Inferring and perturbing cell fate regulomes in human brain organoids

Experimental methods

Stem cell and organoid culture

We used six human iPS cell lines (Hoik1, Wibj2, Kucg2 from the HipSci resource47; 409B2 from the RIKEN BRC cell bank; 01F49i-N-B7 (B7) from Institute of Molecular and Clinical Ophthalmology Basel; and WTC from the Allen Institute) and three human ES cell lines (H1-PAX6YFP (H1) and H9 from WiCell and HES-3 NKX2.1GFP/w (HES3) from the Murdoch Children’s Research Institute). Stem cell lines were cultured in mTESR1 (Stem Cell Technologies, 05851) with mTeSR1 supplement (Stem Cell Technologies, 05852) and supplemented with penicillin–streptomycin (1:200, Gibco, 15140122) on Matrigel-coated plates (Corning, 354277). Cells were passaged 1–2 times per week after dissociation with TryplE (Gibco, 12605010) or EDTA in DPBS (final concentration 0.5 mM) (Gibco, 12605010). The medium was supplemented with Rho-associated protein kinase (ROCK) inhibitor Y-27632 (final concentration 5 µM, STEMCELL Technologies, 72302) the first day after passage. Cells were tested for mycoplasma infection regularly using PCR validation (Venor GeM Classic, Minerva Biolabs) and found to be negative. A total of 4,500–5,000 cells were plated in ultralow-attachment plates (Corning, CLS7007) to generate brain organoids using a whole-brain organoid differentiation protocol2. The use of human ES cells for the generation of brain organoids was approved by the ethics committee of northwest and central Switzerland (2019-01016) and the Swiss federal office of public health.

Single-cell RNA-seq, ATAC–seq and multiome experiments for the developmental time course

Brain organoids were generated from four different stem cell lines (H9, 409B2, Wibj2, Hoik1) simultaneously. Brain organoids of the same batch were dissociated at multiple time points of the course of brain organoids development. We collected these single-cell suspensions from an embryoid body time point (day 4), the time points of neuronal induction (days 7, 9 and 11) and after embedding in Matrigel and starting the neuronal differentiation process (days 12, 16, 18, 21, 26, 31 and 61). Organoids of the four different cell lines were pooled on the basis of size and dissociated together, and the cell lines were later demultiplexed on the basis of the single-nucleotide polymorphism information. Multiple organoids of each line were pooled together to obtain a sufficient number of cells. For the early time points, 15 organoids per cell line were pooled, decreasing this number to minimally 3 organoids for the later time points (Supplementary Table 1). For time points just after Matrigel embedding, Matrigel was dissolved in Cell Recovery Solution (Corning, 354253) for 15 min at 4 °C. The organoids were cut in halves and washed three times with HBSS without Ca2+ and Mg2+ (STEMCELL Technologies, 37250). Single-cell suspensions were acquired by dissociation of the organoids with a papain-based dissociation (Miltenyi Biotec, 130-092-628). Prewarmed papain solution (2 ml) was added to the organoids and incubated for 15 min at 37 °C. Enzyme mix A was added before the tissue pieces were triturated 5–10 times with 1,000 μl wide-bore and P1000 pipette tips. The tissue pieces were incubated twice for 10 min at 37 °C with trituration steps in between and after with P200 and P1000 pipette tips. Cells were filtered with consecutively with 30 µm and 20 µm preseparation filters and centrifuged. Cells were resuspended and viability and cell count were assessed using a Trypan Blue assay on the automated cell counter Countess (Thermo Fisher Scientific). Cell suspensions were split in two and resuspended in CryoStor CS10 (STEMCELL Technologies, 07952) and cryopreserved at −80 °C. The next day, cryotubes were transferred to liquid nitrogen for storage until the scRNA-seq and scATAC-seq experiments were performed.

The cryopreserved single-cell suspensions of each time point were thawed by warming up the cryo for 1–2 min in a water bath at 37 °C and directly centrifuged in 10 ml prewarmed DMEM with 10% FBS. Cells were washed twice with PBS + 5% BSA and filtered through a 40 µm cell strainer (Flomi). For scATAC–seq, nuclei were isolated according to the protocol provided by 10x genomics (Demonstrated protocol CG000169 Rev D) using the low-input protocol and a lysis time of 3 min. Nuclei were loaded at a concentration that would result in the recovery of 10,000 nuclei. In case of less nuclei recovered, the maximum number of nuclei was targeted. scATAC–seq libraries were generated using the Chromium Single Cell ATAC V1 Library & Gel Bead Kit. Before sequencing, an additional clean-up step was performed to enrich shorter fragments by applying a double-sided (1.2–0.75×) clean-up with AMPureXP beads (Beckman Coulter) and Illumina Free Adapter Blocking Reagent was used to reduce potential index hopping. The libraries were sequenced on the Illumina NovaSeq platform.

For scRNA-seq, cells were put in a concentration after counting and viability checking that enabled targeting 10,000 cells and, in case the cell number was not sufficient, all cells were loaded. scRNA-seq libraries were generated using the Chromium Single Cell 3′ V3 Library & Gel Bead Kit. Single-cell encapsulation and library preparation were performed according to the manufacturer’s protocol.

Single-cell multiome datasets were generated from day 15 brain organoids of the stem cell lines Wibj2, Hoik1, 409B2, B7 and WTC, and day 19 brain organoids of stem cell lines (Kucg2, WTC, B7, and H1 and HES-3 NKX2.1GFP/w) using the Chromium Single Cell Multiome ATAC + Gene Expression kit. Before nucleus isolation, organoids were dissociated with the papain-based dissociation. Nuclei were isolated according to the protocol provided by 10x genomics (demonstrated protocol CG000365, Rev B) in the lysis buffer with final amount of 0.01% Tween-20 and 0.01% Nonidet P40 Substitute and a lysis time of 3 min. Single-cell encapsulation and library preparation were performed according to the manufacturer’s protocol.

Libraries were pooled, FAB treated and sequenced on the Illumina NovaSeq platform. A summary of all single-cell experiments is provided in Supplementary Table 1.


Organoids were washed in PBS before fixing in 4% PFA at 4 °C overnight. The samples were washed three times with PBS and the organoids were then transferred to a 30% sucrose solution for 24–48 h for cryoprotection. Finally, organoids were transferred to plastic cryomolds (Tissue Tek) and embedded in OCT compound 4583 (Tissue Tek) for snap-freezing on dry ice. For immunohistochemical stainings, organoids were sectioned in slices of 10 µm thickness using a cryostat (Thermo Fisher Scientific, Cryostar NX50). Organoid sections were quickly washed in PBS to remove any residual OCT and post-fixed in 4% PFA for 15 min at room temperature. The sections were then incubated in antigen-retrieval solution (HistoVT One, Nacalai Tesque) at 70 °C for 20 min. Excess solution was washed away with PBS and the tissue was incubated in blocking-permeabilizing solution (0.3% Triton X-100, 0.2% Tween-20 and 5% normal donkey serum in PBS) for 1 h at room temperature. Next, the sections were incubated overnight at 4 °C in blocking-permeabilizing solution containing mouse anti-SOX2 (1:200, Sigma-Aldrich, AB5603), rabbit anti-TUJ1 (1:200, BioLegend, 801201) and goat anti-GLI3 (1:200, Novus Biological, AF3690) antibodies. The next day, the sections were rinsed three times in PBS before incubation for 1 h at room temperature with 1:500 secondary antibody (donkey anti-rabbit Alexa 488, ab150073 and donkey anti-mouse Alexa 568, ab175472 and donkey anti-goat Alexa 647, ab150135) in blocking-permeabilizing solution. Finally, the secondary antibody solution was washed off with PBS and the sections were stained with DAPI before covering with ProLong Gold Antifade Mountant medium (Thermo Fisher Scientific). Stained organoid cryosections were imaged using a confocal laser scanning microscope, and six different z-plane images (z-step = 2–3 µm) were acquired using a ×20 magnification objective. The images were further processed using Fiji.

Whole-mount HCR RNA-FISH

Probe sets, amplifiers and buffers were ordered from Molecular Instruments. HCR in situ hybridization was performed according to the manufacturer’s instructions by Molecular Instruments with small changes. In brief, 19-day-old organoids were washed once with PBS and transferred to a tube containing fresh 4% PFA at 4 °C and were fixed overnight at 4 °C. The samples were washed three times with PBST and then dehydrated with a PBST–methanol gradient (25%, 50%, 75% to 100%) and stored at −20 °C in 100% methanol until use. The samples were rehydrated with a similar series of graded methanol–PBST washes for 5 min each on ice and washed an additional time with PBST. The samples were then treated with 10 µg ml−1 proteinase K (Invitrogen, 25530-049) for 3 min at room temperature. The samples were washed twice with PBST for 5 min and then post-fixed with 4% PFA for 20 min at room temperature and subsequently washed three times with PBST for 5 min. The organoids were prehybridized in probe hybridization buffer for 30 min at 37 °C. Then, 1 pmol of each probe set was diluted into probe hybridization buffer and the samples were incubated overnight at 37 °C. The samples were washed four times with probe wash buffer at 37 °C and washed twice more with 5× SSCT. The organoids were incubated in amplification buffer for 10 min at room temperature before adding the precooled hairpin mixture diluted in amplification buffer to incubate overnight at room temperature. The excess hairpins were removed with three 5 min washes as well as two longer washes of 30 min. Organoids were stained with DAPI during one of the 30 min washes. The samples were stored at 4 °C and mounted on a µ-Slide chamber (Ibidi, 80807) and covered with 1% agarose. Images were acquired with lambda scanning followed by spectral unmixing on the Zeiss LSM980 system and processed using Fiji.

Doxycycline-inducible Cas9 nuclease and nickase cell line

The human iPS cell line 409B2 was used to create an iCRISPR–Cas9 nickase (Cas9n) and an iCRISPR–Cas9 line as described previously48. The doxycycline-inducible Cas9-expressing cell line was generated by introducing two transcription activator-like effector nucleases (TALENs) targeting the AAVS1 locus, which has shown to be effective for sustained transgene expression, and two TALEN constructs with donor plasmids. One of the donor plasmids contained a constitutive reverse tetracycline transactivator (AAVS1-Neo-M2rtTA) and the other one contained a doxycycline-inducible expression cassette (Puro-Cas9). A D10A mutation was introduced by site-directed mutagenesis of the original Puro-Cas9 donor using the Q5 mutagenesis kit (New England Biolabs, E0554S) to generate the Cas9n. The cell lines used were tested for the proper expression of pluripotency markers SOX2, OCT4, TRA-1-60 and SSEA, quantitative PCR confirmed the doxycycline-inducible Cas9n and digital PCR was used to exclude off-target integration49. Both cell lines showed normal karyotypes after generation, but the iCRISPR–Cas9 line acquired a common stem cell abnormality over time. A total of 55% percent of the cells showed a derivative chromosome 2 with a long arm of chromosome 1 (bands q11q44) attached to the long arm of one chromosome 2 (band q37).

Vector and lentivirus preparation for the perturbation experiment

The perturbation experiment was performed according to the CROP-seq protocol as described previously17 with some small alterations. The experiment was performed in organoids derived from the inducible Cas9 nuclease line, which contains a Puro selection marker. To be able to select for cells that received the CROP-seq vector, Puro was exchanged for eGFP to isolate cells by fluorescence. We selected targeted TFs that had previously been shown in the literature to have correlated expression patterns during human cortex development in organoids and primary tissues, and have been studied in vertebrate models and shown to be involved in regulating forebrain development. The selected TFs had minimal expression in iPS cells and neuroectoderm stages to minimize the chances that organoid development was impaired during the early stages of organoid development. All of the selected TFs were expressed in the organoid dorsal telencephalon, and most were also expressed in at least one other branch. Three gRNA per targeted gene were designed by Applied Biological Materials and synthesized by IDT as 74 base oligonucleotides with 19 and 35 bases of homology to the hU6 promoter and guide RNA backbone, respectively. Oligonucleotides were pooled in equal amounts and were assembled in the vector backbone by Gibson’s isothermal assembly. The plasmid library was sequenced to validate the complexity of the pooled plasmid library. We used 10 ng of plasmid library for generating a sequencing library with a single PCR reaction. Illumina i7 and i5 indices were added by PCR and the library was sequenced on the Illumina MiSeq platform. After validation, lentiviruses were generated by the Viral Core Facility of Charité Universitätsmedizin Berlin.

Generation of mosaic organoids for perturbation experiment

The iCRISPR–Cas9 line was cultured on Matrigel in mTesr1 supplemented with penicillin–streptomycin (1:200) and Cas9 was induced 2 days before lentiviral transduction by adding 2 µg ml−1 doxycycline. Then, 24 h later, cells were dissociated into single cells with TrypLE and 300,000 cells of the iCRISPR–Cas9 cells were plated in at least 12 wells of Matrigel-coated 6-well plates in mTesr1 supplemented with penicillin–streptomycin (1:200), Y-27632 (final concentration 5 µM) and 2 µg ml−1 doxycycline. Next, 24 h later, cells were transduced with a low multiplicity of infection (MOI) where less than 30% of the cells were GFP+ to ensure that the majority GFP+ cells received only one lentivirus per cell. The viral particles were added to the culture medium (mTesr1 supplemented with penicillin–streptomycin, Y-27632 and 2 µg ml−1 doxycycline). Then, 24 h later, the medium was exchanged for mTesr1 supplemented with penicillin–streptomycin and 2 µg ml−1 doxycycline until 70% confluency was reached. Cells were then sorted with fluorescence-activated cell sorting (FACS) for GFP+ cells to enrich for CROP-seq-vector-positive cells and plated on Matrigel-coated plates in mTesr1 supplemented with 100 μg ml−1 Primocin (InvivoGen, ant-pm-1) and Y-27632 (final concentration 5 µM). When cells reached 70% confluency, whole-brain organoids were generated as mentioned previously.

Preparation of single-cell transcriptomes from mosaic perturbed organoids

After 2 months, single organoids and a pool of four organoids were dissociated using a papain-based dissociation kit (Miltenyi Biotec, 130-092-628) as described previously. Cells were sorted using FACS. Cell viability and number was assessed using the Trypan Blue assay and the Countess automated cell counter (Thermo Fisher Scientific). Finally, cells were diluted to an appropriate concentration to obtain approximately 7,000 cells per lane of the 10x microfluidic chip. scRNA-seq libraries were generated using the Chromium Single Cell 3′ V3 Library & Gel Bead Kit. The expression libraries were FAB-treated and sequenced on the Illumina NovaSeq platform.

gRNA detection from single-cell cDNA

gRNA were amplified from 60 ng of cDNA remaining from scRNA-seq preparation with three separate PCR reactions similar to reactions described previously50. First, cDNA was amplified using PCR broadly targeting the outer part of the U6 promoter. Subsequently, the inner portion of the U6 promoter adjacent to the guide sequence and a TruSeq Illumina i5 adapter. Finally, we added Illumina sequencing i7 adapters. PCRs were monitored using quantitative PCR to avoid overamplification and, after every PCR reaction, the samples were purified using SPRI beads (Beckman Coulter) and libraries were sequenced at 1:10 proportion of the transcriptome library on the Illumina NovaSeq system.

gRNA detection from gDNA

Cells from different stages of the organoid protocol were collected (iPS cell, embryoid body, embedded organoids and organoids day 30). QuickExtract (30–60 µl, Epicentre, QE0905T) was added to the cell pellets or organoids and the suspension was incubated at 65 °C for 10 min, 68 °C for 5 min and 98 °C for 5 min to extract the DNA. The same PCR was used to validate the library complexity of the plasmid library17. The PCR was performed using the KAPA2G Robust PCR Kit (Peqlab, 07-KK5532-03) using the supplied buffer B and 5 µl isolated DNA. The following program was used: 95 °C for 3 min; 35 cycles of 95 °C for 15 s, 65 °C for 15 s and 72 °C for 15 s; 72 °C for 60 s. Libraries were sequenced using the Illumina MiSeq system (Nano kit) .

GLI3-KO and control line generation

Two days before lipofection, iPS cell medium was supplemented with 2 µg ml−1 doxycycline (Clontech, 631311) to induce Cas9n expression. Two guides were designed using the Broad Institute’s CRISPR design tool ( The following guide pair was selected: ACAGAGGGCTCCGCCACGTGTGG, CCGCGGGACGGTGTTTGCCATGG. The Alt-R CRISPR–Cas9 System (IDT) was used for guide delivery with lipofection according to the manufacturer’s protocol. To form the crRNA–tracrRNA complex in a 3 µM final concentration for each guide complex, 1.5 µl of each guide crRNA was combined with 3 µl tracrRNA and 44 µl nuclease-free water. For the reverse transfection, 1.5 µl of the crRNA–tracr complex mix and 0.75 µl RNAiMAX (Invitrogen, 13778075) were diluted in 47.75 µl OPTI-MEM (Gibco, 1985-062) for each replicate and incubated for 20 min at room temperature in a well of 96-well plate coated with Matrigel (Corning, 35248). During incubation, around 70% confluent cells were detached with TryplE (Gibco, 12605010), centrifuged and resuspended in 1 ml mTeSR with Y-27632 (final concentration 10 µM, STEMCELL Technologies, 72302). After complex incubation, cells were diluted 30 or 60 times in 100 µl mTeSR with Y-27632 (STEMCELL Technologies, 72302) and 2 µg ml−1 doxycycline (Clontech, 631311) and the cell suspension was added to a well containing the transfection complexes. After 24 h, the medium was replaced with mTeSR1 medium and cells were allowed to recover for 72 h. Wells at 70% confluence were used for further processing after 72 h. Cells were passaged as single cells in a Matrigel-coated (Corning, 35248) six-well plate in mTeSR medium with 1:200 penicillin–streptomycin (Gibco, 15140122) and Y-27632 (STEMCELL Technologies, 72302). Low amounts of cells were plated per well to avoid the fusion of colonies. The medium was changed daily and Y-27632 was added for the first 72 h to prevent apoptosis of the single cells. When colonies were apparent, single colonies were picked by scraping with a 10 μl pipette tip. Two-thirds of the cell suspension was plated in a single well of a Matrigel-coated 96-well plate in mTeSR1 supplemented with 1:200 penicillin–streptomycin and Y-27632. The other portion of the cell suspension was pelleted and used for validation of frameshift mutations by sequencing. Validated clones were expanded, cryopreserved and karyotyped. The three selected lines, one WT and two KO lines, showed a normal karyotype.

Validation of KO lines by sequencing

The cell pellets of picked colonies were resuspended in 10 µl QuickExtract (Epicentre, QE0905T) and the suspension was incubated at 65 °C for 10 min, 68 °C for 5 min and 98 °C for 5 min to extract the DNA. A PCR reaction was performed with primers containing Illumina sequencing adapters for the targeted locus of the GLI3 gene. Amplification was performed using the KAPA2G Robust PCR Kit (Peqlab, 07-KK5532-03) using the supplied buffer B and 2 µl of extracted DNA. The following program was used: 95 °C for 3 min; 35 cycles of 95 °C for 15 s, 65 °C for 15 s and 72 °C for 15 s; and 72 °C for 60 s. Unique P5 and P7 Illumina indices were added to 0.5 µl of the previous PCR product with a second PCR program (98 °C for 30 s; 25 cycles of 98 °C for 10 s, 58 °C for 10 s and 72 °C for 20 s); and 72 °C for 5 min), using the Phusion HF MasterMix (Thermo Fisher Scientific, F-531L). The double-indexed libraries were pooled and purified with SPRI beads. Purified libraries were sequenced on the MiSeq (Illumina) system resulting in paired-end sequences of 2 × 150 bp. LeeHom51 was used to trim the adapters after base calling using Bustard (Illumina).

Western blotting

GLI3 WT and KO organoids of day 15 were collected into Laemmli buffer, homogenized with a pestle (Fisherbrand, 12-141-368) and sonicated for 15 cycles using the Bioruptor Plus. Subsequently, two high and low amounts of protein extractions and ladder (Thermo Fisher Scientific, 26620) were run on an 8% SDS–PAGE (Bio-Rad System) and transferred to a PVDF membrane using Wet-Blot. After blocking for 20 min with 4% milk powder in PBS + 0.1% Tween-20, the primary antibody (1:1,000, stock 0.5 µg µl−1, R&D systems, AF3690) was incubated overnight at 4 °C. After washing three times for 7 min at room temperature in PBS + 0.1% Tween-20 on a shaker, the secondary goat IgG HRP-conjugated antibody (1:7,000, R&D systems HAF017) diluted in 4% milk in PBS + 0.1% Tween-20 was incubated for 2 h. The enhanced chemiluminescence signal was recorded using the ChemiDoc system. The loading control β-catenin (primary antibody: stock 1:10,000, Cell Signaling technologies, L54E2; secondary antibody: stock 0.8 µg µl−1 1:7,000, Jackson ImmunoResearch, 115-035-003) was probed on the same membrane and loading was also controlled by Ponceau staining. Raw images are provided in Supplementary Fig. 1.

Generation of single-cell transcriptome and multiome of GLI3-KO and WT organoids

Organoids of GLI3 WT and KO iPS cells were generated simultaneously and dissociated with a papain-based dissociation kit (Miltenyi Biotec, 130-092-628) as described above. scRNA-seq was performed on day 45 of organoid development for both KO lines and the WT line for two independent organoid batches. After dissociation, cell viability was checked, cells were counted and 7,000 cells were targeted per lane of the 10x microfluidic chip. Libraries were generated with the Chromium Single Cell 3′ V2 Library & Gel Bead Kit and sequenced on the Illumina HiSeq platform.

Combined scRNA-seq and scATAC-seq were generated using the Chromium Single Cell Multiome ATAC + Gene Expression kit. In the case of SHH treatment, GLI3 WT organoids were treated with or without 200 ng ml−1 SHH (R&D systems, 1845-SH-025/CF) every day for three days before the experiment on day 19. GLI3-KO and WT organoids were dissociated with the papain-based dissociation kit on day 19. Nuclei were isolated according to the protocol provided by 10x genomics (demonstrated protocol CG000365, Rev B) with a lysis time of 3 min. The gene expression and accessibility libraries were FAB-treated and sequenced on the Illumina NovaSeq platform.

Bulk CUT&Tag for GLI3 and H3K27ac

Single-cell suspensions of 18- or 23-day-old brain organoids were prepared using the Miltenyi Neural Tissue Dissociation Kit (P) (Miltenyi Biotec, 130-092-628) according to the manufacturer’s guidelines. Cells were counted and directly transferred into CUT&Tag Wash buffer supplemented 0.01% digitonin (20 mM HEPES pH 7.5; 150 mM NaCl; 0.5 mM spermidine; 1× Roche protease inhibitor cocktail). Per experiment, 1.5 million cells were used and incubated with 1.5 µg anti-GLI3 antibodies (R&D systems, AF3690) or 1 µg anti-H3K27ac antibodies (Diagenode, C15410196). All of the following steps were performed as described previously52. The protein A-Tn5 was purified in house as described previously52. The final libraries were sequenced on the NovaSeq platform with paired-end 2 × 50 bp read length.

Data analysis methods

Preprocessing of scRNA-seq data from the organoid time course

We used Cell Ranger (v.3.0.2) with the default parameters to obtain transcript count matrices by aligning the sequencing reads to the human genome and transcriptome (hg38, provided by 10x Genomics, v.3.0.0). Count matrices were further preprocessed using the Seurat R package (v.3.2)19. First, cells were filtered on the basis of unique molecular identifier (UMI) counts, the number of detected genes and the fraction of mitochondrial genes. The threshold of mitochondrial gene fraction was held constant across datasets (<0.2). As sequencing depth varied between time points, the threshold of UMI count and number of detected genes was set individually for each sample as follows: days 4 and 7: #UMI: >10,000, <80,000; #features: >3,000, <8,000; day 11: #UMI: >10,000, <60,000; #features: >3,000, <8,000; day 12: #UMI: >2,500, <40,000; #features: >1,000, <6,000; day 16: #UMI: >10,000, <60,000; #features: >3,000, <8,000; days 18 and 21: #UMI: >2,500, <60,000; #features: >1,500, <8,000; day 26: #UMI: >2,500, <60,000; #features: >2,000, <8,000; day 31: #UMI: >2,500, <50,000; #features: >2,400, <7,500; day 61: #UMI: >1,000, <60,000; #features: >1,000, <8,000.

Transcript counts were normalized to the total number of counts for that cell, multiplied by a scaling factor of 10,000 and subsequently natural-log transformed (NormalizeData()).

Preprocessing of scATAC–seq data from the organoid time course

We used Cell Ranger ATAC (v.1.1.0) with the default parameters to obtain fragment files by aligning the sequencing reads to the human genome and transcriptome (hg38, provided by 10x Genomics, v.1.1.0). Peaks were called from the fragment file using MACS2 (v.2.2.6). Both the fragment files and the peak count matrices were further preprocessed using Seurat (v.3.2)19 and Signac (v.1.1)53. First, peaks were filtered by width (<10,000 bp, >20 bp) to retain only high-quality peaks. Furthermore, the following quality control metrics were computed using Signac: a transcription start site (TSS) enrichment score (TSSEnrichment()), nucleosome signal (NucleosomeSignal()), the percentage of reads in peaks and the ratio of reads in genomic blacklist regions. Subsequently, cells were filtered based on the following metrics: percentage of reads in peaks > 30%; number of peak region fragments > 5,000; blacklist ratio < 0.003; nucleosome signal < 5; number of TSS fragments > 5,000; TSS enrichment score > 2.

We then created a unified set of peaks from the union of peaks from all of the samples by merging overlapping and adjacent peaks. The unified set of peaks was requantified for each sample using the fragment file (FeatureMatrix()). Peak counts were normalized by term frequency–inverse document frequency (tf-idf) normalization using the Signac functions RunTFIDF().

Demultiplexing of different lines based on single-nucleotide variant information

Cells pooled from different stem cell lines were demultiplexed using demuxlet54. Genotyping information was called using bcftools based on (sc)RNA-seq (B7, H1 and HES3) or DNA-seq data (H9 and 409B2)25,55 or downloaded from the HipSci (WIBJ2, HOIK1) or Allen Institute (WTC) website. All files were merged using bcftools and sites with the same genotypes in all of the samples were filtered out. Demuxlet was run with default settings. Cells with ambiguous or doublet assignments were removed from the data. For all other cells, the best singlet assignment was considered.

Integration of transcriptome and chromatin accessibility data

To create a shared feature space between the two modalities, gene activities were calculated from chromatin accessibility data using the Signac function GeneActivity() with the default parameters and subsequently log-normalized with a scaling factor of 10,000. For each time point and line separately, we performed CCA on gene activities and gene expression data using the Seurat function RunCCA() based on 2,000 features, which were selected using the Seurat function SelectIntegrationFeatures(). In CCA space, we performed minimum-cost maximum-flow (MCMF) bipartite matching between the modalities as described previously20 ( The function get_cost_knn_graph() was used with knn_k = 10, null_cost_percentile = 99, capacity_method=’uniform’ and otherwise the default parameters. On the basis of the bipartite matches, matched cells were summarized to metacells containing measurements from both modalities. If multiple cells from one modality were included in a metacell, the arithmetic mean between cells was calculated.

Removal of cells with glycolysis signature

An additional quality-control step was applied at the level of metacells to remove cells with transcriptomic signatures of glycolysis upregulation. This was based on primary cell type predictions using public human fetal brain scRNA-seq data (Nowakowski dataset)4. We fit a multinomial logistic regression model with lasso regularization penalty (alpha = 1), using gene expression ranks of the Nowakowski dataset as the training set, to predict the cell type identity of metacells in the organoid developmental time course. Metacells that were predicted to be of ‘glycolysis’ identity were excluded from the dataset. To fit the logistic regression model and automatically determine the regularization parameter lambda through cross-validation, we used the function cv.glmnet() from the glmnet R package.

Integration of different lines and time points

Integration of lines and time points was performed using the log-normalized gene expression data of metacells. To select a set of features suitable for integration of all lines and time points, we selected the union of the 100 most variable genes for each time point separately (local) as well as across the full dataset (global). Analogously, we selected the union of locally and globally variable transcription factors (Supplementary Table 2). We used the union of the selected genes and TFs and further excluded cell-cycle-related genes56 from the set. Next, we computed cell cycle scores using the Seurat function CellCycleScoring(). Subsequently the data were z-scaled, cell cycle scores were regressed out (ScaleData()) and Principal Component Analysis (PCA) was performed using the Seurat function RunPCA(). We used the first 10 principal components (PCs) to integrate the different time points in the dataset using the CSS method21. To remove any remaining cell cycle signal for any downstream tasks, we again regressed out the cell cycle scores from the integrated CSS matrix. To obtain a two-dimensional representation of the data, we performed UMAP57 using RunUMAP() with spread = 0.5, min.dist = 0.2 and otherwise the default parameters.

Calculation of motif enrichment scores

Position weight matrices of human TF-binding motifs were obtained from the CORE collection of JASPAR202058. Motif positions in accessible chromatin regions were determined using the R package motifmatchr (v.1.14) ( through the Signac function FindMotifs(). Enrichment scores of motifs in accessible regions were calculated for each metacell using chromVAR59 through the Signac function RunChromVAR().

RNA velocity calculation

To obtain count matrices for the spliced and unspliced transcriptome, we used kallisto (v.0.46.0)60 by running the command line tool loompy fromfastq from the Python package loompy (v.3.0.6) ( Spliced and unspliced transcriptomes were summarized to the metacell level as described above. RNA velocity was subsequently calculated using scVelo (v.0.2.2)27 and further analysed using scanpy (v.1.7.0)61. First, 2,000 highly variable features were selected using the function scanpy.pp.highly_variable_genes(). Cell cycle genes56 were excluded from this feature set and the dataset was subsetted to the resulting gene set. Subsequently, moments were computed in CSS space using the function scvelo.pp.moments() with n_neighbors = 30. RNA velocity was calculated using the function with mode=‘stochastic’ and a velocity graph was constructed using with the default parameters. To order cells in the developmental trajectory, a root cell was chosen randomly from cells of the first time point (day 4) and velocity pseudotime was computed with The obtained velocity pseudotime was further rank-transformed and divided by the total number of metacells in the dataset.

Annotation of organoid developmental stages

To annotate different organoid developmental stages, we first divided the dataset into 20 bins on the basis of quantiles of velocity pseudotime. For each bin, we computed the average gene expression and peak accessibility across metacells and computed the pairwise Pearson correlation between log-normal gene expression values of each bin. From the correlation coefficient r, we defined a distance metric as 1 − r and used it to perform hierarchical clustering using the ward.D2 method as implemented in the stats R package (hclust()). On the basis of the resulting clusters, bins were manually annotated as PS cells, neuroectoderm, neuroepithelium, NPCs or neurons.

Identification of stage-specific chromatin access

To find sets of peaks with stage-specific accessibility, we computed for each stage the percentage of metacells in which each peak was detected. We then computed a specificity score by dividing the detection percentage for each stage by the detection percentage of all other metacells. We filtered peaks with an in-stage detection percentage of >15% and a stage specificity of >1.5. From these peaks, we selected the top 5,000 peaks with the highest specificity score. Using these specific peak sets for each stage, we used GREAT31 with the GRCh38 genome assembly and otherwise the default parameters to obtain functional enrichment results. We reported GO biological process enrichments with FDR < 0.01 and that were supported by >30 foreground regions.

Inference of regional cell-fate trajectories

To resolve the regional cell fate branches we relied on CellRank (v.1.3.0)28 to compute transition probabilities into terminal cell states and PAGA62 to obtain a graph abstraction of the transcriptomic manifold. First, terminal neuronal states were annotated manually using VoxHunt (v.1.0.0)8 based on the top 20 structure markers. To resolve the developmental trajectories leading up to the emergence of neurons with distinct regional identities, transition probabilities to each of the terminal states were computed for each cell using CellRank. A transition matrix was constructed by combining a velocity kernel (VelocityKernel()) and a connectivity kernel (ConnectivityKernel()) with weights of 0.5 each. Absorption probabilities for each of the predefined terminal states were computed using the GPCCA estimator. From these probabilities, we computed a transition score by ranking the absorption probabilities and normalizing by dividing by the total number of metacells. We then constructed a graph abstraction of the dataset by high-resolution clustering using the Louvain algorithm63 with a resolution of 20. We used PAGA to compute the connectivites between clusters ( and summarized transition scores for each of the clusters. To find branch points at which the transition probabilities into different fates diverge, we then constructed a nearest-neighbour graph between the high-resolution clusters based on their transition scores (k = 30). We further pruned the graph to retain only edges between nodes with a connectivity score of >0.2 and edges going forward in pseudotime, that is, from a node with a lower velocity pseudotime to a node with a higher velocity pseudotime. The resulting graph is directed with respect to pseudotemporal progression and represents a coarse-grained abstraction of the fate trajectory, connecting groups of cells with both similar transition probabilities to the different lineages and high connectivities on the transcriptomic manifold. To assign fate identities to each branch in the graph, we first selected the nodes with the highest transition probability and pseudotime for each of the terminal states as tips. We then performed 10,000 random walks with 200 steps from each tip along edges backwards in pseudotime using the igraph R package (v.1.2.6) ( Next, we computed for each node the visitation frequency from each of the terminal states. We then assigned branch identities to each node on the basis of the visitation frequencies as follows: if a node’s visitation frequency from one tip was more than 100× higher than from the next highest tip, it was unambiguously assigned the identity of this tip. If the visitation frequencies from multiple tips were within 100× of each other, then the node was assigned the identity of all of such tips. Nodes that were assigned both the dorsal telencephalic and ventral telencephalic identity were relabelled as ‘telencephalon’. Nodes that were assigned all three identities were labelled as ‘early’ to indicate that their fate was not yet committed. Nodes that could not be reached through this procedure were assigned the identity of the node with the highest connectivity score. The final labelled graph was visualized using the Fruchterman–Reingold layout algorithm as implemented in the igraph R package.

Analysis and integration of multiome data in the neuroepithelial stage

Initial transcript count and peak accessibility matrices were obtained with Cell Ranger Arc (v.1.0.0) and further preprocessed using the Seurat (v.3.2)19 and Signac (v.1.1)64 R packages. Transcript counts were log-normalized and peak counts were tf-idf-nomalized. On the basis of the RNA modality, the data were integrated with previously described data from the neuroepithelial stage using Seurat CCA integration with the default parameters. PCA was performed on integrated, log-normalized and z-scaled transcript counts and Louvain clustering was performed using the Seurat function FindClusters() with a resolution of 0.8.

Identification of CREs from multiome data

CREs for genes were discovered by linking peaks to genes by co-accessibility and co-expression between ATAC and RNA modalities, respectively. This was achieved using the Seurat function LinkPeaks() with the default parameters.

GRN inference with Pando

We developed Pando to infer GRNs while taking advantage of multimodal single-cell measurements, where both the RNA and the ATAC components are either measured for each cell or integrated to obtain metacells or clusters with both modalities. The core GRN inference algorithm in Pando can be summarized in four main steps:

  1. (1)

    Selecting candidate regulatory genomic regions.

  2. (2)

    Scanning regions for transcription factor binding motifs.

  3. (3)

    Selecting region–TF pairs for each target gene.

  4. (4)

    Constructing a regression model with region–TF pairs as independent variables and the expression of the target gene as the response variable.

The coefficients (or importances) of this model can now be seen as a measure of interaction between the region–TF pair and the downstream gene, resulting in a regulatory graph. In the following sections, we will describe these steps in more detail.

Selection of candidate regions for GRN inference

To narrow the set of genomic regions that are taken into account for each target gene when constructing the model, we can take advantage of prior knowledge about the potential importance of these regions. Genomic sequence conservation is one such criterion that indicates the relevance of a stretch of DNA, as it has been maintained by natural selection. Thus, we first intersected the peak regions in the ATAC–seq data with the set of PhastCons conserved elements29 from an alignment of 30 mammals (obtained from As exonic regions tend to be conserved regardless of their regulatory relevance, we further excluded exonic regions from this set. Furthermore, we considered candidate cCREs derived from the ENCODE project30. For this, we obtained the set of all human cCREs from (GRCh38) and intersected it with peak regions. The union of the resulting conserved and cCRE regions was carried forward as the set of candidate regions for GRN inference.

Construction of an extended motif database for GRN inference

Because TFs need to be matched with potential binding sites, the availability of a binding motif is required for a TF to be included in the GRN. We therefore aimed to gather motif information for all TFs relevant in our dataset. First, we selected the union of the 4,000 most variable genes in each individual time point (Supplementary Table 2). All TFs in this set were considered to be relevant. We then obtained binding motifs from JASPAR (2020 release)58 taking into account the CORE and the UNVALIDATED collection. For TFs for which no binding motif was available in JASPAR, we further considered the CIS-BP database65. Where possible, motifs with direct experimental evidence were prioritized over inferred motifs and motifs that were inferred based on other JASPAR motifs were prioritized over the rest. For all relevant TFs that were also not covered by CIS-BP, motifs were inferred on the basis of protein sequence similarity to other TFs from the same family. Family information and protein sequences for all TFs were obtained from AnimalTFDB66 and pairwise multiple-sequence alignments were performed using the Needleman–Wunsch algorithm67 as implemented in needle from the EMBOSS software suite (v.6.5.7)68. For each query TF, we considered all TFs from the same family with a global sequence similarity of at least 20% and selected the motifs from the three most similar TFs. TF motifs from all sources were combined into one database and motif positions in accessible chromatin regions were determined using the R package motifmatchr (v.1.14) ( through the Signac function FindMotifs().

Coarse-graining expression and chromatin accessibility data

Before inferring the GRN, we coarse-grained the data to denoise and remove sparsity. First, we summarized the expression and chromatin accessibility of close cells using the pseudocell algorithm outlined in ref. 25. In brief, we randomly selected 30% of all cells in the dataset as the seed cells and constructed a territory for each seed with the ten nearest neighbours based on Euclidean distances using the top 20 PCs. If one cell was assigned to multiple territories, one was randomly chosen. For all cells contained in a territory, gene expression data were summarized using the arithmetic mean. For chromatin accessibility data, an accessibility probability for each territory was computed by averaging binarized read counts. We further performed latent semantic indexing (LSI) on the peak counts of each territory using the Signac functions RunTFIDF() followed by RunSVD(). On the basis of the top 20 LSI components, we further performed high-resolution clustering using the Louvain algorithm with a resolution of 100 and accessibility probabilities were further summarized to a cluster level by computing the arithmetic mean so that each cell in the cluster was represented by the same vector.

Linear model-based GRN inference

Pando used a regression-based approach to infer the regulatory interactions between TF–binding site pairs and the corresponding gene. Although the package implements a variety of regression models, here we used a linear model to perform network inference. Genomic coordinates for all genes were obtained via the R package EnsDb.Hsapiens.v86 ( For each gene, we considered a regulatory region encompassing the gene body and 100 kb upstream of the TSS. We then define a linear model on the log-normalized expression Y of the gene i based on all TF–binding-site interactions in this region:

$${Y}_{i}\,={\sum }_{j}{{\boldsymbol{\beta }}}_{j}\,{e}_{j}\,{a}_{j}+{\varepsilon },$$

where the log-normalized expression of transcription factor j is the accessibility probability of the peak that overlaps its binding region, βj is the fitted coefficient for this interaction and ε is the intercept. The fitted coefficients can then be interpreted as the regulatory effect of TF–binding-site pairs on the downstream genes. To fit the linear model, we use the function glm() from the stats R package using Gaussian noise and an identity link function.

Peak and gene module construction

To prune the network and retain only significant interactions, the fitted coefficients were tested for statistical significance using analysis of variance (ANOVA). We corrected for multiple testing using the Benjamini–Hochberg method to obtain an FDR-adjusted P value, to which a significance threshold of 0.05 was applied. The remaining connections were further summarized to extract sets of negatively (coefficient < 0) and positively (coefficient > 0) regulated target genes and regulatory regions for each transcription factor.

Pando implementation details

Pando was implemented as an R package and is available at GitHub ( Pando was designed for easy use and integrates smoothly with widely used single-cell analysis tools in R, namely Seurat and Signac. Its core functionality is implemented in four main functions:

initiate_grn() selects candidate regions from the dataset and initiates the object for GRN inference. The user can flexibly define custom sets of candidate regions to be taken into account by Pando.

find_motifs() scans candidate regions for transcription factor motifs. The motif database constructed in this work is included in the Pando package, but can also be manually supplied.

infer_grn() selects regulatory regions for each target gene and performs the model fitting. We implemented support for all generalized linear models provided by the stats R package, regularized linear models provided by the glmnet R package69, Bayesian regression models implemented through the brms R package70, gradient boosting regression through the xgboost R package70,71, as well as bagging and Bayesian ridge models through scikit-learn72. Where possible and necessary, we also implemented the appropriate statistical tests to obtain P values for the coefficients. For bagging ridge models, coefficients can be tested across estimators using a t-test or Wilcoxon rank-sum test. For the Bayesian ridge model, we obtain for each coefficient the mean and s.d. and subsequently calculate a P value based on the normal distribution. For Bayesian regression models obtained from brms, we calculated P values using the bayestestR R package73.

find_modules() constructs gene and regulatory modules for each transcription factor.

The implementation is flexible and enables the user to apply the Pando framework to a wide range of use-cases.

Visualization of the GRN

We sought to visualize the inferred transcription factor network based on both co-expression and regulatory relationships between transcription factors. First, we computed the Pearson correlation between log-normalized expression of all transcription factors in the network across all metacells in the atlas. From the correlation value r and estimated model coefficient β between all transcription factors i and j, we then computed a combined score s as

$${S}_{ij}={r}_{ij}\times \sqrt{| {\beta }_{ij}| }+1$$

resulting in a TF-by-TF matrix. We performed PCA on this matrix and used top 20 PCs as an input for UMAP as implemented in the uwot R package ( with the default parameters.

Region-specific GRN

The region-specific GRN was generated by incorporating region-specific accessibility profiles and region-specific TF expression into the Pando-inferred GRN. To get the region-specific accessibility, we first performed outlier analysis on the high-resolution clusters of pseudocells described above when summarizing the peak accessibility probabilities for Pando. In brief, for each predicted TF-binding region, a trimmed z-transformation was applied to the accessibility probabilities across clusters, with the average number of ATAC reads per pseudocell in the cluster as the covariate and regressed out. Here, instead of the arithmetic mean and s.d. across all clusters, only clusters with probabilities between the 5th and 95th percentiles were used to calculate the mean and s.d. for the transformation. The resulting z-scores were converted to P values based on the standard Gaussian distribution, which represents the statistical significance of outlier clusters with significantly lower accessibility (BH-corrected FDR < 0.01, close outliers). Alternatively, the statistical significance of outlier clusters with significantly higher accessibility was represented as 1 − P (BH-corrected FDR < 0.01, open outliers). Next, a step-wise procedure was used to define clusters with this region accessible. In brief, if no close outlier was found, the open outliers were considered as clusters with the region accessible. When close outliers were detected, all of the clusters except for the close outliers were considered to have the region accessible. When no outlier was detected, the region was considered to be accessible in all clusters. Next, this region accessibility was propagated from the clusters to the bimodal metacells. Given the regional identity of the metacells, a χ2 enrichment test was used to identify regions that significantly deplete metacells with the region accessible (two-sided χ2 test, BH-corrected FDR < 0.01, odds ratio < 0.5, inaccessible regions). For each region, the Pando-inferred TF–target regulation mediated by the inaccessible regions in one region was excluded from the region-specific GRN. Finally, the region-specific GRN was further trimmed by excluding any TF with a detection rate of less than 5% in metacells of the region.

Calculation of module activity and analysis of module branch specificity

On the basis of the GRN inferred by Pando, the activity of a transcription factor can be represented by the expression of the set of genes that it regulates (gene modules) or by the accessibility of its set of regulatory regions (regulatory modules). To calculate the activity of gene modules, we used the Seurat function AddModuleScore() with all genes included in GRN inference as the background (pool). For regulatory modules, we used the R package chromVAR (v.1.14)59 to obtain a set of background peaks (getBackgroundPeaks()). We then computed deviations in accessibility from the background for each regulatory module (computeDeviations()). Next, we assessed how the activity of positively regulated gene modules varied during neurogenesis over pseudotime and between branches. For this analysis, we excluded all cells from the PSC and neuroectoderm stage. We fit three gaussian linear models for each gene i module with module activity (Y) as the response variable and branch assignment and/or velocity pseudotime as the independent variables: (1) Yi ~ branch; (2) Yi ~ pseudotime; and (3) Yi ~ branch+pseudotime.

We used the R2 value of these models as the fraction of variance explained by branch (1), pseudotime (2), or branch and pseudotime (3). We further tested for differential module activity between the branches for each branch point separately using a Wilcoxon rank-sum test as implemented in the R package presto74. For the comparison of the dorsal and ventral telencephalon, we considered only cells in the top 30% pseudotime quantile (NPC and neuron stages). To visualize dorsal and ventral telencephalon-specific transcription factor networks, we first selected positively regulated gene modules of transcription factors with branch-specific expression (described above). For each branch, we then selected the top 15 modules of which the module activity was significantly upregulated (FDR < 0.05) based on the mean difference of module activity between the branches.

Preprocessing, integration and annotation of CROP-seq single-cell RNA-seq data

As with the organoid time course, count matrices were obtained using Cell Ranger (v.3.0.2) and further preprocessed using the Seurat R package (v.3.2)19. First, cells were filtered on the basis of UMI counts (>500, <30,000), the number of detected genes (>500, <6,000) and the fraction of mitochondrial genes (<0.1). Transcript counts were normalized to the total number of counts for that cell, multiplied by a scaling factor of 10,000 and subsequently natural-log transformed (NormalizeData()). The different samples were integrated using RSS25 based on the 2,000 most variable features (FindVariableFeatures()). In RSS space, we performed Louvain clustering with a resolution of 3. Regional identities as well as NPC/neuron identities were assigned to Louvain clusters using a combination of VoxHunt similarity maps and canonical marker genes. Cells annotated as off-target cell types such as mesenchyme and choroid plexus were removed from all downstream analyses.

Assignment of gRNA labels to cells

To assign gRNA labels to cells, reads obtained from amplicon sequencing were first aligned to the human genome and transcriptome (hg38, provided by 10x Genomics), which was extended with artificial chromosomes representing the CROP-seq-Guide-GFP construct17, using Cell Ranger. We observed that read counts of gRNA UMIs followed a bimodal distribution, with the lower peak probably representing sequencing or amplification artefacts. To extract the higher peak, we first fit a Gaussian mixture model with two components on natural log-transformed read counts using the function GaussianMixture() from the scikit-learn Python package72. We then used a probability cut-off of 0.5 to extract the mixture component with higher average read counts. From these gRNA UMIs, we constructed a cell x guide count matrix, which was further binarized to obtain the final cell-to-gRNA assignments.

Inference of perturbation probability

To account for a potential mixture of unperturbed and perturbed cells in the population, we inferred probabilities of a gRNA having a phenotypic effect on the cell using the strategy proposed previously15. Here a Bayesian approach is used to obtain the probability of a cell being perturbed given the observed transcriptome. To this end, a regression model is fit with the gene expression matrix as the response Y and the native gRNA assignments, cell and sample covariates as independent variables (X):

$$Y=X{\boldsymbol{\beta }}.$$

After fitting the model, the model fit is re-evaluated for each cell with the gRNA assignment set to 0 (X0). The difference of the squared errors of the two fits can then be transformed into a probability with:

$$P\left({X}_{j}\,=1\right)={\rm{logistic}}\left(\frac{{\sum }_{i}{[{Y}_{ij}-{X}_{0}{\beta }_{i}]}^{2}-{[{Y}_{ij}-{\hat{Y}}_{ij}]}^{2}}{2{\sigma }^{2}}\right)$$

where \({\rm{logistic}}(x)=\frac{1}{1+{{\rm{e}}}^{-x}}.\)

As in the original publication, we used linear regression model with elastic net regularization (alpha = 0.5) using Gaussian noise and an identity link function to fit the model based on 500 most-variable features. The regularization parameter lambda was automatically determined through cross-validation as implemented in the function cv.glmnet() from the glmnet R package. Models were fit for each gene i on log-normalized transcript counts Y with binary assignments X for each gRNA j as well as cell type, sample and number of detected genes as covariates:

$${Y}_{i}\propto {n}_{{\rm{f}}{\rm{e}}{\rm{a}}{\rm{t}}{\rm{u}}{\rm{r}}{\rm{e}}{\rm{s}}}+{\rm{s}}{\rm{a}}{\rm{m}}{\rm{p}}{\rm{l}}{\rm{e}}+{\rm{c}}{\rm{e}}{\rm{l}}{\rm{l}}\,{\rm{t}}{\rm{y}}{\rm{p}}{\rm{e}}+{\sum }_{j}{X}_{j}$$

After computing the above-described perturbation probabilities for each cell and gRNA, they were further summarized to a target gene level by taking the maximum probability among the three gRNAs targeting the same gene.

Determination of transcriptomic perturbation effects in the CROP-seq screen

To determine how gene KOs affect the transcriptomic state of neuronal populations arising in brain organoids, we used a linear model-based approach15. For each neuronal type, we inferred perturbation probabilities p for each target gene j as mentioned above and fit a linear model on log-normal transcript counts (Y) for each gene i as follows:

$${Y}_{i}\sim {n}_{{\rm{f}}{\rm{e}}{\rm{a}}{\rm{t}}{\rm{u}}{\rm{r}}{\rm{e}}{\rm{s}}}+{\rm{s}}{\rm{a}}{\rm{m}}{\rm{p}}{\rm{l}}{\rm{e}}+{\sum }_{j}{X}_{j}.$$

To determine KO effects in neural NPCs, we also used cell cycle phase as a covariate. For this, we inferred the cell cycle phase with the Seurat function CellCycleScoring() and then constructed the linear model as follows:

$${Y}_{i}\propto {n}_{{\rm{f}}{\rm{e}}{\rm{a}}{\rm{t}}{\rm{u}}{\rm{r}}{\rm{e}}{\rm{s}}}+{\rm{s}}{\rm{a}}{\rm{m}}{\rm{p}}{\rm{l}}{\rm{e}}+{\rm{c}}{\rm{c}}\,{\rm{p}}{\rm{h}}{\rm{a}}{\rm{s}}{\rm{e}}+{\sum }_{j}{X}_{j}.$$

To determine the KO effects across all neurons, we inferred global perturbation probabilities on the full dataset and then fit a linear model across neuronal populations on log-normal transcript counts for each gene y as follows:

$${Y}_{i}\propto {n}_{{\rm{f}}{\rm{e}}{\rm{a}}{\rm{t}}{\rm{u}}{\rm{r}}{\rm{e}}{\rm{s}}}+{\rm{s}}{\rm{a}}{\rm{m}}{\rm{p}}{\rm{l}}{\rm{e}}+{\rm{n}}{\rm{e}}{\rm{u}}{\rm{r}}{\rm{o}}{\rm{n}}\,{\rm{t}}{\rm{y}}{\rm{p}}{\rm{e}}+{\sum }_{j}{X}_{j}.$$

The coefficients for each target gene were tested using ANOVA and multiple-testing correction was performed using the Benjamini–Hochberg method to obtain an FDR-adjusted P value. Genes for which the coefficient of a target gene were significant (FDR < 10−4) were treated as differentially expressed genes for this target gene.

Determination of composition changes in the CROP-seq screen

To assess the degree to which the KO of a target gene changes the regional composition of the organoid, we first tested the enrichment of each gRNA in each regional branch. To control for confounding effects through differential gRNA abundance in different organoids, we used a Cochran–Mantel–Haenzel (CMH) test stratified by organoid. Moreover, we performed a Fisher’s exact tests to test for enrichment for each organoid individually. Multiple-testing correction was performed using the Benjamini–Hochberg method. To account for other potential within-sample confounders such as clonal heritage, we first required for each gRNA that the enrichment was significant (FDR < 0.05) in more than one individual organoid and that the direction of each significant enrichment was consistent across organoids. All gRNAs for which this was not the case were removed. In a second step, we further required for remaining gRNAs that the same significant effect (FDR < 0.01) was observed for at least one other gRNA targeting the same gene. For the remaining gRNAs, we summarized the assignments for each target gene i and calculated the log odds ratio of the enrichment in each regional branch j with

$${{\rm{LOR}}}_{ij}=\log \frac{{N}_{g=i{\rm{;}}b=j}/{N}_{g=i{\rm{;}}b\ne j}}{{N}_{g\ne i{\rm{;}}g=j}/{N}_{g\ne i{\rm{;}}b\ne j}}$$

where N is a matrix of cell counts for each target gene in each branch. For each target gene, the maximum log odds ratio across the three branches was treated as a measure of composition change.

Preprocessing and integration of single-cell RNA-seq data from the GLI3-KO experiment

Transcript count matrices were obtained using Cell Ranger (v.3.0.2) and further preprocessed using the Seurat R package (v.3.2)19. First, cells were filtered on the basis of UMI counts (>200, <60,000), the number of detected genes (>200, <6,000) and the fraction of mitochondrial genes (<0.1). Transcript counts were normalized to the total number of counts for that cell, multiplied by a scaling factor of 10,000 and subsequently natural-log transformed (NormalizeData()). From all protein coding, non-mitochondrial and non-ribosomal genes, we selected the 200 most variable based on the vst method (FindVariableFeatures()). PCA was performed based on the z-scaled expression of these features. Different samples were integrated using CSS21 based on the top 20 PCs with the default parameters. To visualize the dataset in two dimensions, we used UMAP on the CSS coordinates with spread = 0.5, min.dist = 0.2.

CRISPResso analysis and protein sequence prediction

To find clones with a frame-shift mutation, CRISPResso was used to analyse the sequencing data75. This tool aligned the amplicons to the wild-type gene sequence to call in-frame and frameshift indels. Analyses were performed using the following parameters: -w20, -min_indentiy_score70 and -ignore_substitutions. Substitutions were ignored, only sequences with a minimum of 70% similarity were used and only indels present in a window of 20 bp from each of the gRNAs were called. Cell lines were considered to be KOs when >98% of the reads were considered to be a non-homologous end-joining event, the indels caused a frameshift, not more than two different indels were seen and were present in a 50:50 distribution. The predicted protein sequence was obtained using the Biopython Python package76.

Preprocessing and integration of multiome data from the GLI3-KO experiment

Initial transcript count and peak accessibility matrices were obtained using Cell Ranger Arc (v.1.0.0) and further preprocessed using the Seurat (v.3.2)19 and Signac (v.1.1)64 R packages. Peaks were called from the fragment file using MACS2 (v.2.2.6) and combined in a common peak set before merging. Cells were filtered based on transcript (UMI) counts (>1,000, <25,000), mitochondrial transcript percentage (<30%), peak fragment counts (>5,000, <700,000) and TSS enrichment score (>1). Transcript counts were normalized to the total number of counts for that cell, multiplied by a scaling factor of 10,000 and subsequently natural-log transformed (NormalizeData()). PCA was performed using the Seurat function RunPCA(). Different samples were integrated based on the top 20 PCs with Harmony77 using the function RunHarmony() from the R package SeuratWrappers (v.0.3.0) ( with max.iter.harmony = 50 and otherwise the default parameters.

Annotation of cells from the GLI3-KO and SHH experiment

To annotate the cell states from both the scRNA and the multiome experiments, we used the annotations of the annotated multi-omic atlas of organoid development that was previously generated. We transferred the regional branch labels using the method implemented in Seurat using the functions FindTransferAnchors() and TransferData(). We then performed Louvain clustering with a resolution 1 for the scRNA data and 0.8 for the multiome data. Clusters were manually assigned to branch identities based on the transferred labels as well as marker gene expression. In the case of the multiome data, we identified populations of mesenchymal and non-neural ectoderm cells, which were excluded from the downstream analysis.

Differential expression analysis for the GLI3-KO and SHH experiment

To assess the transcriptomic effects of the GLI3 KO in ventral telencephalon neurons, we performed differential expression analysis using a linear-model-based approach analogous to the approach used in the CROP-seq screen. We fit a linear model on log-normal transcript counts Y for each gene i with the KO label and number of detected features as independent variables:

$${Y}_{i}\propto {n}_{{\rm{f}}{\rm{e}}{\rm{a}}{\rm{t}}{\rm{u}}{\rm{r}}{\rm{e}}{\rm{s}}}+{\rm{K}}{\rm{O}}\,{\rm{l}}{\rm{a}}{\rm{b}}{\rm{e}}{\rm{l}}.$$

The coefficient of the KO label was tested using ANOVA. To perform differential expression of KO versus control in the multiome data and treated versus control for the SHH experiment, we performed a Wilcoxon rank-sum test using the presto R package (v.1.0.0)74. Multiple-testing correction was applied to all results using the Benjamini–Hochberg method to obtain FDR-adjusted P values.

Differential accessibility analysis for the GLI3-KO experiment

To find peaks with differential accessibility between GLI3 KO and control, we fit a generalized linear model with binomial noise and logit link for each peak i on binarized peak counts Y with the total number of fragments per cell and the KO label as the independent variables:

$${Y}_{i}\propto {n}_{{\rm{f}}{\rm{r}}{\rm{a}}{\rm{g}}{\rm{m}}{\rm{e}}{\rm{n}}{\rm{t}}{\rm{s}}}+{\rm{K}}{\rm{O}}\,{\rm{l}}{\rm{a}}{\rm{b}}{\rm{e}}{\rm{l}}.$$

We also fit a null model, where the KO label was omitted:

$${Y}_{i}\propto {n}_{{\rm{f}}{\rm{r}}{\rm{a}}{\rm{g}}{\rm{m}}{\rm{e}}{\rm{n}}{\rm{t}}{\rm{s}}}.$$

We then used a likelihood ratio test to compare the goodness of fit of the two models using the lmtest R package (v.0.9) ( Multiple-testing correction was performed using the Benjamini–Hochberg method.

Comparison of perturbation effects with GRN

Before using the GRN to interpret the DE results, we first sought to assess the degree to which the transcriptomic effects of the GLI3 KO are consistent with the inferred GRN. We tested the enrichment of DE genes in the first (direct) and second order (indirect) neighbourhood of GLI3 in the GRN graph using a Fisher’s exact test. Furthermore, we computed the shortest path from GLI3 to every DE gene in the GRN graph. To test how accurately the GRN can be used to predict the directionality of the DE, we computed the combined direction of each path as the product of the signs of all individual edges. We then determined the overall predicted effect of GLI3 on each DE gene by computing the mode of the directions of all shortest paths leading to that gene. We defined accuracy as the fraction of genes for which the DE direction was the inverse of the predicted overall effect. Next, we further filtered the paths so that all paths were composed only of DE genes and the direction of each path and subpath was consistent with the DE direction. To visualize this subgraph, we further pruned the graph by retaining only the path with the lowest average log10-transformed P value for each DE gene.

Functional annotation of differentially accessible genomic regions

To better functionally assess the epigenomic effects of the GLI3 KO, we performed functional enrichment analysis using GREAT31. We performed differential accessibility analysis in clusters 0 and 2 (early telencephalon) and applied an FDR threshold of 10−4. From all differentially expressed peaks, we selected the top 5,000 peaks with the lowest (most negative) linear model coefficient (depleted in the KO). We further selected all peaks that were accessible in at least 1% of cells in these clusters as the set of background peaks. Using these two peak sets, we used GREAT with the GRCh38 genome assembly and otherwise the default parameters to obtain functional enrichment results. We reported GO biological process enrichments with FDR < 0.01 and that were supported by >100 foreground regions.

Analysis of GLI3 CUT&Tag data

To assess GLI3 binding with CUT&Tag data, we first obtained bigwig files with intensity scores across genomic coordinates. From these scores, we computed a per-gene binding score by summing the intensities over the gene body plus an extended promoter region of 2 kb.

Statistics and reproducibility

Representative images of organoids in culture are shown from batches with 16–96 organoids per cell line (Extended Data Figs. 1a, 6d and 9c). Immunohistochemistry analysis of SOX2, TUJ1 and GLI3 (Extended Data Fig. 1k) was performed on four different cell lines on 2–3 organoids per cell line from one batch. HCR RNA-FISH (Extended Data Fig. 2g) for BMP7 and WLS was performed on day 18 organoids from four different cell lines with 2–3 organoids per experiment and HCR RNA-FISH for FGF8 and WNT8B was performed on day 18 organoids cell line Wibj2 for 3 organoids.

Reporting summary

Further information on research design is available in the Nature Research Reporting Summary linked to this article.

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