Authors: Qiyun Zhu (qiyunzhu@gmail.com), Katharina Dittmar (katharinad@gmail.com)

Affiliation: Department of Biological Sciences, University at Buffalo, State University of New York, Buffalo, USA

Zhu Q, Kosoy M, Dittmar K. HGTector: an automated method facilitating genome-wide discovery of putative horizontal gene transfers. BMC Genomics. 2014. 15:717.

Usage: Simply execute perl HGTector.pl, or, open GUI.html in a web browser to see a step-by-step wizard.

Download HGTector 0.2.2.

Address of the bookmark: https://github.com/DittmarLab/HGTector

1) A cell line expressing or lacking single TF,

2) Breast tumors divided along PAM50 designations

3) Whole brain samples from WT mice or mice lacking a single TF in a particular neuronal subtype

4) Single cell RNAseq analysis of neurons divided by Immediate Early Gene expression levels.

In summary, MAGIC is a standalone application that produces meaningful predictions of TFs and cofactors in transcriptomic experiments.

More at https://uwmadison.app.box.com/s/8j90e5h2rjrsz3bacaxnq8kor2o64vyg

Address of the bookmark: https://github.com/asroopra/MAGIC

Address of the bookmark: https://github.com/DessimozLab/OMArk

Targeted bait capture is a technique for sequencing many loci simultaneously based on bait sequences. HybPiper pipeline starts with high-throughput sequencing reads (for example from Illumina MiSeq), and assigns them to target genes using BLASTx or BWA. The reads are distributed to separate directories, where they are assembled separately using SPAdes. The main output is a FASTA file of the (in frame) CDS portion of the sample for each target region, and a separate file with the translated protein sequence.

HybPiper also includes post-processing scripts, run after the main pipeline, to also extract the intronic regions flanking each exon, investigate putative paralogs, and calculate sequencing depth. For more information, please see our wiki.

HybPiper is run separately for each sample (single or paired-end sequence reads). When HybPiper generates sequence files from the reads, it does so in a standardized directory hierarchy. Many of the post-processing scripts rely on this directory hierarchy, so do not modify it after running the initial pipeline. It is a good idea to run the pipeline for each sample from the same directory. You will end up with one directory per run of HybPiper, and some of the later scripts take advantage of this predictable directory structure.

Address of the bookmark: https://github.com/mossmatters/HybPiper

Address of the bookmark: http://sysomics.com/deephic

Address of the bookmark: http://christophergandrud.github.io/d3Network/

https://bmcbioinformatics.biomedcentral.com/articles/10.1186/s12859-020-3371-7

Address of the bookmark: https://github.com/vpalombo/PANEV

More at https://www.ncbi.nlm.nih.gov/pmc/articles/PMC2745767/

Address of the bookmark: http://synorth.genereg.net/

More at https://github.com/AntonBankevich/jumboDB

Address of the bookmark: https://github.com/AntonBankevich/jumboDB

What Does DESeq2 Do?
DESeq2 analyzes count data—the number of sequencing reads that map to each gene. It:

Normalizes the data to account for sequencing depth and library size.

Estimates variance (dispersion) for each gene.

Fits a model to compare groups (e.g., control vs treated).

Calculates fold-changes and p-values to determine significance.

Installing DESeq2

You can install DESeq2 via Bioconductor in R:

if (!requireNamespace("BiocManager", quietly = TRUE))
install.packages("BiocManager")
BiocManager::install("DESeq2")

Inputs Needed

A count matrix: genes as rows, samples as columns (raw counts, not normalized).

A sample metadata table (also called colData): defines the condition/group for each sample.

Example:
# Count matrix (rows = genes, columns = samples)
counts <- read.csv("counts.csv", row.names = 1)

# Sample metadata
colData <- data.frame(
row.names = colnames(counts),
condition = c("control", "control", "treated", "treated")
)

DESeq2 Workflow

1. Load the package
library(DESeq2)
2. Create a DESeqDataSet object
dds <- DESeqDataSetFromMatrix(countData = counts,
colData = colData,
design = ~ condition)
3. Run the differential expression analysis
dds <- DESeq(dds)
4. Get the results
res <- results(dds)
head(res)
This gives a table with:

log2FoldChange: how much expression changed

pvalue: statistical significance

padj: adjusted p-value (FDR corrected)

Visualization (Optional but Powerful)

MA Plot
plotMA(res, ylim = c(-2, 2))

Volcano Plot (custom)
library(ggplot2)
res$significant <- res$padj < 0.05
ggplot(res, aes(x=log2FoldChange, y=-log10(padj), color=significant)) +
geom_point() +
theme_minimal()

Heatmap of Top Genes
library(pheatmap)
topgenes <- head(order(res$padj), 20)
vsd <- vst(dds, blind=FALSE)
pheatmap(assay(vsd)[topgenes, ])

Tips for Best Results
Use raw counts (not normalized or TPM/RPKM values).

Have replicates: DESeq2 relies on variance estimates, so at least 3 per group is ideal.

Watch out for batch effects—include them in your design if needed (e.g., ~ batch + condition).

Summary

Step Purpose
DESeqDataSetFromMatrix() Load your data into DESeq2
DESeq() Run the differential expression analysis
results() Extract the output (log fold change, p-values, etc.)
plotMA() / ggplot2 / pheatmap Visualize the results

Final Thoughts
DESeq2 is an essential tool for RNA-seq data analysis. It abstracts away much of the complexity of statistical modeling, while still giving you control when needed. Whether you're a bioinformatician or a wet-lab biologist, DESeq2 offers both ease of use and analytical power.