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Author contributions: C.M.M.: collection and/or assembly of data, data analysis and interpretation, and manuscript writing, Y.G. and T. N.: collection and/or assembly of data and data analysis and interpretation; A.M.T.: provision of study material or patients and collection and/or assembly of data; J.C. and K.H.: collection and/or assembly of data; E.C.: provision of study material or patients; D.S.K.: provision of study material or patients and manuscript writing; J.L.: conception and design, financial support, data analysis and interpretation, and manuscript writing; S.G.: conception and design, financial support, collection and/or assembly of data, data analysis and interpretation, manuscript writing, and final approval of manuscript.
Disclosure of potential conflicts of interest is found at the end of this article.
First published online in STEM CELLSEXPRESS January 17, 2013.
Discovery of the cellular and molecular mechanisms of induced pluripotency has been hampered by its low efficiency and slow kinetics. Here, we report an experimental system with multicolor time-lapse microscopy that permits direct observation of pluripotency induction at single cell resolution, with temporal intervals as short as 5 minutes. Using granulocyte-monocyte progenitors as source cells, we visualized nascent pluripotent cells that emerge from a hematopoietic state. We engineered a suite of image processing and analysis software to annotate the behaviors of the reprogramming cells, which revealed the highly dynamic cell-cell interactions associated with early reprogramming. We observed frequent cell migration, which can lead to sister colonies, satellite colonies, and colonies of mixed genetic makeup. In addition, we discovered a previously unknown morphologically distinct two-cell intermediate of reprogramming, which occurs prior to other reprogramming landmarks. By directly visualizing the reprogramming process with E-cadherin inhibition, we demonstrate that E-cadherin is required for proper cellular interactions from an early stage of reprogramming, including the two-cell intermediate. The detailed cell-cell interactions revealed by this imaging platform shed light on previously unappreciated early reprogramming dynamics. This experimental system could serve as a powerful tool to dissect the complex mechanisms of early reprogramming by focusing on the relevant but rare cells with superb temporal and spatial resolution. STEM CELLS 2013;31:895–905
The discovery of induced pluripotent stem cells (iPSCs) [1–4] has made a profound conceptual impact on many biomedical disciplines, putting forward the hope to derive patient-specific therapeutic cell types and to study human diseases that had been previously difficult to model. Indeed, many somatic cell types can be reprogrammed to pluripotency by forced expression of defined factors such as Oct4, Sox2, Klf4, and c-Myc (OSKM). However, this process generally takes a long time and the cells undergoing successful reprogramming are rare [5, 6]. Due to this inherent slow kinetics and inefficiency, mechanistic studies have relied on analyzing the bulk cell cultures, among which the relevant cells are the minority. Furthermore, even with the help of pluripotency reporters such as Oct-4-GFP or Nanog-GFP [7, 8], assessment of reprogramming can only be made with cells that are already in the late reprogramming phase. Very little is known about the early cellular and molecular events preceding activation of the endogenous pluripotency circuitry .
Direct observation, using time-lapse microscopy has been an important approach to define the molecular and cellular events during early reprogramming [10–13]. However, the utility of these approaches has been compromised by one or more of the following technical limitations. (a) The imaging intervals are long (such as 6 hours or longer) and faithful single cell tracking can be difficult [11, 12]. Cellular events that occur faster than this temporal resolution are not detectable. (b) Constitutive iPS factor expression precludes accurate determination of the onset for factor action, which creates difficulty in identifying the initial founder cells of reprogrammed colonies [10, 11, 13]. (c) The slow kinetics of the reprogramming process (1–2 weeks) either requires medium change during imaging  or constrains imaging to a limited time window (e.g., from day 4.5 ). Medium change can disturb imaging continuity  as well as the local extracellular environment and may physically dislodge cells and generate secondary colonies. (d) Monitoring pluripotency by colony morphology or post-reprogramming staining [11, 12] does not allow real time visualization of the milestones of reprogramming.
Here, we describe an experimental method which overcomes many of the limitations and provides fine temporal and graphical details of early reprogramming. Hematopoietic cells have been often used as source cells to model and reveal reprogramming mechanisms [7, 8]. In particular, we used a well-characterized hematopoietic progenitor population, the granulocyte-monocyte progenitors (GMPs), as source cells for reprogramming since they have been meticulously defined both phenotypically and functionally , can be prospectively isolated to high purity, and support reprogramming with high efficiency . We found that highly dynamic cell migration occurs leading to the formation of sister colonies, satellite colonies, or mixed colonies containing cells of different genetic makeup. We report a two-cell intermediate stage that is characterized by a unique dumbbell-like morphology and induction of intracellular E-cadherin at this early stage. In addition, we demonstrate the feasibility of our system to accommodate additional reporters for interrogation of specific genetic effects during reprogramming by capturing perturbed reprogramming when E-cadherin is knocked down with short hairpin RNA (shRNA). Overall, this system provides a powerful tool to dissect the molecular and cellular mechanisms involved in factor-based pluripotency induction.
MATERIALS AND METHODS
Mouse Maintenance and Blastocyst Injection
The Oct-4-GFP:Rosa26-rtTA mice were derived by crossing Oct4-GFP mice with Rosa26-rtTA mice as described . The tet-O-Cre mice and E-cadherinfl/fl mice were purchased from the Jackson Laboratory (Bar Harbor, Maine, http://www.jax.org) and further crossed with the Rosa26-rtTA mice to achieve doxycycline (dox) inducible inactivation of E-cadherin. All mouse work was approved by the Institutional Animal Care and Use Committee of Yale University.
GMP-derived, dox independent, green fluorescent protein (GFP+) cells with typical embryonic stem cell (ESC) morphology were used for karyotype analysis by standard methods using Wright's stain with 20 spreads counted per iPSC clone. For blastocyst injection, iPSCs were passaged in 2i medium [15, 16] supplemented with leukemia inhibitory factor (LIF) two to three times prior to injection. C57Bl/6Tyrc-2J blastocysts were microinjected with 12–15 iPSCs per blast via standard methods . Injected embryos were transferred to uteri of pseudopregnant CD-1 females as described . Chimeras were measured by % agouti and black on the albino background provided by the host blastocyst. Male chimeras were mated to C57Bl/6Tyrc-2J females, and germline transmission was assessed by observation of agouti coat color.
Cell Culture, Lentivirus Production and Transduction
For reprogramming source cells, mouse embryonic fibroblasts (MEFs) were prepared from day 13.5 embryos of the Oct-4 GFP mice and reprogrammed as described . Wild-type C57Bl6 mouse ESCs (mESCs) were purchased from ATCC and transduced with retrovirus vectors expressing GFP or dsRed as described previously .
For feeder cells, MEFs were derived from CF1 mice or purchased from Millipore (Billerica, MA, http://www.millipore.com). P3 MEFs were inactivated by 2 hour treatment of mitomycin C. Inactivated MEFs were plated on gelatinized dishes and used within 2 days. Lentivirus production was performed as described by the RNAi Consortium at the Broad Institute (http://www.broadinstitute.org/rnai/public/static/protocols/TRC_Protocols_Section_II_Viral_Production_100809.pdf). Lentiviral constructs for shRNAs against E-Cadherin are generous gifts from Dr. N. Geijsen . Hematopoietic progenitor cells were transduced in X VIVO15 medium supplemented with 100 ng/ml murine Stem cell factor (mSCF), 50 ng/ml murine Interleukin 3 (mIL3), 50 ng/ml murine Fms-related tyrosine kinase 3 ligand (Flt3L), and 50 ng/ml murine Thrombopoietin (mTPO) (all from PeproTech, Rocky Hill, NJ, http://www.peprotech.com) supplemented with 4 μg/ml polybrene overnight, washed in PBS, and plated on inactivated MEF feeders at a density of 20,000–50,000 cells per 35 mm dish in complete mESC culture medium (Dulbecco's modified Eagle's medium [DMEM] with 15% Hyclone FBS, nonessential amino-acids, Pen/Strep, L-glutamine, β-mercaptoethanol, and 1,000 U/ml LIF [Billerica, MA, http://www.millipore.com]). Dox was added at 2 μg/ml to induce factor expression.
Fluorescence-Activated Cell Sorting Purification of GMPs
GMPs were stained and fluorescence-activated cell sorted on a BD Aria instrument as described previously [14, 18]. Briefly, mouse bone marrow cells were stained with antibody cocktail containing hematopoietic lineages antibodies, c-Kit allophycocyanin (APC), Sca phycoerythrin (PE) or pacific blue, CD34 fluorescein isothiocyanate (FITC) and CD16/32 PEcy7 (all from BD Biosciences, San Jose, http://www.bdbiosciences.com or eBiosciences). GMPs are defined as lineage negative, c-Kit positive, Sca negative, CD34 and CD16/32 double positive.
Immunofluorescent Staining and Confocal Analysis
The iPSC induction procedure is described as above. Starting from 24 hours after dox addition, cultures in 35 mm dishes were processed for immunostaining every 12 hours by fixation with 3.7% formaldehyde for 15 minutes, and permeabilization with 0.1% Triton X-100 (Sigma-Aldrich, St. Louis, http://www.sigmaaldrich.com) for 15 minutes. Fixed cells were maintained in phosphate buffered saline (PBS) at 4°C before further processing. After all time points were collected, the cultures were stained at the same time with rabbit anti-E-Cadherin antibody (1:200, Cell Signaling, Beverly, MA, http://www.cellsignal.com). Bound antibody was detected using Alexa-555 or Alexa-488 labeled donkey anti-rabbit secondary antibody (Invitrogen, Carlsbad, CA, http://www.invitrogen.com). Fluorescent images were obtained on a Leica SP5 confocal microscope (Leica microsystem, Wetzlar, Germany).
Image Acquisition and Analysis
For all imaging studies, mitomycin C-inactivated MEFs were plated on gelatinized dishes with enhanced optical properties (ibidi) on the day of GMP cell sorting. GMPs following overnight viral transduction were washed and plated on the MEF layer and placed in a VivaView Olympus incubator microscope with motorized stage. Images were acquired by the Metamorph software at defined time intervals with signals being recorded in the differential interference contrast (DIC), GFP, and/or RFP channels with 10× or 20× magnification continuously for 3–5 days.
In some cases, when stitching was not necessary, Metamorph was used to annotate the images and generate movies. In most other cases, TIF images from the VivaView microscope were analyzed with the assistance of a custom suite of programs coded in Matlab, which has user friendly graphical interfaces (Supporting Information Fig. S3). Several steps were taken to process the images. First, to correct for vignetting, background illumination images for each scanning position and each channel were calculated by taking the median values of 60–80 time points (user-definable) at each pixel. Vignetting was corrected by dividing raw TIF images with the background illumination images. Second, images with adjacent positions were stitched together (up to 10 by 10). Stitching overlaps between neighboring images were calculated by minimizing the signal difference of the overlapping areas from the DIC channel of neighboring background-corrected images. The same stitching parameters were then applied to all light channels of the corresponding scanning positions. In the stitched images, overlap areas were represented by the mean of signals from neighboring images. Third, images from different light channels were mixed to create pseudocolor images. User is able to control the background and saturation of each channel, and the fraction by which each channel will be displayed in red, green, and blue channels of the final pseudocolor image. To ensure accuracy of tracing, all iPSC lineages were inspected manually and annotated using a custom program coded in Matlab (Supporting Information Fig. S3B). For all movies, the first time points were stamped as +1 than real time such that they start as 00:30 minute, 00:15 minute, and 00:05 for images acquired at 30 minute, 15 minute, and 5 minute intervals. For still images, the first time points were stamped as 00:00.
GMPs As a Suitable Cell Source for Time-Lapse Imaging
We sought to establish a reprogramming system that is fast, efficient, inducible, and contains a marker for the activation of endogenous pluripotency circuitry . Importantly, the cells undergoing reprogramming should be clearly distinguishable from other cells present in the culture. We focused our attention on GMPs since they are well-defined, can be prospectively isolated to high purity , and support reprogramming with sufficiently high efficiency  (5%–10% apparent efficiency in our hands). We purified GMPs from mice genetically modified to express an Oct-4-GFP reporter as well as a universally expressed (Rosa26) reverse transactivator rtTA  (Supporting Information Fig. S1). Following cell sorting, GMPs were infected with a polycistronic lentivirus encoding doxycycycline (dox) inducible expression of the transcription factors OSKM, plated on feeder cells, and induced to initiate reprogramming by adding dox. Oct-4-GFP+ colonies with ESC-like morphology appeared within the first 3 days following dox addition (Fig. 1A). During this time, the number of cells present in the culture remains limited (<100,000 hematopoietic cells per 35 mm dish containing 3.5 ml of medium) and medium change was not necessary. By 5 days, many of the colonies had grown to large sizes such that passaging was usually required (Fig. 1B). When left without passaging (but with medium change) until day 8, many colonies displayed differentiation-associated changes (Fig. 1C). On day 5 post dox addition, primary GMPs routinely give rise to >5 colonies for every 100 initial cells. The colonies could become dox-independent and be propagated with murine ESC culture conditions. The cells within the colonies have normal karyotypes (data not shown), support high degree chimeric mouse formation and are capable of germline transmission (Fig. 1D), demonstrating their pluripotency.
In addition to fast kinetics and high efficiency, GMP-based reprogramming displays unique imaging-friendly qualities. First, the developing Oct4-GFP+ cell clusters do not seem to contain Oct-4-GFP negative cells (Fig. 1A, 1B, 1E). Partially GFP+ cell clusters are prominent when fibroblasts are used as source cells and are thought to represent various reprogramming intermediates or partially reprogrammed cells [10, 13]. We examined thousands of GMP-derived colonies and have never encountered any colony that had a mixture of Oct-4-GFP positive and negative cells, as long as the cells were not differentiated due to overgrowth (Fig. 1C, red arrows). Figure 1E shows a typical field on a reprogramming culture dish. All colonies with ESC morphology are GFP positive and vice versa. This is true even for very small, nascent colonies (Fig. 1A). Another imaging-friendly feature of GMP is that the cells that are not being reprogrammed retain their round morphology (Fig. 1A, red arrows). Thus, the morphological changes associated with entry into early reprogramming are visually distinct.
Together, these key features indicate that GMP-based reprogramming system is well suited for imaging experiments. We thus performed all subsequent time-lapse experiments using this system.
High Temporal Resolution Microscopy Enables Tracing of Reprogrammed Colonies to Single Founder Cells
We used an incubator-enclosed microscope with a motorized stage, which permits continuous scanning and photographing of partially overlapping visual fields. These fields were stitched together in post experiment analysis, synthesizing a large area sufficient for capturing low-frequency reprogramming events (Supporting Information Fig. S2; Fig. 2A). In addition, the imaging system records signals from DIC, GFP and additional channels when necessary. Through a 10× or 20× objective lens, the resulting images are of high optical resolution and provide fine cellular details (Fig. 2A). Time-lapse microscopy for this entire synthetic field continues for 3–5 days at 5–30-minute intervals (Supporting Information Movie S1). We initiate image acquisition approximately 1 hour after adding dox (time required to stabilize and equilibrate the imaging system). Given that the polycistronic iPS vector needs time to produce RNA and protein after adding dox, this experimental scheme ensures that we capture the very beginning of the reprogramming process.
For image processing, analysis, and annotation, we created a suite of user-friendly computational tools (Supporting Information Fig. S3). During image analysis, we tracked cell movement from Oct-4-GFP+ colonies back in time to a single cell. This is made possible by the ability of the imaging system to capture cell migratory and divisional events at high frequency (every 5–15 minutes), generating reliable accounts for the origin of every emerging cell in view. Many of the reprogramming lineages allowed us to trace back to a single cell at the beginning of image acquisition (Fig. 2B; Supporting Information Movie S2) when factor induction in these hematopoietic cells had occurred for just 1 hour. We define these single cells as “founder” cells. It is important to note that our definition of the founder cells is much more stringent than traceable single progenitors (or ancestors) used in previous methods. For example, a previous study tracked back to single cell progenitors in the middle of reprogramming , after 4.5 days of factor transduction. In such cases, it was difficult to determine the identity of these cells as factor expression had been on for an extended time. Cellular events that happened before this traceable progenitor stage would have been missed.
Given the fast reprogramming kinetics and high efficiency, lack of Oct-4 GFP negative cells in the cell clusters, timed factor expression, and unique cellular morphology, our experimental system is a significant improvement over previous methodologies to characterize the early reprogramming process.
Dynamic Cellular and Clonal Behaviors During Early Reprogramming
Time-lapse observation shows that the cells, either singularly or as cell clusters, display active migratory behavior during the entire imaged process (Supporting Information Movies S1, S2). For example, single cells appeared to roll on top of the feeder cells, which themselves underwent constant morphologic remodeling. The migratory motions appeared to be random in terms of direction, duration, and distance but were widespread and often brought distant cells together. Such migratory behaviors predict that two remote cells and/or colonies could come together resulting in clonal mixing, which can be affected by the local density of migratory cells.
Tracking lineage pedigrees revealed that many of the colonies formed are indeed not clonal, but rather contained cells of different reprogramming origins, including from different founder cells (Fig. 3; Supporting Information Movie S3). To overcome any potential ambiguity associated with tracing single cells, we plated factor transduced GMPs from Rosa26-rtTA mice with or without the Oct-4 GFP reporter. As discussed earlier, all reprogrammed colonies from the Oct-4 GFP reporter-containing GMPs are GFP+. Thus, such a coplating strategy would produce colonies containing both GFP+ and GFP− cells if clonal mixing does occur (Supporting Information Fig. S4). Indeed, we observed numerous colonies containing various amounts of GFP− cells (Fig. 3A). We estimated the extent of mixing by coplating factor transduced GMPs at different densities (Fig. 3B). Mixing was not detectable when GMPs were plated at 130 or fewer per cm2 growth area. Of note, this is a vast underestimation of mixing behavior, since GFP+ versus GFP+ and GFP− versus GFP− mixing could not be detected by this method, which also would miss mixed colonies that contained few cells of a mixing component (i.e., a largely GFP+ colony with few GFP− cells is likely not to be scored as mixed).
To demonstrate that the mixed colonies are formed by cell migration, we performed time-lapse imaging with coplated GMPs (Fig. 3C; Supporting Information Movie S3). We tracked a mixed colony at the end of image acquisition back in time and found that the mixing components entered the imaging field from distinct locations at different times (colored arrows follow the traceable events). Migration occurred with the single cells and continued as the cells developed into small-cell clusters (Fig. 3C; Supporting Information Movie S3). Once within close proximity, the cells established cell-cell contacts and the entire cell aggregate continued migrating while also becoming more compact. As a result, a single colony containing both GFP+ and GFP− cells with normal ESC morphology formed. Since the founder cells are genetically distinguishable by the presence of GFP upon emergence of pluripotency, this observation demonstrates that mixed colonies could occur during pluripotency induction and the morphologic clonal appearance is not always equivalent to true cellular clonality.
In addition to clonal mixing, cellular migration also led to clonal dispersal. Developing small cell clusters are highly dynamic structures, with parts of the cell cluster transiently extending well beyond the focus plane (Fig. 3C; Supporting Information Movie S3). Others could break off, land in remote sites and continue to develop into normal looking colonies (Fig. 4A; Supporting Information Movie S4). This kind of migration would be less dependent on cell plating density, and more on random differences in the local cell microenvironment and/or sheer force.
Clonal dispersal, by which one founder cell gives rise to one or more colonies, could also result from single cell migration. One founder cell could produce one or more distinctive colonies similar in size, which we term “sister” colonies (Fig. 2B; Supporting Information Movie S2). Alternatively, single cells can break away from developing large cell clusters and establish separate colonies (Fig. 4B; Supporting Information Movie S5). Because the resultant new colonies are smaller in size than the main colony, we term them “satellite colonies.” This observation may explain the previously reported satellite colonies arising in fibroblast-based reprogramming cultures without obvious origin [7, 12].
As the migratory behavior is widespread, continuous and apparently random, colony mixing and dispersal coexist for many colonies, involving multiple founder cells (Fig. 3C; Supporting Information Movie S3) and/or multiple alternating rounds of mixing and dispersal (Supporting Information Movie S4), yielding colonies of complex clonal origins. Importantly, the migratory behaviors are not specific for hematopoietic cell-originated pluripotency, as we observed similar mixing and dispersal with other types of pluripotent cells (Supporting Information Movies S6–S8) including iPS cells derived from fibroblasts and ESCs themselves.
Taken together, these data demonstrate that dynamic cell migration accompanies the fate transition into pluripotency and affects the clonality of the colonies formed. Reprogramming efficiency may not be accurately described by the number of morphologically distinct colonies at the end of a reprogramming experiment. More stringent approaches involving the separation of founder cells may be required [7, 8]. Importantly, assessment of iPS cell clonality should be more vigorously performed.
Cell-Cell Interactions During Early Reprogramming Yield a Novel Morphologic Landmark
When back-tracking reprogramming from Oct-4-GFP+ colonies to founder cells, we identified a novel two-cell intermediate stage characterized by a unique “dumbbell” morphology, in which two cells appeared to be connected by an extended thin cellular process (Fig. 5A). Noticeably, the dumbbell intermediates occurred before the Oct4-GFP signal was detectable by time-lapse microscopy. Such two-cell dumbbells were formed as a result of cell division from a single parental cell. The two daughter cells did not fully segregate after division, but appeared “sticky” and become connected by a bridge-like structure, resulting in a dumbbell-shaped intermediate (Fig. 5A, could be seen in Supporting Information Movie S4). Figure 4B also shows a dumbbell at time point 62:00 (arrow, from Movie S5). Often without clear segregation, these two cells within a dumbbell continued with their next cell division(s) and became a partially connected multicell structure containing three to four cells (Fig. 5B, 5C). We traced 37 dumbbell structures across six independent reprogramming experiments and compared their duration and fate outcome (Fig. 5D, 5E). 33 (all type 1 and 2) of them reprogrammed successfully and 4 (all type 3) failed. There is a highly significant difference in the duration of the dumbbells: all dumbbells that lasted until the next cell division (10.5 ± 2.8 hours, type 1, n = 32) led to a colony or migrated to become part of another colony. In contrast, the dumbbells that failed to reprogram existed only briefly (1.5 ± 0.5 hours, type 3, n = 4), quickly broke apart and adopt a morphology similar to that of hematopoietic cells. We did observe one pair of cells (type 2, n = 1) that dissociated transiently but then came together again before proceeding with reprogramming (Fig. 5D, the dumbbell in brackets and Supporting Information Movie S2). In this case, the pair of cells remained in contact with each other for at least 4.5 hours, although the connecting process between the two cells was not as obvious due to the highly dynamic cell behavior. As such, all traceable colonies originated from a dumbbell structure and no colony was seen to have bypassed this stage. This unique structure could also be detected by conventional methods such as immunofluorescence and confocal microscopy (Fig. 5F, second row). Since the brief cell-pairing is minority (10.8%) and much shorter-lived (1.5 ± 0.5 hours as compared to 10.5 ± 2.8 hours) (Fig. 5D, 5E), the great majority of the dumbbell intermediates captured in these assays could be regarded as an early landmark of cells undergoing reprogramming.
Induction of E-cadherin is associated with the pluripotent state [22–24], but the exact timing and cellular stage when E-cadherin is induced remains unclear. With the hypothesis that E-cadherin might be responsible for the cell-cell interaction of the dumbbell stage, we explored the induction of E-cadherin at the two-cell dumbbell stage and subsequent cell clusters using immunofluorescence and confocal microscopy. GMPs and the non-reprogramming cells did not express E-cadherin at a level above the background fluorescence (Fig. 5F top row, yellow arrows of third row and Supporting Information S5A). E-cadherin protein became detectable at the two-cell dumbbell stage, but its distribution is mostly intracellular and peri-nuclear (Fig. 5F, second row). Not until the stage of compacting Oct-4-GFP+ cell cluster formation did E-cadherin start to distribute along the cellular periphery, a distribution pattern that was maintained afterward (Fig. 5F bottom two rows). Interestingly, Oct-4-GFP signal could be detected by immunofluorescence even at the two-cell dumbbell stage (Fig. 5F second row), possibly due to the higher detection sensitivity of low-level GFP by immunostaining as compared to direct fluorescence. These observations suggest that E-cadherin induction occurs very early and coincides with the dumbbell appearance during GMP initiated reprogramming. The distribution pattern of E-cadherin changes to the cell periphery as reprogramming progresses.
Inhibition of E-Cadherin Disrupts Cell-Cell Interactions of Early Reprogramming Intermediates and Prevents the Progression of Reprogramming
Since the two-cell dumbbell intermediate was seen in all lineages that successfully led to Oct-4 GFP+ colonies, and E-cadherin expression could be observed from this stage onward, we sought to determine the requirement for E-cadherin in forming this intermediate stage. Although E-cadherin is required during fibroblast-based reprogramming [22–25], a similar role in hematopoietic cell initiated reprogramming has not been reported . We first examined the function of E-cadherin during GMP-based reprogramming using an E-cadherin blocking antibody [22, 27]. Similar to MEF-based reprogramming, this antibody abolished the formation of Oct-4 GFP+ colonies with tight compact ESC morphology (Fig. 6A). Upon closer examination, some scattered weak GFP+ cells could be detected. In addition, we also used two validated shRNAs against E-cadherin  expressed from viral constructs that also contain tdTomato, such that the transduced cells are marked by red fluorescence. Normal compact colonies developed with the control tdTomato virus (GFP+ and tdTomato+) (Fig. 6B top panel). However, only disseminated colonies (weakly GFP+ and tdTomato+) were seen when shRNAs against E-cadherin were expressed (Fig. 6B middle and bottom panels). The existence of tdTomato negative, Oct-4 GFP+ colonies of normal morphology in all of the cultures suggests that the dysmorphic colony appearance is due to E-cadherin knockdown (Fig. 6B). The scattered weakly GFP positive cells could not be propagated under mESC conditions while the control cells could (data not shown).
To further confirm the role of E-cadherin, we performed reprogramming using GMPs from mice with a conditional E-cadherin allele . For this purpose, E-cadherinfl/fl mice were crossed with mice containing the Rosa26-rtTA  and tetO-Cre  alleles, such that E-cadherin could be inactivated specifically upon the addition of dox (Supporting Information Fig. S5B), which also initiates the reprogramming factor expression. While GMPs from tetO-Cre- mice gave rise to colonies of normal iPSC morphology that also stained positive for alkaline phosphatase activity, GMPs from the tetO-Cre+ littermates produced only loosely scattered cell clusters (Fig. 6C–6F). Inactivation of E-cadherin did not overtly inhibit the number of total cell clusters (Fig. 6D) if morphological abnormality is not considered, even though the lack of clearly defined morphologic boundaries for loose cell clusters may result in an underestimation of their numbers. However, when compactness of the cell clusters was assessed, the Cre+ cultures (hence the E-cadherin gene could be inactivated) were dominated by loose cell clusters (Fig. 6E) while all colonies in the Cre− cultures were compact. The few compact colonies present in the Cre+ cultures could be due to incomplete Cre-mediated gene inactivation , although it is also possible that some cell lineages could better sustain the loss of E-cadherin. The loose cell clusters in Cre+ cultures lacked E-cadherin protein expression as detected by immuno-fluorescence staining and confocal microscopy (Fig. 6F), which also showed little alkaline phosphatase activity (Fig. 6C). These data confirm that, as for MEFs, E-cadherin is required for GMP-initiated reprogramming. Inhibition of E-cadherin results in loosely scattered cell clusters that lack the phenotypes of pluripotent cells.
We then performed time-lapse imaging to examine whether the dumbbell intermediate was perturbed by E-cadherin knockdown, and if so, how reprogramming was affected. We recorded signals from DIC, GFP, and RFP channels at 15-minute intervals. In the presence of E-cadherin shRNAs, as indicated by tdTomato, the two-cell dumbbell intermediate was never observed (Fig. 6G; Supporting Information Movie S9). The cells continued to divide and some of the daughter cells even stayed in close proximity for an extended time. However, a cell-cell interaction mediated by a connecting process was never observed. While cell-cell interaction leading up to compaction is clearly visible beginning at 40.2 ± 4.7 hours post-dox addition in unperturbed reprogramming (from n = 25 reprogramming events across four independent experiments, see Fig. 2B for one example), the cells with E-cadherin shRNAs showed no sign of cell-cell interaction even at 81 hours post-dox addition (Fig. 6G). Oct-4 GFP expression was observed, but the intensity was much reduced (Fig. 6G, small light blue arrows). Of note, some of the cells appeared to have lost their red fluorescence, possibly due to silencing of the viral shRNA construct. These cells appear more normal in morphology and brighter for GFP (Fig. 6G, white block arrow). These observations revealed the perturbed early cell-cell interaction and subsequent formation of loose cell clusters.
Taken together, these experiments demonstrate that E-cadherin is required from the earliest stages of the reprogramming process. The earliest identifiable feature associated with productive reprogramming is the appearance of a unique dumbbell-shaped intermediate which subsequently grows in size as the cells become more compact. Disruption of E-cadherin prevents the formation of this intermediate and normal iPS colonies. Without E-cadherin, the pluripotency network may initiate, as suggested by the appearance of weakly GFP+ cells, but it cannot sustain and mature without proper E-cadherin function due to defective cell-cell interactions (Fig. 7).
We describe a novel experimental system with which we directly visualized the earliest phase of pluripotency induction by Yamanaka factors. In addition to high-temporal resolution up to every 5 minutes, the system overcomes multiple limitations of previously described methods enabling us to confidently trace reprogramming events back to the founder cells in their native somatic state. It is seen that dynamic migration and cell-cell interactions are integral to pluripotency emergence. These processes not only are crucial for reprogramming to proceed but also could compromise the interpretation of conventional reprogramming experiments. A simple founder-colony relationship is inaccurate due to this complex and dynamic process (Fig. 7).
We demonstrate that the dynamic cellular migration associated with pluripotency induction can lead to mixed colonies containing derivatives from multiple founder cells. Clonal mixing (Fig. 7E) challenges the assumption that all cells within the same morphologic boundary share the same genetic make-up. Clonality is a key assumption when interpreting data on pluripotency of iPSC colonies, their molecular similarity and their safety in potential clinical uses. Our data caution against the practice to pick and assume clonality of iPSC colonies only based on their final morphological boundary without rigorously ascertaining their clonality.
Clonal mixing has been suggested by Warlich et al.  using fibroblast as source cells, in which colony mixing was observed. However, it is important to point out that since Warlich et al. imaged MEF reprogramming from day 4.5 postviral transduction, it is not known whether the mixed colonies were coming from different founder cells or from different lineages downstream of the same founder cell. We affirmed the existence of mixed colonies with the enhanced resolution of our imaging system, which was further validated by coplating experiments using genetically distinct cells. The mixing behaviors of early reprogramming across different cell types, the existence of satellite colonies in fibroblast-initiated reprogramming , and the conserved requirement for E-cadherin argue against the dynamic behaviors being the peculiarity of GMP-initiated reprogramming. We demonstrate highly analogous migration behavior also for cells with fully established pluripotency including MEF-derived iPSCs and ESCs, suggesting that these dynamic behaviors are associated with the pluripotent state, rather than being unique to a particular source somatic cell state.
We uncovered a novel reprogramming intermediate with unique morphology. At least in this GMP-initiated reprogramming system, a dumbbell-shaped two-cell intermediate that lasts for about 10 hours appears to be a faithful marker for productive reprogramming. Furthermore, we demonstrate the involvement of E-cadherin in forming this intermediate. E-cadherin is an important mediator for the mesenchymal-to-epithelial transition following Yamanaka factor expression [23, 25, 26]. As E-cadherin is expressed by pluripotent cells and can replace Oct-4 in the original Yamanaka cocktail , it is conceivable that the signaling transduced by E-cadherin could feed into the core pluripotency network [9, 20] and provide a stabilizing effect. Alternatively, this mechanism may provide a crucial survival signal for cells in pluripotency but be dispensable otherwise. In support of this notion, it was reported that disruption of E-cadherin-mediated cell-cell adhesion activates the Rho/ROCK/MLC2 signaling cascade specifically in an epiblast-equivalent pluripotent cell state . Our data are consistent with a cell-autonomous role of E-cadherin in allowing the fate transition into pluripotency to progress further. When E-cadherin function is perturbed, proper cell-cell interactions reflecting cell fate transition into early pluripotency fail leading to impaired reprogramming. Our work provides the first direct visualization of this disrupted process and confirms the role of E-cadherin in the very early stages of pluripotency induction. We describe an imaging system that can be used to address multiple key questions regarding early reprogramming. When coupled with specific molecular perturbations, molecular machineries that underlie early reprogramming can be probed. Additional markers of cellular states can be incorporated to generate richer real-time information. We anticipate that new cellular features that inform stochastic and deterministic behaviors [6, 31] may be uncovered.
We describe an imaging system that can be used to address multiple key questions regarding early reprogramming. This system allows study of reprogramming at a stage much earlier than that accessible by conventional methods. When coupled with specific molecular perturbations, molecular machineries that underlie early reprogramming can be probed. Additional markers of cellular states can be incorporated to generate richer real-time information. We anticipate that new cellular features that inform stochastic and deterministic behaviors 6, 31 may be uncovered.
We thank Dr. Haifan Lin for insightful discussion. This study was supported by NIH grants DK082982 (to S.G.), DK086267, (to D.K.) Yale Center of Excellence in Molecular Hematology and Connecticut Innovations (to J.L. and S.G.).
DISCLOSURE OF POTENTIAL CONFLICTS OF INTEREST
The authors indicate no potential conflicts of interest.