- Methodology article
- Open Access
Massively parallel nanowell-based single-cell gene expression profiling
- Leonard D. Goldstein†1,
- Ying-Jiun Jasmine Chen†1,
- Jude Dunne2,
- Alain Mir2,
- Hermann Hubschle3,
- Joseph Guillory1,
- Wenlin Yuan1,
- Jingli Zhang1,
- Jeremy Stinson1,
- Bijay Jaiswal1,
- Kanika Bajaj Pahuja1,
- Ishminder Mann2,
- Thomas Schaal2,
- Leo Chan2,
- Sangeetha Anandakrishnan2,
- Chun-wah Lin2,
- Patricio Espinoza2,
- Syed Husain2,
- Harris Shapiro2,
- Karthikeyan Swaminathan2,
- Sherry Wei2,
- Maithreyan Srinivasan2Email author,
- Somasekar Seshagiri1Email author and
- Zora Modrusan1Email author
© The Author(s). 2017
- Received: 2 January 2017
- Accepted: 21 June 2017
- Published: 7 July 2017
Technological advances have enabled transcriptome characterization of cell types at the single-cell level providing new biological insights. New methods that enable simple yet high-throughput single-cell expression profiling are highly desirable.
Here we report a novel nanowell-based single-cell RNA sequencing system, ICELL8, which enables processing of thousands of cells per sample. The system employs a 5,184-nanowell-containing microchip to capture ~1,300 single cells and process them. Each nanowell contains preprinted oligonucleotides encoding poly-d(T), a unique well barcode, and a unique molecular identifier. The ICELL8 system uses imaging software to identify nanowells containing viable single cells and only wells with single cells are processed into sequencing libraries. Here, we report the performance and utility of ICELL8 using samples of increasing complexity from cultured cells to mouse solid tissue samples. Our assessment of the system to discriminate between mixed human and mouse cells showed that ICELL8 has a low cell multiplet rate (< 3%) and low cross-cell contamination. We characterized single-cell transcriptomes of more than a thousand cultured human and mouse cells as well as 468 mouse pancreatic islets cells. We were able to identify distinct cell types in pancreatic islets, including alpha, beta, delta and gamma cells.
Overall, ICELL8 provides efficient and cost-effective single-cell expression profiling of thousands of cells, allowing researchers to decipher single-cell transcriptomes within complex biological samples.
- Single cell profiling
- RNA sequencing
- Single-cell transcriptome
Single-cell RNA sequencing (RNA-seq) has rapidly evolved over the last few years, providing new understanding of cell composition and identity in normal and diseased settings [1, 2]. Transcriptional profiling at the single-cell level facilitates identification of new cell types and understanding of cellular heterogeneity, aids in lineage tracing, and elucidates hierarchical relationships among cell types in the course of development or disease progression [2–7]. For example, based on their transcriptome patterns, more than 40 subtypes of neurons were identified in the mouse cortex [7, 8]. Single-cell RNA-seq also identified a rare cell type in colon tissue .
Initial transcriptional profiling at the single-cell level was done using fluorescence-activated cell sorting (FACS). However, FACS-based techniques have limited throughput and are not cost-effective. Recently, methods that enable single-cell transcriptome and whole-genome sequencing without the need for FACS have been reported. Notably, microfluidic-based single-cell isolation (e.g. Fluidigm C1) and transcriptome analysis was performed successfully, though the throughput and the ability to capture a large range of cell sizes is limiting . The C1-based method does not employ molecular barcodes for eliminating PCR duplicates during cDNA conversion and can potentially lead to data bias [6, 9]. Recently, encapsulation of thousands of cells using droplet-based microfluidic methods for single-cell RNA-seq have been demonstrated [10, 11]. While droplet-based technology is encouraging, further development of the experimental technique and analysis tools are needed for its wider adoption [9, 12, 13].
Microchip for single-cell isolation
The ICELL8 microchip is made of aluminum alloy (41 mm2) and contains 5184 nanowells arranged in a square layout (72 × 72 wells). Each nanowell holds 150 nl and contains preprinted oligonucleotides; each oligonucleotide includes an oligo-(dT30) primer, a well-specific sequence (11 bp) used for cell barcoding and a unique molecular identifier (UMI, 10 bp; Fig. 1). The cell barcode is used to identify cDNA molecules generated from an individual cell, while UMIs identify individual mRNA molecules . A similar microchip-based technology has been used previously in targeted sequencing applications [16, 17].
Cell suspensions were fluorescently labeled with live/dead stain (Hoechst 33324/Propidium Iodide, see Methods) prior to their dispensing into the microchip nanowells using the MSND (Additional file 1: Figure S1). The MSND is an 8-channel microsolenoid controlled dispenser that delivers ≥30 nl volumes using non-contact dispensing. The MSND dispenses up to eight different samples (one sample per channel) into a single microchip in approximately 12 minutes. To minimize evaporation, the microchip is enclosed in a controlled humidity and temperature chamber. Cross contamination between nanowells due to dispense tip misalignment was assessed using a checkerboard assay (see Methods, Additional file 2: Figure S2). In a test involving 11 MSND instruments we observed the average percentage of wells affected by misalignment to be 0.08%. Cells are dispensed by a limiting dilution; assuming a Poisson distribution for the number of cells per well, about one third of the 5184 nanowells contain a single cell under optimal conditions.
Following cell dispensing, the microchip was centrifuged to collect cells in a single plane and then imaged using a standard microscope with an automatic stage, a 4× objective and a charge-coupled device (CCD) camera. After imaging, the microchip was sealed and stored at −80 °C until ready for use (Additional file 1: Figure S1). Next we used imaging software (CellSelect, see Materials and Methods) to automatically and/or manually identify wells that contain single cells (Fig. 1b). A file containing positional information on identified candidate wells (dispense file) was then used to selectively deliver reverse transcriptase (RT) master mix to designated wells.
Single-cell barcoding and sequencing
Cells in the microchip were lysed by freeze-thaw (see Methods). Under the directions from the dispense file, the MSND dispensed RT master mix into selected wells and cDNA synthesis was performed in those wells using the Single Cell Barcoding and Sequencing method (SCRB-seq) . cDNAs from hundreds of cells were then pooled into a single tube, purified and amplified by standard practices. The amplified cDNAs were subjected to transposon-mediated fragmentation (“tagmentation”), PCR amplified and converted to an Illumina-compatible NGS library (Additional file 1: Figure S1). RNA-seq libraries were sequenced using paired-end sequencing where read 1 (25 bp) contained the well barcode and UMI and read 2 (50 bp) captured the cDNA sequence (Fig. 1c).
Sequencing data processing and quality control
Gene detection and reproducibility of single-cell expression profiles
To assess the sensitivity of the platform and allow comparison with other single-cell systems, we down-sampled reads for each cell and determined the median number of detected genes and transcripts with increasing sequencing depth (Fig. 2c and d). At an average sequencing depth of 100 K reads per cell we detected a median of ~2500 genes in Ba/F3 cells. The number of detected genes increased to >4000 at higher sequencing depths (Fig. 2c).
To assess the reproducibility between cells when profiling a relatively homogeneous sample type, we compared per-gene transcript counts between pairs of Ba/F3 cells. Pairwise comparisons generally showed high correlation with median r = 0.83 (Pearson correlation coefficient) and interquartile range of 0.81–0.84; an example is shown in Additional file 6: Figure S6a (r = 0.77). When performing the same analysis using per-gene read counts, we observed lower correlation (r = 0.69; Additional file 6: Figure S6b), illustrating the advantage of UMIs in reducing PCR amplification bias. Next we asked whether single-cell gene expression data accurately reflected expression profiles obtained from bulk cells. We processed total RNA from bulk Ba/F3 cells on the same microchip as Ba/F3 single cells and found that the bulk expression profile was highly correlated with the ensemble (average) of single-cell profiles (r = 0.95; Additional file 6: Figure S6c).
Assessment of cell multiplet rate and single-cell impurity
Single-cell expression profiles of cultured cell lines
Identification of cell subtypes from pancreatic islets
Finally we determined whether the platform can distinguish cell types within a solid tissue sample. For this purpose we profiled 468 cells from adult mouse pancreatic islets. Pancreatic islets consist of the endocrine cells of the pancreas, with insulin-producing beta cells forming the majority. The other three major cell types include glucagon (Gcg)-producing alpha cells, somatostatin (Sst)-producing delta cells and pancreatic polypeptide (Ppy)-producing gamma cells (also known as PP cells). Hierarchical clustering based on known marker genes revealed the four distinct cell populations (Fig. 4c) and the relative abundance of cell types tracked the known composition of adult mouse pancreatic islets, including 38% beta cells (n = 179), 26% alpha cells (n = 124), 22% delta cells (n = 101), and 14% PP cells (n = 64). Unsupervised principal component analysis based on the 500 most variable genes did not show clear clusters of four major islet cell subtypes; however beta and alpha cells were largely separated (Additional file 8: Figure S8).
Transcriptome profiling of individual cells by single-cell RNA-seq is a powerful approach for deciphering the cell composition of complex tissues; however, broader use of this method has been limited by its ease of use, scalability, cost and turn-around time. Here we report a novel system for high-throughput single-cell RNA-seq, ICELL8, which uses nanowell-based cell capture and relies on cell- and transcript-specific barcoding to obtain transcript counts for individual cells. Although the ICELL8 system uses similar chemistry for single-cell RNA-seq library generation as other platforms, it features unique components, including i) an MSND instrument for dispensing single-cell suspensions into nanowells, ii) software for automated identification of hundreds to over a thousand of single-cell-containing wells, and iii) UMI-based transcript counting. The ease of dispensing cells of any size or shape into nanowells with the MSND eliminates errors associated with manual pipetting of viscous reagents into microfluidic devices. Cells as large as cardiomyocytes (~100 μm) and spheroids have been dispensed, imaged and processed for single-cell RNA-seq using the system (data not shown). The system also provides flexibility, allowing for processing of up to eight samples on the same microchip. Taken together, the ICELL8 system enables processing of several chips per day, which translates to processing tens of thousands of individual cells. Ease of use and fast turn-around time are key features of the system, which allow experiments with a variety of biological samples. Overall, it takes ~3 days on ICELL8 to process one sample from cell dispensing to library QC (see Additional file 1: Figure S1), compared to ~2 days on the 10× Genomics system. The consumable cost including chips, cell-handling reagents, enzymes and primers is in a range similar to many current commercial technologies.
Here we assessed the performance of the ICELL8 system by profiling a mixture of human and mouse cell lines to determine single-cell purity (94–97%) and cell multiplet rate (<3%). Performance characteristics were comparable to other single-cell RNA-seq platforms (e.g. multiplet rate in 10× Genomics: ~1% at 1000 cell density and ~6% at 6000 cell density ). In this study we profiled panels of human and mouse cell lines, as well as mouse pancreatic islets. Unsupervised principal component analysis did not show clear clusters of the four major islet cell subtypes . Future versions of the ICELL8 system may benefit from improvements in sample processing including minimizing ambient RNA.
The ICELL8 system adds to the growing number of technologies that have been developed to understand biology at the single-cell level and complements existing microfluidic and droplet-based technologies. Besides enabling applications such as single-cell RNA-seq, it can empower other high-throughput sequencing applications that require imaging and selection to process only cells of interest. The current configuration uses nanowells with volumes of 150 nl. These wells can be configured to larger dimensions for volumes as high as 1 μl. Thus the ICELL8 system is capable of accommodating applications that require several reagent additions such as whole-genome amplification, combined readouts of DNA and RNA, or RNA and protein. Future technology improvements, including miniaturization that could result in a chip with >100 K nanowells, would enable enormously parallel processing of single cells. In addition, we have developed technologies where single cells can be targeted to occupy each well, thereby generating occupancy rates of >80% (http://www.freepatentsonline.com/20160045884.pdf). Furthermore, imaging enables the selection of wells not only based on Hoechst/Propidium Iodide staining but also based on fluorescent antibody staining. Thus, cells sorted by FACS can be orthogonally validated and selected and processed for single-cell RNA-seq and other applications.
We demonstrated the performance and utility of a novel nanowell-based single-cell RNA sequencing system, ICELL8, which enables expression profiling of thousands of cells. Based on single-cell expression profiling data generated by ICELL8, we were able to identify representative cell types in mouse pancreatic islets and discriminate between mixed human and mouse cells. The technological advancements of ICELL8 enable more time- and cost-efficient transcriptome characterization of single cells, providing researchers with deeper insight into complex biological samples.
Human (K562, A375, HCT116, NCI-H2452, Miapaca2 and KU812) and mouse (3T3, Ba/F3, Beta-TC6, 307 and 307-lung) cell lines were used for evaluating the ICELL8 single-cell RNA-seq system. The melanoma cell line A375 was cultured in DMEM media with 10% fetal bovine serum (FBS, Thermo Fisher); the colon cancer cell line HCT116, mesothelioma cell line NCI-H2452, pancreatic adenocarcinoma cell line Miapaca2, chronic myelogenous leukemia (CML) cell line KU812 and K562 were cultured in RPMI 1640 media supplemented with 10% FBS. The mouse pancreatic beta cell line Beta-TC6 was cultured in DMEM media supplemented with 15% FBS; the mouse fibroblast 3 T3 cell line was cultured in DMEM supplemented with 10% FBS and 1 mM sodium pyruvate; the mouse pro-B cell line Ba/F3 was maintained in RPMI 1640 supplemented with 10% FBS and 2 ng/ml mouse IL-3 (R&D Systems). 307 and 307-lung cells were derived from a conditional Pik3ca knock-in mouse model  and were cultured in Epicult B basal medium (STEMCELL Technologies). All cell media contain 2 mM L-glutamine (except for 307 and 307-lung), 100 U/ml penicillin, and 100 mg/ml streptomycin. Cells were prepared as single-cell suspensions either by trypsinization and gentle washing, for adhesive cells, or direct washing, for suspension cells. Adult mouse pancreas was first perfused with the Liberase solution through the common bile duct, and then dissected and incubated at 37 °C for 10 min. Islets were separated from acinar tissue using histopaque density centrifugation (Sigma). Liberase solution was made by dissolving 5 mg Liberase TL (Roche) in 20 ml 1xHBSS buffer containing 25 mM HEPES (pH 7.2), 1.8 mM CaCl2, 10 μg/ml DNase and 0.1% BSA. Purified islets were dissociated into single cell suspension using Accumax cell dissociation solution (Innovative Cell Technologies) for up to 30 min at room temperature.
Cell isolation by limiting dilution
Cells were stained with Hoechst 33324 and Propidium Iodide (Thermo Fisher) for 20 min. The cell viability and density was checked with ViCell XR (Beckman Coulter) using Trypan Blue. Cells were diluted to achieve a density of 1-2 cells per 50 nl in a final dispensing mix which contained a diluent, RNAsin (New England Biolab) and 0.35X PBS (without Ca++ and Mg++, pH 7.4, Thermo Fisher). A 384-well source plate with 8 designated wells containing cell suspensions, 1 well for positive control, 1 well for negative control, and 1 well for fiducial mix (fluorescent dye permitting image alignment confirmation) was placed in the MSND (WaferGen). Each of the 8 sample source wells in the 384-source plate was sampled by 1 of the 8 channels in MSND. Cells, positive controls, negative controls, and fiducial mix, were dispensed onto one chip within 16 min. Each well received 50 nl of either cell mix, positive control, negative control, or fiducial mix. Total RNA (~10 pg) from K562 cells was dispensed into selected nanowells and used as in-process positive controls. For Ba/F3 data, total RNA (~10 pg) from Ba/F3 cells was dispensed into selected nanowells and used as bulk in analyses.
MSND quality testing
For each tested MSND, cross contamination between nanowells was measured using a checkerboard assay performed on a single microchip (Additional file 2: Figure S2). First negative control master mix (no template DNA) was dispensed into wells located on one half of the microchip (NTC wells, n = 2520). The percentage of wells that showed signal was considered background unrelated to misalignment of the dispensing tips. In the second half of the chip, lambda DNA master mix (Positive wells, n = 1024) and negative control master mix (Test wells, n = 1496) were dispensed in an alternate checkerboard pattern. The dispensed chip was sealed with a film, centrifuged and a real-time PCR analysis was performed. If the dispenser tip is misaligned, lambda DNA master mix is inadvertently added to test wells, resulting in Ct values indicative of cross contamination. Ct values were used to determine the number of Test wells and NTC wells that showed signal. To ensure that only intended PCR products were quantified, a melt-curve analysis was performed. Test wells and NTC wells with melting temperature 3 standard deviations outside of the mean melting temperature for Positive wells were excluded. Percentage of misalignment was calculated as the difference between the percentage of Test wells with signal minus the percentage of NTC wells with signal (i.e. % misalignment = % Test wells that show signal - % NTC wells that show signal).
Microchip imaging and selection of single-cell-containing nanowells
After dispensing, each chip was sealed and centrifuged at 300 g for 5 min at 4 °C before imaging with a Leica microscope (Leica). A total of 288 images, 144 each for Hoechst 33,342 and for Propidium Iodide were captured. Each image comprised the picture of 36 wells. Following imaging (~7 min), the microchip was stored at −80 °C for at least 45 min or until ready for further processing.
Microchip images were analyzed using CellSelect software (WaferGen) to determine the viability and number of cells present in each nanowell. Briefly, to identify cells in an image, a Laplacian of Gaussian (LoG) image was calculated with a user-selectable scale. The LoG image was then segmented using auto-provided or user-defined thresholds. The resulting shapes were then classified by user-defined size and shape. Objects that do not meet the criteria were rejected. These steps eliminate many artifacts that may appear in the microscope images. This segmentation and classification process was performed for images obtained using both Hoechst 33324 (channel 1) and Propidium Iodide (PI, channel 2) images. In the default configuration, cells visible in channel 2 indicate PI positive (dead cells) which are auto-excluded from further processing. Using the default configuration, CellSelect identified all nanowells that have one cell in channel 1 (Hoechst) and no cells in channel 2 (PI). Nanowells that had one bright cell and additional dim cells or debris were further excluded. In summary, nanowells that contained only one cell were selected as candidates and additional visual inspection was performed to confirm the presence of single viable cells. After selecting the highest confidence candidate cells, the software auto-generated multiple files used to streamline the downstream processing (e.g. sample-barcode file, filter file for dispensing reverse transcription mix, cell dispense and Poisson summary statistics).
Single-cell cDNA generation
Microchips were removed from −80 °C and left at room temperature for 10 min. Cells were lysed by freeze-thaw at this step. Chips were then centrifuged at 3800 g for 5 min at 4 °C and transferred to a thermocycler with a program of 72 °C for 3 min and 4 °C hold to anneal preprinted oligonucleotides to polyA mRNAs. The microchips were centrifuged as previously and were placed back into the MSND. A separate 384-well source plate containing reverse transcription (RT) reagents (1 mM dNTP, 1 μM E5 Oligos, Maxima H Minus RT buffer and 12 U/μl of Maxima H Minus reverse transcriptase) in 4 wells was used in the MSND, which delivered 50 nl of reverse transcription mix to selected nanowells. The microchips were spun down and transferred to a thermocycler with a program of 42 °C for 90 min and 4 °C hold to perform RT. Post reaction chips were inverted and centrifuged (3800 g 10 min at 4 °C) to simultaneously collect and pool well contents into a single microcentrifuge collection tube. Double-stranded cDNA was cleaned by the DNA Clean & Concentrator™-5 kit (Zymo Research). Eluate was treated with Exonuclease I (37 °C for 30 min, 80 °C for 20 min). A PCR program of 95 °C for 1 min, 18 cycles of 95 °C for 15 s, 65 °C for 30 s, 68 °C for 6 min, and 1 cycle of 72 °C for 10 min and 4 °C hold was performed using Advantage 2 polymerase. Amplicons were purified using Agencourt AMPure XP magnetic beads (Beckman Coulter). cDNA quality was assessed using a Bioanalyzer High Sensitivity DNA chip (Agilent Technologies) and quantity was determined by a Qubit High Sensitivity kit (Thermo Fisher Scientific).
RNA-seq library construction and sequencing
One ng of cDNA was used for library construction using the Nextera XT kit (Illumina) according to manufacturer’s instruction. A custom-made Nextera P5 (WaferGen) and a P7 index primer provided by the Nextera XT kit (Illumina) were used to amplify the “tagmented” fragments. Libraries were purified and size selected using Agencourt AMPure XP magnetic beads (Beckman Coulter) to obtain an average library size of 500 bp. A typical yield for a library comprised of ~1500 cells was ~15 nM. Libraries were sequenced on either a HiSeq2500 or HiSeq4000 (Illumina) to obtain on average ~ 1-2 million 25 × 50 bp reads per cell.
RNA-seq data processing
Read pairs were de-multiplexed requiring a perfect match between the first 11 bases of read 1 and one of the expected barcodes. The second read was then mapped to the reference genome using GSNAP  retaining the UMI sequence for each aligned read. Only uniquely mapping reads were considered. After mapping, the number of captured transcripts per gene was inferred based on UMIs. Read pairs with UMIs containing Ns were excluded. To avoid inflation of transcript counts due to errors in UMI sequences, we clustered UMIs with similar sequences for each gene (allowing for 1 mismatch). To remove low-abundance UMIs that may be the result of chimeric PCR products (Additional file 9: Figure S9), we only considered UMI clusters represented by at least two reads. Per-gene transcript counts were based on the number of distinct UMI clusters. For downstream analyses, per-gene transcript counts were normalized by dividing the counts for each cell by a cell-specific scale factor, calculated as the total transcript count for a given cell, divided by the median total transcript count across cells. No additional normalization was performed between microchips.
Read depth simulation
We assessed the effect of sequencing depth on the number of detected genes and transcripts using Ba/F3 data. Ba/F3 cells were sequenced at an average read depth D of ~1 M reads per cell. To simulate an average read depth d < D, for each cell we sampled a fraction d/D from the subset of reads aligning to annotated genes, and recalculated the number of detected genes and transcripts as described above.
Sequence reads were mapped independently to the human and mouse genomes. Reads that mapped to both genomes with ≤3 mismatches were excluded. In Fig. 3 the total number of detected mouse transcripts was plotted against the total number of detected human transcripts for each cell. Cells that had more than 2925 human transcripts were classified as human (n = 247). Cells that had more than 1955 mouse transcripts were classified as mouse (n = 243). Cells that were classified as both human and mouse were considered cross-species multiplets (n = 6). Cells that were not classified as either species were excluded from the analysis (n = 3). The cutoff for human (mouse) cells was determined by considering cells with more transcripts mapping to mouse (human) and computing the median plus five times the inter-quartile range of the number of human (mouse) transcripts. Single-cell purity estimates for human (mouse) cells were obtained by considering cells classified as human (mouse), dividing the number of transcripts detected in human (mouse) by the sum of transcripts detected in either species, and taking the median across cells.
Most variable genes were determined based on the variance of normalized transcript counts after log2(x + 1) transformation. PCA and hierarchical clustering was performed based on normalized transcript counts after log2(x + 1) transformation and mean-centering genes. Hierarchical clustering was performed with 1 - Pearson correlation as distance metric and average linkage using the R package NMF.
We thank Connie Ha and Sherry Heldens for help with experimental set-up, Bernard Chow for sequencing data processing, Oleg Mayba for statistical advice, and members of the FACS lab for technical assistance. We also thank Allison Bruce for art illustrations.
This study was funded by Genentech, Inc.
Availability of data and materials
RNA-seq data will be deposited at the European Genome-phenome Archive under accession code EGAS00001002320.
Conceptualization: SS, MS and ZM; Experimental investigation: YJC, WY, IM, LC, SA; Material generation: JZ, BJ, KBP; Sequencing data generation: JG, JS; Data analysis: LDG, HS, KS and SW; Software development: HH; Hardware development: SH, PE, TS and CWL; System integration: JD and AM; Writing: LDG, YJC, SS, SM and ZM. All authors read and approved the final manuscript.
Ethics approval and consent to participate
All protocols involving animals were approved by Genentech’s Institutional Animal Care and Use Committee, in accordance with guidelines that adhere to and exceed state and national ethical regulations for animal care and use in research.
Consent for publication
L.D.G., Y.J.C., J.G., W.Y., J.Z., J.S., B.J., K.B.P., S.S. and Z.M. are employees of Genentech. L.D.G., Y.J.C., J.G., W.Y., J.S., B.J. K.B.P., S.S. and Z.M hold shares in Roche. H.H. is a consultant for WaferGen. J.D., A.M., I.M., T.S., L.C., S.A., C.W.L., P.E., S.H., H.S., K.S., S.W. and M.S. are employees of WaferGen and hold shares in WaferGen.
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