robustSingleCell
Overview
robustSingleCell is a pipeline designed to identify robust cell subpopulations using scRNAseq data and compare population compositions across tissues and experimental models via similarity analysis as described in Magen et al. (2019) bioRxiv [1].
Installation
Install the following dependencies before installing the package:
if(!require(devtools))
install.packages("devtools")
if (!requireNamespace("BiocManager", quietly = TRUE))
install.packages("BiocManager")
BiocManager::install("limma")
BiocManager::install("grimbough/biomaRt")You can then install the stable version from CRAN:
install.packages("robustSingleCell")To access the latest features or bug fixes, you can install the development version from GitHub.
devtools::install_github("asmagen/robustsinglecell")This pipeline currently supports slurm for parallel batch jobs.
Getting help
If you identify a bug, please submit an issue with a reproducible example.
Tutorial
We used two replicates of CD44+ T cell data sets from Ciucci
et al. 2019 [2] as an example to demonstrate the use of
robustSingleCell. The analysis requires at least 8G of memory on
slurm [3] high performance computing workload manager (for example,
you can start by requesting srun --pty -p <partition> --mem=8G -t 1:00:00 bash to start an interactive session).
We first download the raw 10X data from GEO using GEOquery, which can
be obtained using the following command if not already installed:
source("https://bioconductor.org/biocLite.R")
biocLite("GEOquery")The two datasets LCMV1, LCMV2 will be downloaded into TMPDIR. Each
folder will contain the matrix.mtx, gene.tsv and barcode.tsv files
as in 10X genomics format.
library(robustSingleCell)
download_LCMV()Note: when using your own data, the 10X genomics files
(matrix.mtx, gene.tsv and barcode.tsv) will be typically located
at outs/filtered_gene_bc_matrices/mm10, depending on the genome
used for alignment. Copy the contents of this directory to the working
directory data.path specified in initialize.project below.
We cluster each dataset separately to account for dataset-specific technical and biological differences. Then, we measure the transcriptional similarity and divergence between the clusters identified in the two datasets using correlation analysis.
Individual analysis of LCMV1 and LCMV2
First, we set up the directory where the results of the analysis will be stored.
LCMV1 <- initialize.project(datasets = "LCMV1",
origins = "CD44+ cells",
experiments = "Rep1",
data.path = file.path(tempdir(), "LCMV"),
work.path = file.path(tempdir(), "LCMV/LCMV_analysis"))read.data function reads the data in 10X genomics format and performs
quality filtering as described in Magen et al 2019. We randomly
downsampled the datasets to 500 cells to shorten the simplify this
example.
LCMV1 <- read.data(LCMV1, subsample = 500)Next, we identify highly variable genes for the following PCA and clustering analyses. We also compute the activation of gene sets of interest, such as cell cycle genes, for confounder correction.
LCMV1 <- get.variable.genes(LCMV1)
exhaustion_markers <- c('Pdcd1', 'Cd244', 'Havcr2', 'Ctla4', 'Cd160', 'Lag3', 'Tigit', 'Cd96')
LCMV1 <- add.confounder.variables(LCMV1,
ribosomal.score = ribosomal.score(LCMV1),
mitochondrial.score = mitochondrial.score(LCMV1),
cell.cycle.score = cell.cycle.score(LCMV1),
Exhaustion = controlled.mean.score(LCMV1, exhaustion_markers))Figure 1 shows the mitochondrial score versus number of UMIs, pre and post filtering.
Fig 1. Mitochondrial genes score vs. number of UMIs for pre (top) and post (bottom) quality control filtering.
The PCA function performs multiple simulation analyses of shuffled
data to determine the appropriate number of PCs. You can also run each
simulation in parallel using the option local = F.
LCMV1 <- PCA(LCMV1, local = T)We then perform clustering analysis for a range of clustering
resolutions. The analysis is repeated multiple times over shuffled data
to estimate the appropriate clustering resolution and control for false
discovery of clusters. At the end of the clustering, the function will
prompt you to choose an optimal clustering resolution. We choose 0.05
for our KNN ratio, which is the smallest value tested with
mdlrty/mean.shfl > 2.
LCMV1 <- cluster.analysis(LCMV1, local = T)
Fig 2. Bar plot shows the clustering modularity of the original data versus shuffled data across multiple clustering resolutions. Numbers on top represent the fold change of original versus shuffled analysis for each resolution.
We select the appropriate resolution, typically the one where there is more than two (2) fold change modularity difference relative to the shuffled analysis.
The summarize function which performs differential expression
analysis, computes tSNE and visualizes the results in the analysis
folder. After differential expression analysis, get.cluster.names
assigns clusters with names using a customized set of marker genes which
users should adapt to their own data.
types = rbind(
data.frame(type='Tfh',gene=c('Tcf7','Cxcr5','Bcl6')),
data.frame(type='Th1',gene=c('Cxcr6','Ifng','Tbx21')),
data.frame(type='Tcmp',gene=c('Ccr7','Bcl2','Tcf7')),
data.frame(type='Treg',gene=c('Foxp3','Il2ra')),
data.frame(type='Tmem',gene=c('Il7r','Ccr7')),
data.frame(type='CD8',gene=c('Cd8a')),
data.frame(type='CD4', gene = c("Cd4")),
data.frame(type='Cycle',gene=c('Mki67','Top2a','Birc5'))
)
summarize(LCMV1, local = T)
LCMV1_cluster_names <- get.cluster.names(LCMV1, types, min.fold = 1.0, max.Qval = 0.01)
LCMV1 <- set.cluster.names(LCMV1, names = LCMV1_cluster_names)
summarize(LCMV1, local = T)Figure 3 shows violin plots indicating the activation of the cell cycle genes.
Fig 3. Violin plot pf cell cycle score.
Figure 4 places individual cells on a two dimensional grid corresponding
to the scores of the first two PCs (note that the PCA figures are
created in the next step via summarize function below).
Fig 4. Single cells placement on a 2D grid corresponding to the first two PCs.
The genes driving the PCs are visualized in figure 5 according to the PCA loadings after removing the lowly ranked genes.
Fig 5. Top ranked genes contribution to PC1 and PC2 scores.
The average expression of genes driving the PCs can be visualized as a heatmap visualized in figure 6 according to the PCA loadings after removing the lowly ranked genes.
Fig 6. Heatmap shows loadings of the first PC.
Figure 7 shows the tSNE visualization of the cells, color coded by cluster assignment.
Fig 7. t-SNE plot colored by cluster assignment.
We can also visualize the average expression of selected T cells marker genes for initial evaluation (Figure 8).
canonical_genes <- c("Cd8a", "Cd4", "Mki67", "Foxp3", "Il2ra", "Bcl6",
"Cxcr5", "Cxcr6", "Ifng", "Tbx21", "Id2", "Rora",
"Cxcr3", "Tcf7", "Ccr7", "Cxcr4", "Pdcd1", "Ctla4")
plot_simple_heatmap(LCMV1, name = "canonical", markers = canonical_genes, main = "Expression of marker genes")
Fig 8. Heatmap shows row-normalized average expression of selected marker genes per cluster.
We repeat the same procedure for LCMV2 dataset.
LCMV2 <- initialize.project(datasets = "LCMV2",
origins = "CD44+ cells",
experiments = "Rep2",
data.path = file.path(tempdir(), "LCMV"),
work.path = file.path(tempdir(), "LCMV/LCMV_analysis"))
LCMV2 <- read.data(LCMV2, subsample = 500)
LCMV2 <- get.variable.genes(LCMV2)
LCMV2 <- add.confounder.variables(
LCMV2,
ribosomal.score = ribosomal.score(LCMV2),
mitochondrial.score = mitochondrial.score(LCMV2),
cell.cycle.score = cell.cycle.score(LCMV2),
Exhaustion = controlled.mean.score(LCMV2, exhaustion_markers))
LCMV2 <- PCA(LCMV2, local = T)
LCMV2 <- cluster.analysis(LCMV2, local = T)
summarize(LCMV2, local = T)
LCMV2_cluster_names <- get.cluster.names(LCMV2, types, min.fold = 1.0, max.Qval = 0.01)
LCMV2 <- set.cluster.names(LCMV2, names = LCMV2_cluster_names)
summarize(LCMV2, local = T)
plot_simple_heatmap(LCMV2, name = "canonical", markers = canonical_genes, main = "Expression of marker genes")Dataset Integration by Correlation Analysis
We then initialize the aggregate analysis of the two independent runs, providing the information of which analyses folders should be used to pull the data for integration.
pooled_env <- initialize.project(datasets = c("LCMV1", "LCMV2"),
origins = c("CD44+ cells", "CD44+ cells"),
experiments = c("Rep1", "Rep2"),
data.path = file.path(tempdir(), "LCMV"),
work.path = file.path(tempdir(), "LCMV/LCMV_analysis"))
pooled_env <- read.preclustered.datasets(pooled_env)
pooled_env <- add.confounder.variables(
pooled_env,
ribosomal.score = ribosomal.score(pooled_env),
mitochondrial.score = mitochondrial.score(pooled_env),
cell.cycle.score = cell.cycle.score(pooled_env),
Exhaustion = controlled.mean.score(pooled_env, exhaustion_markers))
pooled_env <- PCA(pooled_env, clear.previously.calculated.clustering = F, local = T)
summarize(pooled_env, contrast = "datasets", local = T)We assessed the similarity between pairs of clusters and identify reproducible subpopulations across the two replicates. Figure 9 shows the correlation between clusters’ FC vectors across replicates (as described in Magen et al 2019).
cluster.similarity <- assess.cluster.similarity(pooled_env)
similarity <- cluster.similarity$similarity
map <- cluster.similarity$map
filtered.similarity <- get.robust.cluster.similarity(
pooled_env, similarity, min.sd = qnorm(.9), max.q.val = 0.01, rerun = F
)
robust.clusters <- sort(unique(c(filtered.similarity$cluster1,
filtered.similarity$cluster2)))
visualize.cluster.cors.heatmaps(pooled_env, pooled_env$work.path,
filtered.similarity)
Fig 9. Correlation between clusters’ FC vectors across the two replicates.
Finally, the cluster similarity between all clusters integrated by this analysis is shown in Figure 10. Unlike the simplified example shown here, this analysis is typically used for estimating subpopulation similarity and divergence across multiple tissue-origins or experimental settings, including corresponding pre-clinical to clinical datasets as described in Magen et al 2019.
similarity <- filtered.similarity
visualize.cluster.similarity.stats(pooled_env, similarity)
Fig 10. Correlation among all the clusters in the two datasets.
Identification and visualization of robust novel marker genes
differential.expression.statistics = get.robust.markers(
pooled_env, cluster_group1 = c('LCMV2_Tfh_CD4', 'LCMV2_Tfh_Tcmp_CD4'),
cluster_group2 = c('LCMV2_CD8_1', 'LCMV2_CD8_2'),
group1_label = 'CD4 T Cells', group2_label = 'CD8 T Cells')
Fig 11. Scatter plot indicating gene activation across two independent groups of cells. X and Y axis values annotate fractions of cells expressing (>0 UMIs) each gene.
Using the expression statistics output and the figure (generated to ‘robust.diff.exp.pdf’) you may identify genes showing exclusive expression in one (or more) selected population (cluster_group1) versus the others (cluster_group2). We can annotate the tSNE with the expression level of selected genes or draw contour plots resembling Flow Cytometric analysis.
plot_contour_overlay_tSNE(pooled_env, genes = c('Cd4','Cd8a'))
Fig 12. tSNE overlay with contour annotation of normalized expression level of CD4 and CD8a.
plot_pair_scatter(pooled_env, gene1 = 'Cd4', gene2 = 'Cd8a',
cluster_group1 = c('LCMV2_Tfh_CD4', 'LCMV2_Tfh_Tcmp_CD4'),
cluster_group2 = c('LCMV2_CD8_1','LCMV2_CD8_2'),
group1_label = 'CD4 T Cells', group2_label = 'CD8 T Cells')
Fig 13. Contours of CD4 vs CD8 normalized expression level.
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Magen et al. “Single-cell profiling of tumor-reactive CD4+ T-cells reveals unexpected transcriptomic diversity” bioRxiv 543199
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Ciucci, Thomas, et al. “The Emergence and Functional Fitness of Memory CD4+ T Cells Require the Transcription Factor Thpok.” Immunity 50.1 (2019): 91-105.
