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First published online August 25, 2008
doi: 10.1242/10.1242/dev.021519
1 Developmental Biology Program, Sloan-Kettering Institute, New York, USA.
2 Faculty of Life Sciences, Manchester University, Manchester, UK.
3 Department of Experimental Embryology, Institute of Genetics and Animal
Breeding, Polish Academy of Sciences, Jastrze
biec, Poland.
Authors for correspondence (e-mails:
Berenika.Plusa{at}manchester.ac.uk;hadj{at}mskcc.org)
Accepted 24 July 2008
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SUMMARY |
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 TOP SUMMARY INTRODUCTIONMATERIALS AND METHODSRESULTSDISCUSSIONREFERENCES |
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) as an
early-expressed protein that is also a marker of the later PrE lineage. By
combining live imaging of embryos expressing a histone H2B-GFP fusion protein
reporter under the control of Pdgfra regulatory elements with the
analysis of lineage-specific markers, we investigated the events leading to
PrE and EPI lineage segregation in the mouse, and correlated our findings
using an embryo staging system based on total cell number. Before blastocyst
formation, lineage-specific factors are expressed in an overlapping manner.
Subsequently, a gradual progression towards a mutually exclusive expression of
PrE- and EPI-specific markers occurs. Finally, cell sorting is achieved by a
variety of cell behaviours and by selective apoptosis.
Key words: Lineage specification, Mouse blastocyst, ICM, Primitive endoderm, Epiblast, Pdgfr, Histone H2B-GFP fusion, Live imaging
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INTRODUCTION |
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TOPSUMMARYINTRODUCTIONMATERIALS AND METHODSRESULTSDISCUSSIONREFERENCES |
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The initial differentiation of the TE depends on asymmetric positional
signals that induce cell polarisation, followed by epithelialisation (reviewed
by Yamanaka et al., 2006
).
Only the maintenance of TE, rather than its initial differentiation, is
dependent on known TE-specific transcription factors, such as Cdx2 and Eomes
(Niwa et al., 2005;
Ralston and Rossant, 2008).
Similarly, specification of PrE was previously believed to occur in response
to positional signals at the interface between the ICM and the blastocyst
cavity, reflecting the ultimate position of the tissue (reviewed by
Yamanaka et al., 2006). This
view was supported by the observation that when embryonic stem (ES) cells are
allowed to form embryoid bodies, the outer layer of cells differentiates to
form PrE-derived tissue (Becker et al.,
1992; Martin and Evans,
1975; Murray and Edgar,
2001).
Recently, an alternative model has been proposed from the observation that
two early markers of EPI (Nanog) and PrE (Gata6) lineages exhibit an
apparently random and mutually exclusive (`salt- and-pepper') distribution
within the ICM at the mid-blastocyst stage, prior to PrE formation
(Chazaud et al., 2006;
Rossant et al., 2003).
Moreover, individually labelled mid-blastocyst ICM cells exhibited a
propensity to contribute to either the EPI or PrE, but not both. These data
suggest that EPI and PrE cells are fated at a relatively early stage, and only
later sort into their respective layers
(Chazaud et al., 2006). We
reasoned that live imaging of PrE formation would provide validation of the
model, and that a fluorescent reporter of PrE precursors would provide the
necessary tool.
A microarray analysis of gene expression in single cells isolated from the
mouse blastocyst revealed that expression profiles largely fall within two
cohorts: one characterised by PrE-specific genes, the other by EPI-specific
genes (Kurimoto et al., 2006).
The gene encoding platelet-derived growth factor receptor alpha (Pdgfr)
stood out within the PrE-specific cohort, as it was also identified in
expression profiles of extraembryonic endoderm (XEN) cells
(Kunath et al., 2005). A
functional role for Pdgfr in PrE specification was also plausible
because of evidence suggesting a role for receptor tyrosine kinase signalling
in this process (Chazaud et al.,
2006). Activation of the PI3K pathway by PDGFRs promotes actin
reorganisation, directs cell movements and inhibits apoptosis. PDGFRs have
also been implicated in the integrin-induced enhancement of cell migration and
cell survival (reviewed by Andrae et al.,
2008; Hoch and Soriano,
2003).
We used the PdgfraH2B-GFP mouse strain
(Hamilton et al., 2003), in
which a cassette containing human histone H2B fused to enhanced green
fluorescent protein (H2B-GFP) was targeted to the Pdgfra locus, to
image PrE formation. The localisation of H2B-GFP to active chromatin
facilitated the identification and tracking of individual reporter-expressing
cells in vivo (Hadjantonakis and
Papaioannou, 2004; Kanda et
al., 1998).
Our live imaging experiments combined with an immunohistochemical analysis of lineage-specific factors revealed a series of sequential and distinct phases in the process of PrE formation. Our data lead us to propose a model in which the early overlapping expression of transcription factors precedes the maturation of inhibitory regulatory pathways and lineage-restricted expression after around the 64-cell stage. Cell sorting then occurs via a combination of behaviours, including cell movement, adhesion and selective apoptosis.
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MATERIALS AND METHODS |
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TOPSUMMARYINTRODUCTIONMATERIALS AND METHODSRESULTSDISCUSSIONREFERENCES |
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)
females mated with ICR or PdgfraH2B-GFP/+ males.
PdgfraH2B-GFP/H2B-GFP embryos were indistinguishable from
PdgfraH2B-GFP/+ embryos at all stages examined.
Preimplantation embryos were flushed from uteri or oviducts in M2 (Chemicon)
and cultured in KSOM (Chemicon) under mineral oil (Sigma) at 37°C and 5%
CO2 in air. Postimplantation embryos were dissected in PB-1
(Papaioannou and West, 1981).
For live imaging, embryos were cultured in agarose-coated glass-bottom dishes
(MatTek) in an environmental chamber (Solent Scientific).
Detection of Pdgfr protein and transcripts in early embryos
Oocytes/embryos were collected from natural matings of ICR animals. Pooled
embryos were lysed by three rounds of heat shock. Reverse transcription was
performed using Superscript III First-strand Kit (Invitrogen). RT-PCR and
nested RT-PCR were performed using an equivalent of 0.5 to 1
oocytes/embryos.
For Hprt detection, conditions of RT-PCR were 95°C for 3
minutes, then 35 cycles of 94°C for 30 seconds, 58°C for 1 minutes and
72°C for 1 minutes; this was followed by 10 minutes at 72°C. For
Pdgfr detection, a first round of PCR was performed using the
conditions stated above but with 25 amplification cycles. A second round of
PCR was performed under similar conditions with 20 amplification cycles, using
5 µl of the first PCR reaction. Hprt primers:
5'-GTTCTTTGCTGACCTGCTGGATTAC-3',
5'-GTCAAGGGCATATCCAACAACAAAC-3'. Pdgfra primers (first
round of amplification): 5'-AATCCTGCAGACGAGAGCAC-3',
5'-GCCACCAAGGGAAAAGATTT-3'. Pdgfra primers (second round
of amplification): 5'-CACACAGTATGTCCCCATGCT-3',
5'-GCCATAGGACCAGACGTCACT-3'.
Immunostaining
The zona pellucida was removed using acid Tyrode's solution (Sigma).
Embryos were fixed in 4% paraformaldehyde (PFA) in PBS with 0.1% Tween 20
(Sigma) and 0.01% Triton X-100 (Sigma) overnight (2% PFA for 2 hours for
Pdgfr immunostaining) at 4°C, permeabilised in 0.55% Triton X-100
in PBS for 15 minutes and blocked in 10% fetal bovine serum in PBS for 1 hour.
Primary antibodies used were: anti-cleaved caspase-3 (Cell Signalling),
anti-Cdx2 (BioGenex), anti-DAB2 (BD Transduction Laboratories), anti-Gata4
(Santa Cruz), anti-Gata6 (R&D Systems), anti-GFP (Invitrogen) and
anti-Pdgfr (Santa Cruz, eBioscience) at 1/100, and anti-Nanog
(Chemicon) at 1/150. Secondary Alexa Fluor (Invitrogen)-conjugated antibodies
were used at a dilution of 1/500. DNA was visualized using Hoechst 33342 (5
µg/ml, Molecular Probes).
TUNEL analysis
Freshly recovered embryos were fixed in 4% paraformaldehyde for 15 minutes
at room temperature, washed three times in PBSA and permeabilised for 2
minutes in 0.1% Triton X-100 and 0.1% sodium citrate in PBSA. Embryos were
then washed three times in PBSA and incubated in TUNEL reaction mixture
(Roche) for 1 hour at 37°C.
Cell number staging system for preimplantation embryos
By convention, mouse developmental stages are defined by the calculated
time from which copulation is presumed to occur. However, embryos collected at
the same time vary substantially in terms of cell number and developmental
stage. Thus, we based our staging system on total cell number and collected
embryos at approximately 3-hour intervals between E2.75 and E4.75. Fixed
specimens were stained with a nuclear dye (Hoechst 33342). For in vivo
observations, we used the nuclear- and plasma membrane-labelling vital dye
FM4-64 (Invitrogen) at a dilution of 1/10 in M2 medium for 30 minutes at
37°C. Only non-dividing cells with clearly visible nuclei were included
when scoring for nuclear-localised transcription factors by
immunostaining.
Embryo transfer
Laser live-imaged embryos were transferred to pseudopregnant females and
allowed to develop to term (Nagy,
2003). Four to six CAG::mRFP1Tg/+
(Long et al., 2005) `carrier'
age-matched embryos were co-transferred.
Image acquisition
Laser scanning confocal images were acquired on a Zeiss LSM 510 META.
Immunostained embryos were mounted in Vectashield (Vector Laboratories).
Fluorescence was excited with a 405-nm laser diode (Hoechst), a 488-nm Argon
laser (GFP), a 543-nm HeNe laser (Alexa Fluor 543, 555, FM4-64 and mRFP1) and
a 633-nm HeNe laser (Alexa Fluor 633 and 647). Images were acquired using a
Plan-apochromat 20x/NA 0.75 objective. Optical section thickness ranged
from 1 µm to 4 µm. For 3D time-lapse imaging, 10-20 xy planes
were acquired, separated by 3-4 µm. Time intervals between
z-stacks were 7-15 minutes, for a total of 6-17 hours.
Image processing and analysis
Raw data were processed using Zeiss AIM software (Carl Zeiss Microsystems).
Movies of time-lapse sequences were compiled and annotated using QuickTime
(Apple Computer) and ImageJ (NIH). For fluorescence quantification
measurements, images were analysed using IMARIS 6.0.1 software (Bitplane AG).
Nuclei were identified using the `spot' option with an estimated diameter of
7-10 µm in the Hoechst channel. The number of nuclei identified by the
software was confirmed manually. Protein levels were analysed as mean
fluorescence intensities inside `spot' regions of interest (ROI), and were
normalised by dividing by mean fluorescence intensity in the Hoechst
channel.
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RESULTS |
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TOPSUMMARYINTRODUCTIONMATERIALS AND METHODSRESULTSDISCUSSIONREFERENCES |
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protein is localised within ICM
cells adjacent to the blastocyst cavity, consistent with the PrE. At E4.0,
Pdgfr was co-expressed with Gata4, a zinc-finger-containing
transcriptional regulator and known PrE marker
(Fig. 1A, see also Movie 1 in
the supplementary material).
We next investigated whether a pre-existing PdgfrH2B-GFP
line (Hamilton et al., 2003)
could serve as a reporter of PrE. In E4.0 PdgfraH2B-GFP
embryos, GFP was colocalised in all cells with detectable endogenous
Pdgfr, which localised to the plasma membrane
(Fig. 1B). We were able to
detect GFP fluorescence earlier than Pdgfr protein. In embryos with
16-32 cells (n=9), in which endogenous Pdgfr was undetectable,
some cells were weakly GFP-positive (see Fig. S1A in the supplementary
material), whereas in 33- to 64-cell embryos (n=6; see Fig. S1B in
the supplementary material), a subset of GFP-positive cells was negative for
Pdgfr (endogenous protein was always localised to GFP-positive cells).
This was not unexpected, because a lower level of total fluorescence is
required for detection in a volumetrically constrained structure, such a
nucleus, than in a volumetrically dispersed structure, such as the plasma
membrane. By the 64-cell stage, all GFP-positive cells were positive for
Pdgfr protein (n=10; see Fig. S1C in the supplementary
material). These observations were supported by RT-PCR (see Fig. S1D in the
supplementary material).
We next demonstrated the colocalisation of GFP with markers of the PrE,
including Gata4, Gata6 and the cell adhesion protein Dab2
(Fig. 1C-F). GFP fluorescence
was restricted to cells of the parietal (arrowheads) and visceral endoderm,
the two derivatives of the PrE (Fig.
2F,G). The co-expression of the PdgfrH2B-GFP
reporter and endogenous Pdgfr protein with established PrE markers
confirmed that Pdgfr could be used as a marker of PrE formation.
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H2B-GFP reporter expression correlate with specific developmental stages
70-84 hours post coitum (hpc), 16-34 cells], but none in
8-cell embryos (n=7). In the majority of GFP-positive morulae, we
detected GFP expression in some outer cells destined to form the TE, as well
as in some inner cells destined to form the ICM (15/20;
Fig. 2A). By the early
blastocyst stage (78-93 hpc, 29-63 cells), GFP could be detected in both
the ICM and the TE (Fig. 2B,
arrowhead) in some embryos (12/30), whereas, in the remainder (18/30),
expression was restricted to the ICM (see Movie 2 in the supplementary
material). By the mid-blastocyst stage (87-96 hpc, 64 to 79 cells),
GFP was almost always restricted to the ICM and was distributed in an
apparently random, heterogeneous manner, resembling the distribution of other
known PrE markers (Chazaud et al.,
2006; Gerbe et al.,
2008). Although the level of fluorescence varied among cells, the
majority of ICM cells (68.2% of 151 cells scored) were GFP positive
(Fig. 2C,D; n=7
embryos). Interestingly, as total cell number increased, the strongest GFP
expression became progressively more restricted to cells lining the cavity,
whereas cells exhibiting reduced levels of GFP fluorescence were located
deeper within the ICM (Fig.
2D). In the majority of late blastocysts (96-114 hpc, >80
cells), GFP-positive cells were found exclusively in the nascent PrE layer
(8/12; Fig. 2E,F).
Our observation of PdgfrH2B-GFP reporter expression
between the early morula and the late blastocyst revealed distinct phases
during PrE formation that correlated with developmental stage as defined by
total cell number.
Expression of lineage-specific transcription factors is not mutually exclusive in the morula (16-33 cells) and early blastocyst (<32 cells)
To elucidate the significance of early PdgfrH2B-GFP
expression, we examined the distribution of the EPI-specific homeobox
transcription factor Nanog and the PrE-specific factors Gata4 and Gata6 during
this period (reviewed by Yamanaka et al.,
2006). Expression of Gata6 has previously been reported in
blastocysts (Chazaud et al.,
2006; Koutsourakis et al.,
1999), and in `late morulae/early blastocysts'
(Rossant et al., 2003),
whereas the expression of Nanog has been reported as early as the 8-cell stage
(Dietrich and Hiiragi 2007). We
used total cell number for staging embryos, as we noted that embryos collected
at the calculated same time after mating varied in cell number (see Fig. S2A
in the supplementary material), even within the same litter (see Fig. S2B in
the supplementary material). Interestingly, although total cell number
appeared to increase approximately linearly with time (see Fig. S2C in the
supplementary material), embryos with 30-36 cells and 58-72 cells were
disproportionately over-represented (see Fig. S2D in the supplementary
material), suggesting that some degree of synchrony in the cell cycle may
exist until at least the 64-cell stage. This also appeared to be supported by
a relative `levelling out' in the rate of increase in cell number at these
stages (see Fig. S2C in the supplementary material).
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), we detected Nanog in most 8-cell stage embryos
(10/11). GFP expression was detected from the 16-cell stage in a subset of
cells (Fig. 2A) in
PdgfraH2B-GFP embryos, and from its onset overlapped with
expression of Gata6 (Fig. 3A).
At the morula stage, Nanog (n=33), and Gata6 (n=12) were
detectable in almost all non-dividing inner and outer cells (88.8% of 770
cells were Nanog positive and 92.2% of 380 cells were Gata6 positive), in
agreement with previous observations
(Strumpf et al., 2005).
Strikingly, the localisation of these two factors was not mutually exclusive
and overlapped at these early stages (see Table S1 in the supplementary
material). Moreover, we observed strong Gata6- and/or Nanog-positive staining
in both inside and outside cells (Fig.
3C). This observation mirrors a recent report for the expression
of Nanog relative to that of the TE-associated transcription factor Cdx2
(Dietrich and Hiiragi,
2007).
A comparable expression pattern was observed in very early blastocysts of
up to 33 cells (n=43 for Nanog, n=7 for Gata6), with both
factors detected in both ICM and TE cells (83.3% of 1314 cells analysed were
Nanog positive and 91% of 221 cells were Gata6 positive;
Fig. 3D). Similar to at earlier
stages, Nanog and Gata6 expression were not mutually exclusive at this stage
(n=19; Fig. 3C,D; see
also Table S1 in the supplementary material). This is in contrast to previous
reports describing the localisation of these factors in later blastocysts
(Chazaud et al., 2006;
Gerbe et al., 2008).
To investigate further the relationship between Nanog and Gata6 expression, we measured signal intensity within each cell nucleus for these factors and calculated correlation coefficients (see Table S2 in the supplementary material). Embryos of less than 30 cells generally showed no correlation between Nanog and Gata6 expression. With increasing total cell number, an increased frequency of positive correlations was noted when calculated across all cells. When calculated across only the 25% of cells exhibiting the highest Nanog and Gata6 expression (defined as the product of normalised Nanog and Gata6 signal intensities), we recorded strong negative correlations, with the frequency increasing with total cell number (see Table S2 in the supplementary material). Thus, positive correlations in low-expressing cells may reflect a variation amongst cells in general levels of transcription, whereas negative correlations observed in high-expressing cells may suggest that the effect of mutually inhibitory pathways becomes significant with the increased expression of these factors.
At around the 32-cell stage, the pattern of PdgfrH2B-GFP
expression showed no consistent relation to Nanog distribution (n=7;
see Table S3 in the supplementary material). We were unable to detect
expression of the PrE-specific factor Gata4 during these stages
(Fig. 4A).
We also noted that strongly Nanog-positive cells in the TE did not exhibit
reduced levels of Cdx2 (see Fig. S3 in the supplementary material), in
agreement with a recent report (Dietrich
and Hiiragi, 2007) revealing no reciprocal relationship between
Nanog and Cdx2 at these stages. Thus, in embryos with up to 32 cells, PrE and
EPI markers are not restricted to the ICM, nor, together with Cdx2, are they
mutually exclusive.
Changes in lineage-specific gene expression during the 32- to 64-cell transition
We observed a decreasing proportion of Nanog-positive and Gata6-positive
cells (63.3% of 2303 cells scored in n=54 embryos and 62.7% of 346
cells in n=8 embryos, respectively) in blastocysts that had entered
the next round of cell divisions (between 33 and 63 cells). This was more
pronounced in TE cells. During this transition, the expression patterns of
Gata6 and Nanog became increasingly mutually exclusive (n=8;
Fig. 3E; see also Table S1 in
the supplementary material). Ubiquitous or near-ubiquitous Nanog expression
was not observed in blastocysts of more than 36 cells
(Fig. 3E,
Fig. 4B). We speculate that
this period reflects a transition to a transcription factor-dependent phase of
TE maintenance, following an earlier phase of Cdx2-independent TE
differentiation (Niwa et al.,
2005; Ralston and Rossant,
2008).
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PrE formation is preceded by the downregulation of Nanog and upregulation of Gata4 in presumptive PrE precursors at around the 64-cell stage
At around the 64-cell stage, the localisation of lineage-specific markers
underwent a dramatic transition. The number of embryos with Gata4-positive
cells increased significantly between the stages of 64 to 80 cells (81.5%,
n=27). Consistent with previous observations of other PrE markers
(Chazaud et al., 2006;
Gerbe et al., 2008),
Gata4-positive cells were distributed in an apparently random heterogeneous
pattern within the ICM (Fig.
4B, Fig. 5A,B).
Similar to during the 32- to 64-cell transition, we observed very little
overlap between Gata4 and Nanog staining. In 40 embryos of 58-79 cells, only
7.8% (n=204) of Gata4-positive cells were also Nanog positive. This
is in agreement with a single-cell microarray analysis
(Kurimoto et al., 2006), in
which Gata4 was more consistently expressed than Gata6 in cells exhibiting a
PrE-like expression profile. Together, these results indicate that Gata4 is a
more specific marker of PrE fate than Gata6, and for this reason it was
favoured in our further analyses of PrE formation.
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It is interesting to note that the decrease in both the proportion and the absolute number of Nanog-positive cells correlated with the appearance of Gata4-positive cells, whose number increased approximately linearly thereafter (correlation coefficient: +0.78). Meanwhile, the number of Nanog-positive cells remained constant with increasing total cell number (correlation coefficient: +0.025; Fig. 4E). Considering their mutual exclusiveness during this period, it is likely that the divergence in relative numbers of Nanog- and Gata4-expressing cells was largely due to differences in proliferation rates.
Establishment of the nascent primitive endoderm layer occurs in embryos of more than 80 cells
Approximately one half of embryos with 80-100 cells exhibited partial or
complete segregation of Gata4-positive cells to the PrE layer and
Nanog-positive cells to the EPI layer (53.1%; n=32;
Fig. 5I), whereas the remainder
still exhibited a salt-and-pepper distribution. In the latter, Gata4 and GFP
expression were almost invariably exclusive from Nanog expression. In embryos
with partial segregation of the EPI and the PrE, which we defined as an
essentially formed PrE with one or two Gata4-positive cells persisting in
deeper layers of the ICM (Fig.
5C), those cells usually exhibited lower levels of fluorescence
than did GFP-positive/Gata4-positive cells in the PrE layer (see Fig. S4 in
the supplementary material).
In 80.2% (n=96) of embryos of >100 cells, Gata4-positive cells
were restricted to the PrE layer (Fig.
4D, Fig. 5I). PrE
formation was invariably complete in embryos with more than 155 cells
(n=8). At no stage was Gata4 observed in TE cells. We found that the
number of GFP-positive cells increased approximately linearly
(Fig. 4F). Significantly, in
PdgfrH2B-GFP embryos of >64-cells, Gata4 was expressed
only in GFP-expressing cells (n=80), although in 64- to 100-cell
embryos GFP-positive/Gata4-negative cells were frequently encountered. These
data indicate that Gata4-expressing PrE precursors are recruited from the
population of Pdgfr-expressing cells at around the 64-cell stage.
Subsequently, they become segregated to the layer of cells lining the cavity.
This process starts at around the 80-cell stage and is almost complete in
embryos of >100cells.
Live-imaged PdgfraH2B-GFP embryos progress through stages comparable with in vivo development
To document the dynamics of sorting of PrE and EPI precursors, we performed
a 3D time-lapse analysis. Live-imaged PdgfraH2B-GFP
embryos progressed through stages comparable with development in utero
(Fig. 5E-H). The earliest cells
expressing GFP were distributed in a random heterogeneous manner in morulae
and early blastocysts (see Movie 5 in the supplementary material). By the
mid-blastocyst stage, the majority of ICM cells expressed GFP at variable
levels. Subsequently, GFP-positive cells comprised the layer of cells lining
the cavity, which we interpreted as the nascent PrE
(Fig. 5; see also Movie 6 in
the supplementary material). As an additional criterion, we were also able to
identify the PrE morphologically under bright-field illumination (arrowheads,
Fig. 5H').
Although the transition from an apparently random distribution of GFP-positive cells to a nascent PrE layer is usually a gradual process taking several hours, our data revealed that this transition can occur very rapidly - within only 15 minutes - in some embryos (see Movie 7 in the supplementary material). After the PrE was formed, in some cases we were still able to distinguish cells with weak GFP signal deeper within the ICM. However, from movies of embryos that had been cultured beyond the 128-cell stage, it could be seen that these cells either downregulated GFP until it was no longer detectable or underwent cell death, evident by nuclear fragmentation. Concomitantly, the GFP signal intensity in cells lining the cavity increased (see Fig. S4 and Movie 8 in the supplementary material).
PrE- and EPI-specific markers showed normal (similar to in utero) segregation in embryos fixed after 17 hours of live imaging (n=24; see Fig. S5 in the supplementary material). Embryos transferred to recipient females after >14 hours of imaging developed to term, were viable and exhibited normal fertility in adult life. Thus, live imaging did not compromise either the viability of embryos or the process of lineage segregation. The latter was similar to that observed in stage-matched freshly flushed embryos.
Directionally biased relocation and apoptosis of GFP-positive cells contribute to cell sorting during PrE formation
It was recently suggested that cell sorting of PrE and EPI precursors leads
to the segregation of these two lineages
(Rossant et al., 2003;
Chazaud et al., 2006). To
explore this process, we analysed the behaviour of 90 GFP-positive cells in
six embryos developing through the 32- to 64-cell transition (early-stage
movies; see Movie 5 in the supplementary material) and 150 GFP-positive cells
in six embryos developing through the 64- to 128-cell transition (late-stage
movies; see Movies 6 and 7 in the supplementary material). We scored the
original position of each GFP-positive ICM cell within the embryo as being
either `cavity' (in contact with the cavity) - or `inner' (lying within the
deeper layers of the ICM). We then scored the final position (at the end of
the movie; see Table S4 in the supplementary material) of the original cell,
or of its daughter cells if the cell had divided.
We observed that almost half of GFP-positive cells in the early-stage movies (42/90) and a third in the late-stage movies (52/150) acquired a position within a layer different from that of its original position (or that of its parental cell in cases where division had occurred). Some of the cells analysed exhibited downregulation of GFP to undetectable levels or underwent apoptosis (see Table S4 in the supplementary material). These cells were not included in the calculation of the final position of cells within an embryo, as this could not be reliably determined.
In the early stage movies, the vast majority (72.5%, n=40) of GFP-positive cells originating in the cavity layers maintained their position there, whereas only 34% of GFP-positive cells (n=47) originating in the inner layers maintained their position. This indicated that although relocation of GFP-positive cells could occur in any direction, it was strongly biased towards the cavity. During the 64- to 128-cell stage transition, this tendency became even more pronounced, as 100% of GFP-positive cells (n=64) originating in the cavity layer maintained their position, whereas only 15.8% of GFP-positive cells originating in the inner layers maintained theirs (n=57). GFP-positive cells that remained in the inner layers once the PrE layer had formed were observed to be undergoing apoptosis or downregulating GFP (see Movie 8 and Fig. S4 in the supplementary material).
It has previously been reported that a small proportion of cells in mid- to
late blastocysts undergo apoptosis (Copp,
1978). As H2B-GFP localises to chromatin, it served as a live
imaging reporter of the nuclear fragmentation associated with cell death.
Indeed, we observed apoptosis during the 64- to 128-cell transition (see Table
S4 in the supplementary material), but not during the 32- to 64-cell stage
transition (n=90). We detected a steadily increasing rate of
apoptosis in embryos of more than 64 cells. The number of GFP-positive cells
lining the cavity, observed in late-stage movies, that underwent apoptosis
(8.1%, n=123 cells) was similar to that reported previously for ICM
cells (Copp, 1978).
Surprisingly, in the subset of GFP-positive cells that remained deeper within
the ICM and isolated from other GFP-positive cells, the rate of apoptosis was
considerably higher (48.2%, n=27). GFP-positive cells that maintained
an inside position during the 64- to 128-cell transition yet did not apoptose
were more likely to downregulate reporter expression (9/15 cells). These
observations were confirmed by TUNEL analysis and activated-caspase staining
(see Fig. S6 in the supplementary material).
These results are consistent with the recent model of PrE formation
(Rossant et al., 2003;
Chazaud et al., 2006), whereby
cells expressing PrE markers relocate unidirectionally towards the cavity,
whereas those already lining the cavity are likely to maintain their position.
In addition, our data point to apoptosis as being an additional mechanism that
ensures appropriate segregation of the PrE and EPI layers. GFP-positive cells
that do not contribute to PrE or downregulate Pdgfr are eliminated from
the EPI layer by apoptosis.
Multiple cell behaviours contribute to cell sorting during PrE formation
We distinguished several modes by which GFP-positive cells could contribute
to the cavity layer (Fig. 6;
see also Movie 9 in the supplementary material). `Intercalation due to cavity
expansion' occurred when a cell intercalated into the layer of cells lining
the cavity due to expansion of the cavity and the accompanying `stretching' of
cell layers. `Intercalation by cell division' occurred when a cell either
acquired a position different from that of its parent cell because of the
orientation of division of that parent cell, or acquired a new position
because of cell rearrangements resulting from the division of a neighbouring
cell. In another category, termed `cell allocation due to other reasons', a
cell changed its original position for reasons that could not be distinguished
as being either a `passive' mechanism (such as intercalation by cell division
or cavity expansion) or active migration. The frequencies of each mode of cell
behaviour during early- and late-stage movies are shown in
Fig. 6B.
During the 32- to 64-cell transition, the majority of GFP-positive cells that were positioned in the cavity layer by the end of the time-lapse sequence originated in the cavity layer and/or were passively incorporated into it as a result of cavity expansion (75.4%, n=61, Fig. 6), similar to during the 64- to 128-cell transition (67.3%, n=113, Fig. 6). Only a minority of GFP-positive cells acquired their final position in the cavity layer by cell allocation due to other reasons in both early-stage (18%) and late-stage (31.2%) movies (Fig. 6B). In summary, several types of cell behaviour contributed to the positioning of GFP-positive cells within the cavity layer by the end of the time-lapse period. However, the predominant contributors appeared to be passive mechanisms, dependent on either the original position of the cell in the cavity layer or passive intercalation due to cavity expansion.
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DISCUSSION |
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TOPSUMMARYINTRODUCTIONMATERIALS AND METHODSRESULTSDISCUSSIONREFERENCES |
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Pdgfr is a novel marker for PrE. A mouse line expressing histone
H2B-EGFP reporter from the Pdgfra locus served as a live imaging
reporter of PrE. PdgfrH2B-GFP expression is initially
distributed in an apparently random, heterogeneous manner until approximately
the 64-cell stage, or after six rounds of divisions. The early heterogeneous
expression of PdgfrH2B-GFP is reminiscent of the recently
reported salt-and-pepper expression of Nanog and Gata6 in the ICM of the E3.5
blastocyst (Chazaud et al.,
2006; Rossant et al.,
2003). This, along with the lineage tracing studies, has led to a
model for lineage specification in which EPI and PrE precursors are specified
in a possibly random manner within the ICM and later segregate to their
respective layers. This is in contrast to the previously assumed model that
cell position with respect to the blastocyst cavity is the primary determinant
of PrE fate (reviewed in Yamanaka et al.,
2006).
Our results revealed a multi-step process of PrE formation that shares
features of both of these models. As also shown by Dietrich and Hiiragi
(Dietrich and Hiiragi, 2007),
lineage-specific factors initially exhibit widespread and overlapping
expression in early blastocysts. This is followed by progression towards the
mutually exclusive expression of Cdx2 in the TE
(Dietrich and Hiiragi, 2007)
(this study) and Nanog, Gata6 and Pdgfr in the ICM (this study, see
Fig. 7) and, subsequently, by
the mutually exclusive expression of EPI- and PrE-specific markers in the ICM
during the 32- to 64-cell transition.
We also noticed that at early stages (morula and early blastocyst), the
levels of Gata6 and Nanog vary among cells throughout the embryo and generally
appear to be mutually independent. A similar observation was described by
Dietrich and Hiiragi for TE and ICM markers
(Dietrich and Hiiragi, 2007).
There are two possible explanations for this type of expression. First, the
relative levels of different factors, while varying among cells, may remain
fairly constant within individual cells. Differences would then become
amplified by the maturation of mutually inhibitory pathways at later stages.
Alternatively, it is possible that the relative levels of factors fluctuate
with time. Interestingly, it was reported recently that Nanog
expression fluctuates in ES cells (Chambers
et al., 2007). Low levels of Nanog predisposed cells towards
differentiation, but did not mark commitment. In another study, cells were
flow-sorted according to their level of Nanog expression and, when
subsequently cultured, they reverted to their original heterogeneous state. An
association between stochastic gene expression and differentiation has been
reported in other systems (Hu et al.,
1997), but evidence during embryo development, especially in the
mouse, has previously been lacking (reviewed by
Laforge et al., 2005;
Martinez-Arias and Hayward,
2006).
It seems plausible that such a mechanism may operate within the ICM. We
propose that before blastocyst formation, a large number of genes exhibit
fluctuating and mutually independent expression at low levels. As
transcription factor levels increase, mutually inhibitory regulatory pathways
begin to take effect. The latter is supported by our observation that mutually
exclusive expression is typically observed only in the subset of cells with
the highest expression levels. Heterogeneous expression of Nanog that
correlated negatively with Gata6 expression has recently been reported in
mouse ES cells (Singh et al.,
2007). Nanog was shown to repress Gata6 directly, through binding
of its promoter. Conversely, the Grb/Mek pathway, which regulates Gata6
expression, has been shown to repress Nanog expression
(Hamazaki et al., 2006).
Our data suggest that downregulation of Nanog and Gata6 occurs in two phases. The first reflects downregulation in TE cells, which was often evident immediately after blastocyst formation but had invariably commenced in all blastocysts of at least 37 cells. The second phase initiates around the 64-cell stage, when the number of Nanog-positive cells drops dramatically and thereafter remains relatively constant. This phase reflects the maturation of the presumed inhibitory mechanisms between Nanog- and Gata4/Gata6-expressing pathways, analogous to the state of ES cells.
|
) suggests that 30% of ICM cells from early blastocysts have a
dual fate, with daughter cells occupying both EPI and PrE layers. This is in
contrast to the restricted fate of ICM cells found in what were likely to be
later stage blastocysts (Chazaud et al.,
2006). This would suggest that fate becomes restricted around the
mid-blastocyst (64-cell) stage, and is coincident with changes in marker
expression.
Our data support the restriction of ICM cell fate preceding cell sorting.
Despite this, our live imaging data revealed an upregulation of
PdgfrH2B-GFP expression in cells lining the blastocyst
cavity and downregulation in deeper-lying cells, supporting a role for
positional signals. The variety of behaviours of GFP-positive cells we
observed in our live imaging studies suggests a more complex model of cell
sorting than a simple segregation of precursors to the respective EPI and PrE
layers. The failure of some GFP-positive cells to contribute to the PrE
suggests that, although the mutually exclusive expression of Nanog and Gata6
biases cells towards a particular fate, positional signals are required to
complete or reinforce specification. Cell polarisation is likely to be
involved, consistent with the observation that, prior to PrE formation, the
sub-cellular localisation of the PrE markers Lrp2 (megalin) and Dab2 becomes
polarised only in cells lining the cavity
(Gerbe et al., 2008).
We observed that GFP-positive cells lining the cavity rarely changed their
position. By contrast, deeper-lying cells tended to be more migratory, but
lost this property upon reaching the cavity. Thus, even a randomly directed
migration of deeper-lying cells would suffice to drive the majority of cell
sorting because PrE precursors, once in contact with the cavity, will remain
there. The probability of PrE precursors reaching the cavity would also be
enhanced by adhesive contacts with any neighbouring PrE precursors that
already line the cavity. The adhesive properties of PrE precursors have
previously been implicated in PrE formation (reviewed by
Yamanaka et al., 2006).
Once a PrE precursor reaches the cavity, its position may be maintained by
establishing cell polarity and epithelial properties, to the competitive
exclusion of non-polarised cells. In a study of mouse blastocyst formation, it
was shown that differences in epithelial properties between subsets of cells
were sufficient to influence their propensity to occupy an outer position and
to contribute to the TE (Plusa et al.,
2005). Thus, PrE precursors occupying the cavity surface may have
a propensity to flatten, due to cell polarisation. Increased flattening would
cause cells to occupy a greater surface area of the cavity, to the competitive
exclusion of non-polarised EPI precursors. Deeper-lying PrE precursors that
maintain contact with such cells would thus be able to maintain proximity to
the cavity.
An additional selective mechanism, using apoptosis, appears to account for
the minority of PrE precursors that fail to come into contact with the cavity.
The prevalence of apoptosis in deeper-lying GFP-positive cells after the
64-cell stage suggests that the stabilisation of PrE-specific transcription
factor expression in strongly GFP-positive cells excludes EPI potential, and
leaves the cell with either of two possible outcomes: contributing to the PrE
or defaulting to apoptosis. More weakly GFP-expressing cells showed a tendency
to downregulate expression, suggesting that they may retain the potential to
form EPI. In agreement with our observations, a surge in the frequency of cell
death in the ICM of embryos of 60-110 cells was previously reported
(Copp, 1978). We suggest that
one of the primary functions of apoptosis within the ICM is the elimination of
inappropriately positioned PrE precursors. This is supported by our
observation that the probability of GFP-positive cells undergoing apoptosis is
much greater for inner cells than for those in the PrE layer.
In summary, our results reconcile the two apparently disparate models of PrE lineage specification within the ICM of the mouse blastocyst. Our observations lead us to propose a three-step model in which stochastic expression of lineage-specific transcription factors, at the 16- to 32-cell stage, precedes the maturation of mutually inhibitory regulatory pathways, leading to a salt-and-pepper distribution of EPI and PrE precursors in the ICM after the 64-cell stage. This is followed by cell sorting, which may be largely, if not completely, explained by a passive, selective mechanism involving cell movement, cell adhesion and apoptosis.
Supplementary material
Supplementary material for this article is available at
http://dev.biologists.org/cgi/content/full/135/18/3081/DC1
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ACKNOWLEDGMENTS |
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|
Footnotes |
|---|
Present address: Department of Zoology, University of Melbourne, Victoria,
Australia
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