comput Biol 10, e1003501.
    OpenUrlCrossRefPubMed
  28. ↵
    McCracken, K. W., Howell, J. C., Wells, J. M. and Spence, J. R. (2011). Generating human intestinal tissue from pluripotent stem cells in vitro. Nature protocols 6, 1920–1928.
    OpenUrl
  29. ↵
    McLean, C. Y., Bristor, D., Hiller, M., Clarke, S. L., Schaar, B. T., Lowe, C. B., Wenger, A. M. and Bejerano, G. (2010). GREAT improves functional interpretation of cis-regulatory regions. Nat Biotechnol 28, 495–501.
    OpenUrlCrossRefPubMedWeb of Science
  30. ↵
    McPherson, C. E., Shim, E. Y., Friedman, D. S. and Zaret, K. S. (1993). An active tissue-specific enhancer and bound transcription factors existing in a precisely positioned nucleosomal array. Cell 75, 387–398.
    OpenUrlCrossRefPubMedWeb of Science
  31. ↵
    Meerbrey, K. L., Hu, G., Kessler, J. D., Roarty, K., Li, M. Z., Fang, J. E., Herschkowitz, J. I., Burrows, A. E., Ciccia, A., Sun, T., et al. (2011). The pINDUCER lentiviral toolkit for inducible RNA interference in vitro and in vivo. Proc Natl Acad Sci U S A 108, 3665–3670.
    OpenUrlAbstract/FREE Full Text
  32. ↵
    Mustata, R. C., Vasile, G., Fernandez-Vallone, V., Strollo, S., Lefort, A., Libert, F., Monteyne, D., Perez-Morga, D., Vassart, G. and Garcia, M. I. (2013). Identification of Lgr5-independent spheroid-generating progenitors of the mouse fetal intestinal epithelium. Cell reports 5, 421–432.
    OpenUrl
  33. ↵
    Offield, M. F., Jetton, T. L., Labosky, P. A., Ray, M., Stein, R. W., Magnuson, M. A., Hogan, B. L. and Wright, C. V. (1996). PDX-1 is required for pancreatic outgrowth and differentiation of the rostral duodenum. Development 122, 983–995.
    OpenUrlAbstract
  34. ↵
    Pinello, L., Farouni, R. and Yuan, G. C. (2018). Haystack: systematic analysis of the variation of epigenetic states and cell-type specific regulatory elements. Bioinformatics 34, 1930–1933.
    OpenUrlCrossRef
  35. ↵
    Ramirez, F., Dundar, F., Diehl, S., Gruning, B. A. and Manke, T. (2014). deepTools: a flexible platform for exploring deep-sequencing data. Nucleic Acids Res 42, W187–191.
    OpenUrlCrossRefPubMedWeb of Science
  36. ↵
    Robinson, J. T., Thorvaldsdottir, H., Winckler, W., Guttman, M., Lander, E. S., Getz, G. and Mesirov, J. P. (2011). Integrative genomics viewer. Nat Biotechnol 29, 24–26.
    OpenUrlCrossRefPubMedWeb of Science
  37. ↵
    San Roman, A. K., Aronson, B. E., Krasinski, S. D., Shivdasani, R. A. and Verzi, M. P. (2015). Transcription factors GATA4 and HNF4A control distinct aspects of intestinal homeostasis in conjunction with transcription factor CDX2. J Biol Chem 290, 1850–1860.
    OpenUrlAbstract/FREE Full Text
  38. ↵
    Saxena, M., Roman, A. K. S., O’Neill, N. K., Sulahian, R., Jadhav, U. and Shivdasani, R. A. (2017). Transcription factor-dependent ‘anti-repressive’ mammalian enhancers exclude H3K27me3 from extended genomic domains. Genes Dev 31, 2391–2404.
    OpenUrlAbstract/FREE Full Text
  39. ↵
    Silberg, D. G., Sullivan, J., Kang, E., Swain, G. P., Moffett, J., Sund, N. J., Sackett, S. D. and Kaestner, K. H. (2002). Cdx2 ectopic expression induces gastric intestinal metaplasia in transgenic mice. Gastroenterology 122, 689–696.
    OpenUrlCrossRefPubMedWeb of Science
  40. ↵
    Simmini, S., Bialecka, M., Huch, M., Kester, L., van de Wetering, M., Sato, T., Beck, F., van Oudenaarden, A., Clevers, H. and Deschamps, J. (2014). Transformation of intestinal stem cells into gastric stem cells on loss of transcription factor Cdx2. Nat Commun 5, 5728.
    OpenUrlCrossRefPubMed
  41. ↵
    Spence, J. R., Mayhew, C. N., Rankin, S. A., Kuhar, M. F., Vallance, J. E., Tolle, K., Hoskins, E. E., Kalinichenko, V. V., Wells, S. I., Zorn, A. M., et al. (2011). Directed differentiation of human pluripotent stem cells into intestinal tissue in vitro. Nature 470, 105–109.
    OpenUrlCrossRefPubMedWeb of Science
  42. ↵
    Stegmann, A., Hansen, M., Wang, Y., Larsen, J. B., Lund, L. R., Ritie, L., Nicholson, J. K., Quistorff, B., Simon-Assmann, P., Troelsen, J. T., et al. (2006). Metabolome, transcriptome, and bioinformatic cis-element analyses point to HNF-4 as a central regulator of gene expression during enterocyte differentiation. Physiol Genomics 27, 141–155.
    OpenUrlCrossRefPubMedWeb of Science
  43. ↵
    Stringer, E. J., Duluc, I., Saandi, T., Davidson, I., Bialecka, M., Sato, T., Barker, N., Clevers, H., Pritchard, C. A., Winton, D. J., et al. (2012). Cdx2 determines the fate of postnatal intestinal endoderm. Development 139, 465–474.
    OpenUrlAbstract/FREE Full Text
  44. ↵
    Stringer, E. J., Pritchard, C. A. and Beck, F. (2008). Cdx2 initiates histodifferentiation of the midgut endoderm. FEBS Lett 582, 2555–2560.
    OpenUrlCrossRefPubMed
  45. ↵
    Subramanian, A., Tamayo, P., Mootha, V. K., Mukherjee, S., Ebert, B. L., Gillette, M. A., Paulovich, A., Pomeroy, S. L., Golub, T. R., Lander, E. S., et al. (2005). Gene set enrichment analysis: a knowledge-based approach for interpreting genome-wide expression profiles. Proc Natl Acad Sci U S A 102, 15545–15550.
    OpenUrlAbstract/FREE Full Text
  46. ↵
    Tamai, Y., Nakajima, R., Ishikawa, T., Takaku, K., Seldin, M. F. and Taketo, M. M. (1999). Colonic hamartoma development by anomalous duplication in Cdx2 knockout mice. Cancer Res 59, 2965–2970.
    OpenUrlAbstract/FREE Full Text
  47. ↵
    Tapscott, S. J., Davis, R. L., Thayer, M. J., Cheng, P. F., Weintraub, H. and Lassar, A. B. (1988). MyoD1: a nuclear phosphoprotein requiring a Myc homology region to convert fibroblasts to myoblasts. Science 242, 405–411.
    OpenUrlAbstract/FREE Full Text
  48. ↵
    Tsai, Y. H., Hill, D. R., Kumar, N., Huang, S., Chin, A. M., Dye, B. R., Nagy, M. S., Verzi, M. P. and Spence, J. R. (2016). LGR4 and LGR5 Function Redundantly During Human Endoderm Differentiation. Cell Mol Gastroenterol Hepatol 2, 648–662 e648.
    OpenUrl
  49. ↵
    Tsai, Y. H., Nattiv, R., Dedhia, P. H., Nagy, M. S., Chin, A. M., Thomson, M., Klein, O. D. and Spence, J. R. (2017). In vitro patterning of pluripotent stem cell-derived intestine recapitulates in vivo human development. Development 144, 1045–1055.
    OpenUrlAbstract/FREE Full Text
  50. ↵
    Verzi, M. P., Shin, H., He, H. H., Sulahian, R., Meyer, C. A., Montgomery, R. K., Fleet, J. C., Brown, M., Liu, X. S. and Shivdasani, R. A. (2010). Differentiation-specific histone modifications reveal dynamic chromatin interactions and partners for the intestinal transcription factor CDX2. Dev Cell 19, 713–726.
    OpenUrlCrossRefPubMedWeb of Science
  51. ↵
    Verzi, M. P., Shin, H., Ho, L. L., Liu, X. S. and Shivdasani, R. A. (2011). Essential and redundant functions of caudal family proteins in activating adult intestinal genes. Mol Cell Biol 31, 2026–2039.
    OpenUrlAbstract/FREE Full Text
  52. ↵
    Verzi, M. P., Shin, H., San Roman, A. K., Liu, X. S. and Shivdasani, R. A. (2013). Intestinal master transcription factor CDX2 controls chromatin access for partner transcription factor binding. Mol Cell Biol 33, 281–292.
    OpenUrlAbstract/FREE Full Text
  53. ↵
    Wang, A., Yue, F., Li, Y., Xie, R., Harper, T., Patel, N. A., Muth, K., Palmer, J., Qiu, Y., Wang, J., et al. (2015). Epigenetic priming of enhancers predicts developmental competence of hESC-derived endodermal lineage intermediates. Cell Stem Cell 16, 386–399.
    OpenUrlCrossRefPubMed
  54. ↵
    Wells, J. M. and Melton, D. A. (2000). Early mouse endoderm is patterned by soluble factors from adjacent germ layers. Development 127, 1563–1572.
    OpenUrlAbstract
  55. ↵
    Young, T., Rowland, J. E., van de Ven, C., Bialecka, M., Novoa, A., Carapuco, M., van Nes, J., de Graaff, W., Duluc, I., Freund, J. N., et al. (2009). Cdx and Hox genes differentially regulate posterior axial growth in mammalian embryos. Dev Cell 17, 516–526.
    OpenUrlCrossRefPubMedWeb of Science
  56. ↵
    Zhang, Y., Liu, T., Meyer, C. A., Eeckhoute, J., Johnson, D. S., Bernstein, B. E., Nussbaum, C., Myers, R. M., Brown, M., Li, W., et al. (2008). Model-based analysis of ChIP-Seq (MACS). Genome Biol 9, R137.
    OpenUrlCrossRefPubMed
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Posted September 24, 2018.
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The Lineage-Specific Transcription Factor CDX2 Navigates Dynamic Chromatin to Control Distinct Stages of Intestine Development
Namit Kumar, Yu-Hwai Tsai, Lei Chen, Anbo Zhou, Kushal K. Banerjee, Madhurima Saxena, Sha Huang, Jinchuan Xing, Ramesh A. Shivdasani, Jason R. Spence, Michael P. Verzi
bioRxiv 425827; doi: https://doi.org/10.1101/425827
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