Lecture 8: A Sprint Through Single Cell RNA-Seq

“ A Sprint Through Single Cell RNA-Seq” is licensed under CC BY by Simon Coetzee.

• Across and within tissues there is a great diversity of cell types, states, and interactions.

• Across and within tissues there is a great diversity of cell types, states, and interactions.
• Single Cell RNA-seq offers a glimpse of what genes are being expressed at the level of individual cells.

• Across and within tissues there is a great diversity of cell types, states, and interactions.
• Single Cell RNA-seq offers a glimpse of what genes are being expressed at the level of individual cells.

• Explore which cell types are present in a tissue.
• Identify unknown/rare cell types or states.
• Examine the changes in gene expression during differentiation processes, or across time, or across states.
• Identify genes that are differentially expressed in particular cell types between conditions (treatment, disease, etc.)
• Explore these changes while incorporating spatial, regulatory, or protien information.

• compares averages of cellular expression.
• is a good choice for quantifying expression signatures for disease studies.
• potential for the discovery of disease biomarkers if you're not expecting or concerned about cellular heterogeneity.

The steps of the workflow are:

• Generation of the count matrix (method-specific steps): formating reads, demultiplexing samples, mapping and quantification
• Quality control of the raw counts: filtering of poor quality cells
• Clustering of filtered counts: clustering cells based on similarities in transcriptional activity (cell types = different clusters)
• Marker identification and cluster annotation: identifying gene markers for each cluster and annotating known cell type clusters
• Optional downstream steps

Regardless of the analysis being done, conclusions about a population based on a single sample per condition are not trustworthy. BIOLOGICAL REPLICATES ARE STILL NEEDED! That is, if you want to make conclusions that correspond to the population and not just the single sample.

scRNA-seq is able to capture expression at the cellular level, however

• sample generation and library prep is more expensive.
• the analysis is much more complicated and more difficult to interpret.

The data complexity involves:

• Large volumes of data
• Low depth of sequencing per cell
• Technical variability across cells/samples
• Biological variability across cells/samples

Expression data from scRNA-seq represents tens or hundres of thousands of reads for thousands of cells.

This output is much larger than normal bulk RNA-seq, and requires higher amounts of memory to analyze, larger storage requirements, and more time to run the analysis.

Uninteresting sources of biological variation can result in gene expression between cells being more similar/different than the actual biological cell types/states, which can obscure the cell type identities. Uninteresting sources of biological variation (unless part of the experiment’s study) include:

• Transcriptional bursting: Gene transcription is not turned on all of the time for all genes. Time of harvest will determine whether gene is on or off in each cell.
• Varying rates of RNA processing: Different RNAs are processed at different rates.
• Continuous or discrete cell identities (e.g. the pro-inflammatory potential of each individual T cell): Continuous phenotypes are by definition variable in gene expression, and separating the continuous from the discrete can sometimes be difficult.
• Environmental stimuli: The local environment of the cell can influence the gene expression depending on spatial position, signaling molecules, etc.
• Temporal changes: Fundamental fluctuating cellular processes, such as cell cycle, can affect the gene expression profiles of individual cells.

Technical sources of variation can result in gene expression between cells being more similar/different based on technical sources instead of biological cell types/states, which can obscure the cell type identities. Technical sources of variation include:

• Cell-specific capture efficiency: Different cells will have differing numbers of transcripts captured resulting in differences in sequencing depth (e.g. 10-50% of transcriptome).
• Library quality: Degraded RNA, low viability/dying cells, lots of free floating RNA, poorly dissociated cells, and inaccurate quantification of cells can result in low quality metrics
• Amplification bias: During the amplification step of library preparation, not all transcripts are amplified to the same level.
• Batch effects: Batch effects are a significant issue for scRNA-Seq analyses, since you can see significant differences in expression due solely to the batch effect.

Goals

• To filter the data to only include true cells that are of high quality, so that when we cluster our cells it is easier to identify distinct cell type populations.

• To identify any failed samples and either try to salvage the data or remove from analysis, in addition to, trying to understand why the sample failed

Challenges

• Delineating cells that are poor quality from less complex cells

• Choosing appropriate thresholds for filtering, so as to keep high quality cells without removing biologically relevant cell types

There are three columns of information:

• orig.ident: this column will contain the sample identity if known. It will default to the value we provided for the project argument when loading in the data
• nCount_RNA: this column represents the number of UMIs per cell
• nFeature_RNA: this column represents the number of genes detected per cell

In order to create the appropriate plots for the quality control analysis, we need to calculate some additional metrics. These include:

• number of genes detected per UMI: this metric with give us an idea of the complexity of our dataset (more genes detected per UMI, more complex our data)
• mitochondrial ratio: this metric will give us a percentage of cell reads originating from the mitochondrial genes

Now that we have generated the various metrics to assess, we can explore them with visualizations. We will assess various metrics and then decide on which cells are low quality and should be removed from the analysis:

• Cell counts
• UMI counts per cell
• Genes detected per cell
• UMIs vs. genes detected
• Mitochondrial counts ratio
• Novelty

The cell counts are determined by the number of unique cellular bar codes detected. For this experiment, between 12,000 -13,000 cells are expected.

In an ideal world, you would expect the number of unique cellular bar codes to correspond to the number of cells you loaded. However, this is not the case as capture rates of cells are only a proportion of what is loaded.

10X capture efficiency is between 50-60%.

Occasionally a hydrogel can have more than one cellular barcode. Similarly, with the 10X protocol there is a chance of obtaining only a barcoded bead in the emulsion droplet (GEM) and no actual cell. Both of these, in addition to the presence of dying cells can lead to a higher number of cellular barcodes than cells.

The UMI counts per cell should generally be above 500, that is the low end of what we expect. If UMI counts are between 500-1000 counts, it is usable but the cells probably should have been sequenced more deeply.

For high quality data, the proportional histogram should contain a single large peak that represents cells that were encapsulated.

There can be a small shoulder to the left of the major peak (not present in our data), or a bimodal distribution of the cells.

• some cells that failed?
• biologically different types of cells
  • quiescent cell populations
  • less complex cells
  • cells that are much smaller

Two metrics that are often evaluated together are the number of UMIs and the number of genes detected per cell.

Cells that are poor quality are likely to have low genes and UMIs per cell.

Mitochondrial read fractions are only high in particularly low count cells with few detected genes (darker colored data points). This could be indicative of damaged/dying cells whose cytoplasmic mRNA has leaked out through a broken membrane, and thus, only mRNA located in the mitochondria is still conserved.

This metric can identify whether there is a large amount of mitochondrial contamination from dead or dying cells. We define poor quality samples for mitochondrial counts as cells which surpass the 0.2 mitochondrial ratio mark, unless of course you are expecting this in your sample.

Can't count on this absolutely - kidney cells often have high mitochrondrial RNA levels - the tissue is associated with mitochondrial function.

Novelty score is computed by taking the ratio of nGenes over nUMI.

If there are many captured transcripts (high nUMI) and a low number of genes detected in a cell, this likely means that you only captured a low number of genes and simply sequenced transcripts from those lower number of genes over and over again.

These low complexity (low novelty) cells could represent a specific cell type (i.e. red blood cells which lack a typical transcriptome), or could be due to some other strange artifact or contamination.

Generally, we expect the novelty score to be above 0.80 for good quality cells.

Consider the joint effects of these metrics when setting thresholds and set them to be as permissive as possible to avoid filtering out viable cell populations unintentionally.

Often the recommendations are a rough guideline, and the specific experiment needs to inform the exact thresholds chosen. We will use the following thresholds:

• nUMI > 500
• nGene > 250
• log10GenesPerUMI > 0.8
• mitoRatio < 0.2

Goals:

• To accurately normalize and scale the gene expression values to account for differences in sequencing depth and overdispersed count values.
• To identify the most variant genes likely to be indicative of the different cell types present.

Challenges:

• Checking and removing unwanted variation so that we do not have cells clustering by artifacts downstream

Recommend:

Regress out number of UMIs (default using sctransform), mitochondrial content, and cell cycle, if needed and appropriate for experiment, so not to drive clustering downstream.

Correction for biological covariates serves to single out particular biological signals of interest, while correcting for technical covariates may be crucial to uncovering the underlying biological signal.

The most common biological data correction is to remove the effects of the cell cycle on the transcriptome.

The raw counts are not comparable between cells and we can’t use them as is for our exploratory analysis.

To assign each cell a score based on its expression of G2/M and S phase markers, we can use the Seuart function CellCycleScoring(). This function calculates cell cycle phase scores based on canonical markers that required as input.

After scoring the cells for cell cycle, we would like to determine whether cell cycle is a major source of variation in our dataset using PCA. To perform PCA, we need to first choose the most variable features, then scale the data.

Scaling data is requred so that our “highly variable genes” don't just reflect high expression.

• adjusting the expression of each gene to give a mean expression across cells to be 0
• scaling expression of each gene to give a variance across cells to be 1

Goals:

To align same cell types across conditions.

Challenges:

Aligning cells of similar cell types so that we do not have clustering downstream due to differences between samples, conditions, modalities, or batches

Recommendations:

Go through the analysis without integration first to determine whether integration is necessary