Chromosomal instability leading to aneuploidy is pervasive in early human embryos1,2,3 and is considered as a major cause of infertility and pregnancy wastage4,5. Here we provide several lines of evidence that blastocysts containing aneuploid cells are worthy of in vitro fertilization transfer. First, we show clinically that aneuploid embryos can lead to healthy births, suggesting the presence of an in vivo mechanism to eliminate aneuploidy. Second, early development and cell specification modelled in micropatterned human ‘gastruloids’ grown in confined geometry show that aneuploid cells are depleted from embryonic germ layers, but not from extraembryonic tissue, by apoptosis in a bone morphogenetic protein 4 (BMP4)-dependent manner. Third, a small percentage of euploid cells rescues embryonic tissue in mosaic gastruloids when mixed with aneuploid cells. Finally, single-cell RNA-sequencing analysis of early human embryos revealed a decline of aneuploidy beginning on day 3. Our findings challenge two current dogmas: that a single trophectoderm biopsy at blastocyst stage to perform prenatal genetic testing can accurately determine the chromosomal make-up of a human embryo, and that aneuploid embryos should be withheld from embryo transfer in association with in vitro fertilization.
Although chromosomal mosaicism is common in human embryos derived from in vitro fertilization (IVF), most IVF centres consider the mosaic or aneuploid embryos to be abnormal, and thus withhold them from transfer into uteri6. Indeed, more than 80% of these embryos contain aneuploid blastomeres, while only 12.5% of fertilized oocytes are aneuploid7; approximately 60% of embryos are euploid–aneuploid mosaic and only 22% are euploid8. The use of preimplantation genetic testing for aneuploidy (PGT-A) before embryo transfer to screen out aneuploidy has been proposed to improve delivery rates and reduce miscarriages in association with IVF9 and has become an increasingly common clinical practice. Whether PGT-A improves IVF outcomes has, however, remained controversial10,11,12. The high false-positive and false-negative rates in PGT-A means that a substantial number of diagnosed aneuploid or euploid embryos are actually mosaic13. As spontaneous and IVF pregnancies demonstrate similar levels of mosaicism (12% versus 6.3%)14, excluding all embryos containing aneuploid cells from transfer would therefore deprive patients of options.
To test whether mosaic human embryos develop normally, we report on 32 women who underwent frozen-thawed embryo transfers with 77 blastocysts that were diagnosed as mosaic and aneuploid by PGT-A. Nine clinical pregnancies were established (28.2%) from these transfers, 4 of which miscarried (44.4% of pregnancies, 12.5% of cycles), and the remaining ones were delivered (15.6%; Supplementary Table 1). Characteristics of participants and IVF cycles are presented in Supplementary Table 2. Median age was 40.6 ± 4.1 years. Our observed pregnancy and live birth rate matched or even exceed the national average of expected outcomes for age-matched individuals who did not use PGT-A diagnostics (18% pregnancy and 12% live birth rate at age 40)15. Interestingly, while all transferred embryos were aneuploid, prenatal chromosomal analyses performed with chronic villus biopsies (CVS) or amniocenteses in delivered pregnancies uniformly revealed normal karyotypes. Comprehensive chromosomal analysis on the products of conception from three participants who miscarried in the first trimester showed that two demonstrated the same chromosomal abnormalities as previously detected in the original PGT-A analysis of the transferred embryos (Supplementary Table 1, patients 8 and 9), while the third (patient 7) had a normal karyotype, indicating the elimination of aneuploidy and suggesting a different cause for her miscarriage. Furthermore, successful cases of transferring diagnosed mosaic embryos have been reported16,17,18. Together, these clinical results unveil the developmental capacity of mosaic embryos, thereby supporting the possibility of a developmental rescue mechanism.
Indeed, an innate ability of the embryo to select against aneuploid cells has been demonstrated using a mouse model19. The mouse aneuploid cells of the inner cell mass (ICM) were eliminated by apoptosis, whereas trophectodermal aneuploid cells displayed proliferative defects but less apoptosis19. Even small percentages of euploid cells in the ICM resulted in normal euploid offspring19,20,21. However, in contrast to humans, spontaneous occurrence of aneuploidy is uncommon in mice, affecting less than 1% of embryos22. Therefore, a human model is needed to unravel the consequences of aneuploidy in early development and decipher the cellular and molecular mechanisms underlying the depletion or decrease of mosaicism during pregnancy.
In order to establish a development model for aneuploidy, we used RUES2 (NIHhESC-09-0013) human embryonic stem (ES) cells with reversine, a small molecule inhibitor of monopolar spindle 1 kinase that inactivates the spindle assembly checkpoint23. Reversine is known to cause severe chromosome segregation defects that efficiently generate aneuploidy in many cell types19,24,25. We confirmed the high efficiency of reversine treatment in generating aneuploid RUES2 cells using metaphase spreads; 94% of cells were aneuploid after 24 h of reversine treatment (0.5 μM; Extended Data Fig. 1a–c). Reversine treatment yielded a karyotypically heterogeneous aneuploid cell population, with metaphase spreads exhibiting abnormal chromosome numbers with random nuclear fragmentation and abnormal chromosome crossovers. Karyotying showed that the parental RUES2 cell line exhibits a completely normal karyotype (Extended Data Fig. 1d), whereas the induced aneuploid cells comprise, but are not limited to, trisomies and monosomies (Extended Data Fig. 1e). Additionally, while remaining pluripotent, RUES2 cells treated with reversine for 48 h displayed an enlarged size and irregular nuclear shape, a morphology typically associated with aneuploidy26 (Fig. 1a and Extended Data Fig. 1f,g). We then cultured these reversine-treated cells in confined geometry on 500-μm- and 1,000-μm-diameter circular micropatterned substrates for another 48 h under pluripotency conditions to further investigate their stability and physiology (Fig. 1b). The colonies of reversine-treated cells comprised fewer cells than the colonies of untreated cells after 48 h of micropattern culture (Fig. 1c). Reversine-treated RUES2 cells exhibited increased expression of the DNA damage repair marker p53 but no difference in expression of the apoptosis marker CASP3 compared with untreated cells, and more importantly, the cells maintained the state of pluripotency, as indicated by expression of the pluripotency markers OCT4 (also known as POU5F1) and NANOG (Fig. 1d and Extended Data Fig. 1h).
We previously showed that gastruloids (models of human gastrulation derived from human ES cells) provide a robust and highly quantitative in vitro model to study early differentiation events with subcellular resolution and in real time27. When stimulated with BMP4, RUES2 cells self-organize and differentiate to generate embryonic and extraembryonic fates that are patterned in radially symmetrical domains with ectoderm at the centre, extraembryonic and endoderm at the edge and mesoderm in between. In the extraembryonic territory, cells express markers of early trophectoderm that are expressed in day 5 embryos (for example, CLDN4, SLC7A2 and TACSTD2), thus modelling aspects of preimplantation development, including that of trophectodermal lineages28. To probe the effects of aneuploidy at these critical stages of development, aneuploid RUES2 gastrulpoids generated with reversine treatment were cultured in 1,000 μm and 500 μm micropatterned colonies and then stimulated with BMP4. In response to BMP4, almost all cells in the aneuploid gastruloid colonies were positive for GATA3, suggesting global conversion or differential survival of extraembryonic tissue (Fig. 2a). SOX2+ and BRA+ domains were largely absent. We further verified the extraembryonic identity of the remaining GATA3+ cells in the aneuploid gastruloids, which showed expression of CDX2 and TFAP2A at the protein level as well as nuclear YAP staining, a characteristic of trophectoderm29,30 (Extended Data Fig. 2a). We demonstrated previously that cell density has a strong influence on the self-organization of gastruloids31. To investigate whether the loss of patterning in reversine-treated aneuploid gastruloids was caused by low cell density, we generated compact aneuploid micropatterned colonies by either directly seeding twice as many cells or allowing cells to divide further to reach a density comparable to or higher than that of control untreated colonies before stimulation. Increasing density had no effect on the observed patterning phenotype, thus eliminating the possibility of density-related effects (Extended Data Fig. 2b,c).
To evaluate the extent to which differentiation plays a role in the survival from aneuploidy, we compared micropatterned colonies derived from reversine-treated aneuploid RUES2 cells with and without 48 h BMP4 stimulation. In the absence of BMP, the colonies remained pluripotent, exhibiting high density and without an obvious pattern of widespread cell death (Fig. 2b). Despite seeding the same quantity of cells initially, we detected significantly lower cell numbers after 48 h of BMP4 treatment in the colonies derived from reversine-treated RUES2 (Fig. 2b,c), indicating that cell death during gastruloid formation is not a consequence of reversine but of induced BMP-stimulated differentiation. In response to BMP4, aneuploid RUES2 cells differentiated with prompt downregulation of pluripotent marker NANOG in the majority of cells and an increase in cell death marker CASP3 in gastruloids (Fig. 2b,d). To further evaluate how aneuploid cells perform compared with euploid cells following treatment with BMP4, fluorescently tagged reversine-treated aneuploid (RFP-H2B-RUES2, pink) and untreated control euploid (VENUS-H2B-RUES2, green) cells were mixed in a 1:1 ratio in the same micropatterned colonies and cultured for 48 h either with or without BMP4. Live-cell imaging showed that, while the euploid control RUES2 predominate in both conditions, reversine-treated cells were more severely depleted in the colony that was induced by BMP4 (Supplementary Video 1, right) compared with non-induced colonies in pluripotency medium (Supplementary Video 1, left). Therefore, differentiation (that is, escape from pluripotency) reduces cell tolerance towards aneuploidy. To address cell-type specificity in the BMP4-dependant apoptosis, we performed an experiment addressing the consequence of inducing aneuploidy after allowing BMP4 to begin differentiation. We reasoned that since reversine takes at least one cell cycle to generate aneuploidy, and BMP4 transduces signals within less than 1 h, differentiation will be induced before aneuploidy exert its effects. Consistent with specification occurring before induction of aneuploidy, the cells of embryonic germ layers (SOX2+ and BRA+) were induced together with GATA3+ layer, in concentric rings. However, examination of p53 and CASP3 revealed a significant enhancement in the SOX2+BRA+ territory (Fig. 2e). This result demonstrates that aneuploidy-induced cell death exhibits lineage preference during early specification, and that the GATA3+ extraembryonic-like cell population is particularly resilient to aneuploidy.
These lineage-specific findings parallel studies in mouse embryos that detected a higher frequency of apoptosis in aneuploid cells in ICM than in trophectoderm, where reversine was also used to induce aneuploidy19,32. As aneuploidy in mouse embryos is rare compared with human embryos, the fact that aneuploidy can be depleted in vivo suggests evolutionary conservation of this embryonic activity. Notably, both pluripotent epiblast and differentiated trophectoderm cells tolerated aneuploidy and displayed significantly lower levels of apoptosis, suggesting the presence of a similar underlying mechanism. As pluripotent cells have been shown to lack key regulators of the cell cycle, which allow the bypassing of checkpoints, the tolerance of trophectoderm may also be due to cell cycle checkpoint regulation similar to the one in pluripotency33. Further studies of trophectodermal cell cycle checkpoints will clarify this possibility.
To probe the putative rescue mechanism during mosaic embryo development, we constructed a mosaic gastruloid model and investigated whether the presence of euploid cells can rescue the lineage formation and the spatial patterning of aneuploid gastruloids. To this end, we treated VENUS-H2B-RUES2 cells with reversine and mixed the treated cells at different ratios with non-tagged RUES2 cells to generate mosaic gastruloids (Fig. 3a (I–VI)). We used three ratios of reversine-treated VENUS-H2B RUES2:non-tagged RUES2 cells: 1:3 (25% aneuploid cells; Fig. 3a (I and IV)), 1:1 (50% aneuploid cells; Fig. 3a (II and V)) and 3:1 (75% aneuploid cells; Fig. 3a (III and VI)). As the control, we used the same mixing ratio to combine untreated VENUS-H2B-RUES2 with non-tagged RUES2 (Fig. Fig. 3 (VII–XII)). When aneuploid cells comprised 25% of the cell population, the gastruloids exhibited self-organization of normal spatial patterning and complete cell lineages compared with controls (Fig. 3a (I and IV) versus Fig. 3a (VII and X)). Gastruloids with 100% reversine-treated or untreated VENUS-H2B RUES had the same phenotypes as those with the parental RUES2 cell line (Fig. 3b). Surprisingly, the mosaic micropatterned colonies containing 50% or 75% of aneuploid cells were also able to form gastruloids with normal self-organization of embryonic and extraembryonic germ layers (Fig. 3a (II, III, V and VI)). However, we note that the SOX2+ territory decreases in size with increasing aneuploidy ratio (Fig. 3c). Characterization and quantification of the cells in mosaic gastruloids revealed a significantly lower percentage of aneuploid SOX2+ cells (18.32%, 15.79% and 27.16% lower for 1:3, 1:1 and 3:1 ratios, respectively). Of note, a significantly higher percentage of aneuploid cells in the mosaic gastruloid contributed to GATA3+ extraembryonic cells (16.90%, 17.22% and 30.02% higher for 1:3, 1:1 and 3:1 ratios, respectively) (Fig. 3d). The tendency of aneuploid cells to acquire extraembryonic fate seems more pronounced if the mosaic gastruloids contain fewer euploid cells, suggesting the existence of a threshold of depletion. Together, our results demonstrate that even a small fraction of euploid cells in the mosaic gastruloid is sufficient to generate normal self-organizing radial patterns, with aneuploid cells being preferentially allocated to the trophectodermal layer.
Our clinical and gastruloid data suggest the existence of an apoptotic depletion mechanism for aneuploid cells in embryos that depends on their differentiation trajectory and timing. We sought to probe the timing of the depletion of aneuploid cells by investigating its prevalence in early human embryos. We analysed two existing single-cell RNA-sequencing (scRNA-seq) datasets from a total of 101 embryos34,35. The chromosome-wide analysis was used to identify gross abnormalities in gene expression and infer aneuploidy from scRNA-seq data using a strategy similar to the one described by Griffiths et al.36 (Fig. 4a). The data from Petropolous et al. analyse 1,529 cells from 88 preimplantation embryos34 collected from embryonic day 3 (E3) to E7, while the data from Zhou et al. analyse of 5,911 cells from 21 embryos from E6 to E14, where cells from day 8 and beyond were collected from in vitro attached embryos35. For each chromosome in a cell, we calculated a normalized sum of expression levels across all genes and converted it to a z-score. When z-score values for the X chromosome between E3 and E7 were calculated34, two distinct cell populations were observed at E3–E5, reflecting the existence of both male and female cells. These populations subsequently merged into a single cluster by E6–E7 (Fig. 4b), indicating the inactivation of one X chromosome in female cells during preimplantation stages34. Since even in this extreme case of variation in sex chromosome gene expression, the z-score values were confined between ±3, values outside this range are probably due to aneuploidy. After identifying aneuploidy in single cells, we calculated the percentage of aneuploidy both for each day and, independently, for the two datasets to avoid any bias introduced by technical variance (Fig. 4c). A high aneuploidy rate (81.82%) was observed in preimplantation embryos at E3, with a sharp decline starting from E4–E5. The aneuploidy rate decreased to 5.36% by E7. Our analysis showed that data from both datasets demonstrate consistent aneuploidy rates from E6 to E8, while the data from Zhou et al.35 additionally displayed a persistently low aneuploidy rate up to E14 (Fig. 4d). Consistent with the cell aneuploidy rates, the aneuploidy ratio per embryo was highly variable, being more abundant in the early stages, and showed a decline over time. On day 3, every embryo in the dataset was more than 50% aneuploid, whereas the aneuploidy rate in mosaic embryos decreased from E3 to E6, with the median aneuploidy rate decreasing from 83.33% to 11.1% from E3 to E4. Embryos with 100% aneuploid cells were not present after E6, suggesting their lack of potential for survival (Fig. 4e). Overall, our analysis shows that aneuploidy is pervasive in human embryos, but the prevalence of aneuploid cells in mosaic embryos progressively declines, suggesting a mechanism that eliminates aneuploidy similar to the one that we have described in gastruloids.
Recent bioinformatic analysis of scRNA-seq data from in vitro cultured human post-implantation embryo further revealed a higher tolerance to aneuploidy in the trophectoderm lineage than in primitive endoderm and epiblast lineages derived from ICM37. The enrichment of aneuploidy tolerance in trophectoderm compared with other lineages becomes more extreme as development proceeds. Based on our gastruloid data, which recapitulated this lineage-specific observation, we propose that aneuploid cells in mosaic embryos tend to survive in the trophectoderm, with little influence on ICM development. This could explain why confined placental mosaicism (CPM) is common, occurring in at least 2% of ongoing natural pregnancies38, and why the prevalence of genetic mosaicism is low in postnatal DNA samples39. A recent study showed that chromosome instability frequently occurs in both naturally conceived and IVF pregnancies and that the prevalence decreases at later stages of prenatal development14. Some aneuploid cells in early-cleavage-state embryos were segregated into placental lineage only14. This in vivo finding offers strong evidence in support of our proposal. Given that studies have demonstrated that CPM40,41,42,43 does not appear to be associated with adverse pregnancy outcomes, and that an extensive load of copy number variations was detected in human placenta44, aneuploidy in the extraembryonic lineage should not necessarily be viewed as abnormal. The tolerance towards chromosome instability in extraembryonic tissue, like that seen in cancer, might be associated with rapid proliferation, migration and invasiveness. The presence of aneuploidy in trophectoderm of blastocyst-stage embryos may, therefore, have physiological functions.
In sum, this study presents a comprehensive picture of aneuploid cell fate in early human development. Our results directly demonstrate the developmental potential and robust aneuploidy depletion ability of mosaic embryos, thus challenging the clinical relevance of ploidy analysis in trophectoderm biopsies as part of routine IVF practice. Gastruloids that recapitulate early embryonic development serve as a competent in vitro model for probing the underlying mechanism of the observed aneuploidy elimination in human embryos. To our knowledge, lineage-specific behaviours of aneuploid cells in humans have not previously been examined with quantification at the cellular level. Analysis of the available embryo single-cell data also suggests an aneuploidy elimination mechanism similar to the one described in gastruloids. Furthermore, the effects of BMP4-induced differentiation in aneuploid human ES cells presented in this study pave the way to future studies on the role of BMP signalling in aneuploidy depletion, and on the precise order and timing of events, particularly how the gastruloid results relate to the earlier aneuploidy depletion inferred from currently available single-cell transcriptomics. Additional studies using more targeted strategies that generate aneuploidy with defined karyotypes will be required to further address the molecular basis of aneuploidy depletion. Newly developed 3D models of a human epiblast will also provide methods to investigate embryonic aneuploid cell fate acquisition in a spontaneously symmetry-breaking model of human embryogenesis45.
Individuals undergoing embryo transfers at the Center for Human Reproduction, New York (CHR) with PGT-A showing chromosomal-abnormal designated embryos, in addition to routine IVF consent, signed an additional informed consent since 2014, specifically advising them of the hypothetically increased risks that such transfers may lead to chromosomal-abnormal ongoing pregnancies and/or miscarriages and mandating early prenatal diagnosis by CVS or amniocentesis. Anonymized clinical data extraction for this study was approved by the Institutional Review Board of the CHR (ER03302015/01).
Participant selection and transfer of diagnosed aneuploid embryos
Embryo transfers occurred at the CHR. As the CHR does not recommend PGT-A, almost all embryos in this study were produced at other IVF centres, where they were cryopreserved. Embryos with reported trisomies of chromosomes 13, 18 or 21 or sex chromosome abnormalities were not transferred unless patients insisted on such transfers, in which case they were asked to sign an additional ‘against medical advice’ consent. Other trisomies were transferred after genetic counselling and followed a routine protocol. The morphology of the transfered embryos were graded by the Garden score46. Transfer results from 32 individuals with ages ranging from 27 to 47 were analysed. Patient and IVF cycle characteristics including patient number and age are presented in Supplementary Table 2. Their initial chromosomal analyses were performed by national PGT-A laboratories, using next-generation sequencing and, in a few cases, comparative genomic hybridization (Supplementary Table 2), following guidelines of the Preimplantation Genetic Diagnosis International Society47. Pregnancy outcomes were determined by routine CVS or amniocentesis in later first or second trimesters of pregnancy.
Human ES cells (registered RUES2 human ES cell line NIHhESC-09-0013) were grown in mouse embryonic fibroblast-conditioned HUESM medium (MEF-CM) supplemented with 20 ng ml−1 basic fibroblast growth factor (bFGF). The culture medium was changed daily. Cells were tested for mycoplasma infection before beginning experiments and again at two-monthly intervals. The tissue culture dishes that cells were grown on were coated with Geltrex (Life Technologies) solution. The dishes were coated overnight at 4 °C and then incubated at 37 °C for at least 20 min before the cells were plated. Cells were passaged using Gentle Cell Dissociation Reagent (Stem Cell Technologies) and replated in MEF-CM with 10 μM ROCK inhibitor Y-27632 (Abcam). For reversine treatment, cells that were approximately 75% confluent were treated with 0.5 μM reversine (Cayman Chemicals) in MEF-CM media supplemented with 20 ng ml−1 bFGF with a medium change after 24 h.
DAPI staining of chromosome metaphase spreads from RUES2 cells
To obtain chromosomes at the mitotic stage, we treated RUES2 cells with colchicine (Sigma) at a final concentration of 0.3 μg ml−1 for 2 h in the culture medium before collecting them. Cells were dissociated from the culture dish with StemPro Accutase (Life Technologies) and then resuspended in 50 μl 1.0% sodium citrate solution (in distilled water) and incubated on ice for 5 min. To spread the chromosomes, 5 μl cell suspension was loaded onto each slide by pulling the pipette tip from one side of the slide to the other while pushing the cell suspension out of the tip. Fixative solution (3:1 methanol:acetic acid, Sigma) was immediately added onto each slide in a drop by drop manner. The slides were air-dried thoroughly and then pre-wetted in PBS supplemented with 0.5%(v/v) Photo-Flo (Kodak) and 1% (w/v) bovine serum album (Sigma) for 15 min before staining. The slides were stained with 200 μl 4 μM DAPI (Thermo Fisher Scientific) for 5 min at room temperature and then washed twice with PBS supplemented with 0.5%(v/v) Photo-Flo for 5 min and once with distilled water for 5 min. ProLong Gold antifade mounting medium (Thermo Fisher Scientific) was used to mount coverslips onto slides. G-banding karyotyping was conducted by a commercial service from Cell Line Genetics.
Flow cytometry of aneuploid cells
To analyse the cells obtained after reversine treatment (0.5 mM for 24 h), we used the two-camera ImageStream (X) imaging flow cytometer. The control and reversine-treated RUES2 samples, 263,000 and 67,500 cells, respectively, were stained with DAPI and collected on ImageStream X (Amnis). The instrument combines the high capacity and immunofluorescent sensitivity and capacity of a flow cytometer with high-resolution microscopy and high-content image analysis pipelines. Images were captured using a ×40 objective and with INSPIRE acquisition software (Amnis v.6.2). Post-acquisition data analysis was performed using IDEAS software (Amnis v.6.2). Single cells in focus were gated using Gradient RMS (focus), then plots of area versus aspect ratio of the bright-field channel were used to select the main cluster of cells to be further analysed. Next, the intensity and area of the DAPI channel were used to characterize the two populations. The intensity feature was used as input for the cell cycle module of IDEAS.
Generation of cell-tracking RUES2 lines
Two cell-tracking human ES cell lines (VENUS-H2B-RUES2 and RFP-H2B-RUES2) were generated from the parental RUES2 line using the ePiggyBac system. Accordingly, ePiggyBac plasmids were designed. To generate RFP-H2B-RUES2 line, we nucleofected the cells with an ePiggyBac plasmid containing RFP-H2B driven by the CAG promoter and also containing a blasticidin resistance (BSD) gene (ePB-BSD-CAG-RFP-H2B). Cells were then selected with 5 μg ml−1 BSD. To generate the VENUS-H2B-RUES2 line, we nucleofected the cells with an ePiggyBac plasmid containing H2B-VENUS driven by the CAG promoter and also containing a puromycin resistance (Puro) gene (ePB-Puro-CAG-H2B-VENUS). Cells were selected with 1 μg ml−1 of puromycin. Cells that survived selection were passaged as single cells using StemPro Accutase (Life Technologies), plated in MEF-CM supplemented with 10 mM ROCK inhibitor and allowed to grow into colonies. Individual colonies were picked and plated into separate wells with growth medium and ROCK inhibitor. Each clone was isolated and controlled for normal karyotype (G-banding) and pluripotency maintenance.
Micropattern culture and gastruloid differentiation
The culture chips for RUES2 to form gastruloids were made using micropatterned glass coverslips (Arena A and Arena EMB A) from Cytoo (Cambridge). The micropatterns were coated with 800 ml of 10 μg ml−1 recombinant laminin 521 (BioLamina) in PBS with calcium and magnesium (PBS++) for 3 h at 37 °C before cell plating. The micropatterned coverslips were stored in 35 mm plastic tissue culture dished and then serially washed with PBS++ to remove laminin. After two washes with PBS, RUES2 cells were dissociated from the culture dish with StemPro Accutase (Life Technologies) for 5 min and resuspended in MEF-CM with 10 μM ROCK inhibitor. Eight-hundred-thousand cells in 2 ml of MEF-CM with 20 ng ml−1 bFGF, 100 μg ml−1 Normocin (Invivogen) and ROCK inhibitor were seeded in each cultured dish containing one micropatterned coverslip. The ROCK inhibitor was removed from the medium 3 h after seeding and cells were incubated overnight (12–18 h) before BMP4 induction. To induce gastruloid differentiation, the cells grown on the micropattern in the culture dish were cultured with 2 ml induction medium (MEF-CM supplemented with 20 ng ml−1 bFGF, 100 μg ml−1 normocin and 50 ng ml−1 BMP4 (R&D systems)) for 48 h.
Cells were washed once with PBS and then fixed with 4% paraformaldehyde (Electron Microscopy Sciences) for 30 min. After three washes for 5 min with PBS, samples were blocked and permeabilized with blocking buffer (PBS supplemented with 3% normal donkey serum (Jackson Immunoresearch) with 0.3% Triton X-100 (Sigma)) for 30 min. Cells were then incubated with primary antibodies diluted in blocking buffer at room temperature for 2 h and followed by three washes with PBS. Secondary antibodies conjugated to Alexa 488, Alexa 555, Alexa 594 or Alexa 647 (1:1,000 dilution, Molecular Probes for mouse, rabbit and goat; Thermo Fisher Scientific) and 10 ng ml−1 DAPI were added for 30 min before three washes with PBS. The coverslips were then mounted on to glass slides using ProLong Gold antifade mounting medium (Invitrogen) for imaging. Primary antibodies used are listed in Supplementary Table 3.
Imaging and image analysis
Chromosome spreads were imaged under a microscope (Olympus BX51) with a ×100 oil-immersion objective. Image process and chromosome counts were performed with ImageJ (FIJI). All micropattern confocal images were acquired on a Zeiss Inverted LSM 780 laser scanning confocal microscope with a ×10, ×20 or ×40 water-immersion objective. Quantification of fluorescent intensity and area fraction was performed by ImageJ (FIJI) using the Analyse/Measure command. Quantification for cell numbers on the micropattern colonies was performed with Ilastik and ImageJ. In brief, for segmentation of individual cells, we first used Ilastik classification to separate foreground from background. The classifier was trained for each experiment on the DAPI images of four randomly chosen colonies from that experiment. The cell counting was then conducted using the Analyze/Analyze Particles command in ImageJ. Quantification of the cell-tracking line for different cell fates was also performed in ImageJ using the colocalization plugin for ComDet version 0.4.1. The quantification of the radial area of ectoderm (SOX2+) of each colony was quantified using custom software written in Matlab. Live-cell-tracking imaging for the cell-tracking RUES2 lines that generated Supplementary Video 1 was performed with a spinning-disc microscope (CellVoyager CV1000, Yokogawa), acquired using the CellVoyager CV1000 spinning disk confocal system (Yokagawa/Olympus) with a ×20 dry objective, deconvolved using Autoquant software, and analysed in Imaris.
Aneuploidy detection from scRNA-seq
To detect the aneuploidy rate in human embryos, we analysed two published scRNA-seq datasets, which contain 1,529 cells from 88 E3–E7 embryos34 and 5,911 cells from 21 E6–E14 embryos35. These two sets of data were analysed separately to avoid the bias induced by the technical variance. The method applied uses chromosome-wide expression imbalances to identify aneuploidies from scRNA-seq data as previously described36, which provides quantitative aneuploidy calls. In brief, expression level (expressed as counts per million) was normalized the by the median of the gene across cells, and highly expressed genes (median > 50 counts) were selected. For each chromosome and cell, expression levels across genes were summed. The sum was normalized by the number of considered genes on each chromosome to make it comparable across chromosomes. Within each cell, we convert this normalized sum into a score (S-score) centred at 1 across chromosomes. If no chromosome within a cell has gain or loss of copy number, this score will deviate randomly around 1. Otherwise, their scores will be increased or decreased accordingly. To demonstrate whether a chromosome displays aberrant copy number, we then converted this score into a Z-score where the variance was estimated separately for each chromosome across cells using the median absolute deviation. We defined cells with any chromosome expression profile above |3| to be putatively aneuploid. Aneuploid chromosomes were identified using a false discovery rate-corrected P < 0.1, where the P-value was obtained using Student’s t-distribution. To call an aneuploidy, we not only required that the corrected P-value was less than 0.1 but also imposed an effect-size threshold such that cell–chromosomes where 0.8 < S < 1.2 were not considered significant.
Statistical analysis and reproducibility
No statistical methods were used to predetermine sample size. The gastruloid experiments were randomized as each cell colony analysed was randomly selected from both control and experimental groups. Each experiment was repeated independently at least three times with similar results, unless otherwise stated. The investigators were not blinded to allocation during experiments and outcome assessment. Unbiased analysis of data was carried out wherever possible. All statistical procedures performed are indicated in the figure captions. P-values are calculated using Student’s t-test.
Further information on research design is available in the Nature Research Reporting Summary linked to this article.
Publicly available expression matrices of human embryo single-cell RNA-seq data were obtained from ArrayExpress E-MTAB-3929 and the Gene Expression Omnibus (accession number GSE109555). All other data supporting the findings of this study are available from the corresponding author upon reasonable request. Source data are provided with this paper.
For the chromosome-wide analysis of aneuploidy in human embryos using scRNA-seq data, a strategy similar the one described in ref. 36 was used. The specific code used for these data is available upon request. Source data are provided with this paper.
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This work was supported by private funds provided by the Foundation for Reproductive Medicine to the Center for Human Reproduction, and private funds from The Rockefeller University. M.Y. was supported by a fellowship from the Lalor Foundation. We are particularly grateful to the patients who moved their embryos for transfer to CHR. We thank our colleagues at CHR and members of the Brivanlou Laboratory for their advice and constructive criticism; A. North for access and advice to the Rockefeller Core Imaging Facility; S. Mazel and S. Semova of the Flow Cytometry Research Center; and J.-M. Santel and A. Souza for their assistance in preparing this manuscript under the challenging COVID-19 situation in New York City.
N.G. and A.H.B. are co-founders of OvaNova Inc. A.H.B. is a co-founder of Rumi Scientific Inc. The other authors declare no competing interests.
Peer review information Nature Cell Biology thanks Joris Vermeesch and the other, anonymous, reviewers for their contribution to the peer review of this work.
Publisher’s note Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.
Extended Data Fig. 1 Reversine treatment induces aneuploidy in RUES2.
a, Representative images of metaphase spreads stained with DAPI of reversine-treated and untreated control RUES2. RUES2 treated with reversine (24 h) have abnormal chromosome numbers. Arrows indicate chromosome fragmentation or abnormal crossover. b, Percentage of aneuploid cells detected in reversine-treated (80 cells) and control RUES2 (100 cells). n = 3 independent experiment replicates. c, Chromosome counts from metaphase spreads of reversine-treated (80 cells) and control cells (100 cells). d, G-banding karyotype of untreated RUES2 cell line. e, G-banding karyotypes of reversine-treated RUES2 cells. f, Representative cell images of reversine-treated and untreated control RUES2 taken by imaging flow cytometry. Reversine-treated RUES2 exhibit different nuclear (DAPI) morphology than control RUES2. BF, bright field. g, Plot of DNA content (mean nuclear area; DAPI) obtained from flow cytometry of reversine-treated and untreated RUES2. Compared to control, reversine-treated RUES2 displays larger nuclei. h, Normalized fluorescent pixel intensity and area fraction were quantified for P53 and CASP3 on micropatterned colonies after 48 hr culture in pluripotency medium. Reversine-treated cell colonies have a significant higher level of P53 in both fluorescence intensity and area fraction compared with untreated colonies. CASP3 level has no significant difference between treated and control groups. N=3 biologically independent cell colonies Results are shown as the mean ± s.d. and statistical significance was calculated using a two-tailed Student’s t-test. For a and f, scale bar= 10 μM.
Extended Data Fig. 2 Depletion of embryonic cell fate domain in aneuploid gastruloids is density-independent.
a, RUES2 (standard amount; 8x105) were seeded on laminin-coated micropatterns and cultured with 50 ng/ml BMP4 for 48 hr to generate gastruloids. The cells in gastruloids derived from reversine-treated RUES2 express CDX2, TFAP2A at the protein-level and show nuclear YAP staining consistent with it acquiring a trophectoderm/ amnion fate. b, Standard (8x105) or twice the standard amount of reversine-treated aneuploid RUES2 was seeded on laminin-coated micropatterns and cultured with 50 ng/ml BMP4 to form gastruloids. The gastruloids derived from aneuploid RUES2 with both cell concentrations are depleted of the ectoderm center (SOX2+) and mesoderm ring (BRA+). c, RUES2 were seeded and treated with 0.5 μM reversine for 48 hr on the micropatterns before BMP4 induction. Direct reversine treatment on the micropatterns allows the aneuploid cells to proliferate to the ideal density before BMP4 induction. The gastruloids derived are still depleted of SOX2+ and BRA+ domains. For a-c, scale bar = 100 μm. Only 500μm micropattern substrates are shown.
Supplementary Fig. 1
Supplementary Table 1: IVF cycles leading to pregnancy. Supplementary Table 2: Patient/IVF cycle characteristics. Supplementary Table 3: Antibody information.
Supplementary Video 1
Supplementary Video 1: 48 h live (time-lapse) imaging of micropatterned colonies with 50% control RUES2 (VENUS-H2B, green) and 50% reversine-treated RUES2 (RFP-H2B, pink) with/without BMP4 induction. 30 min acquisition.
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Yang, M., Rito, T., Metzger, J. et al. Depletion of aneuploid cells in human embryos and gastruloids. Nat Cell Biol 23, 314–321 (2021). https://doi.org/10.1038/s41556-021-00660-7
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