Skip to content

Latest commit

 

History

History
692 lines (561 loc) · 22.7 KB

README.md

File metadata and controls

692 lines (561 loc) · 22.7 KB
Raw

Transcriptome landscape of kleptoplastic sea slug Elysia viridis

Manuel Mendoza, Sara Rocha, Jesus Troncoso, David Posada and Carlos A. Canchaya

Sea slugs from the superorder Sacoglossa can sequester functional chloroplast through feeding and keep them photosynthetically active inside their digestive tubules (de Vries, Christa, and Gould 2014). A small polyphyletic group of sacoglossan species can maintain the stolen plastids (kleptoplasts) functional for more than a month (Händeler et al. 2009). Despite an extensive research record (de Vries et al. 2014), some questions remain unsolved: How are the plastids recognised from the other components of prey’s cells? Why do the sea slugs remain alive after weeks of starvation if the photosynthates are not essential? Even if the ability to sequester the plastids has multiple independent origins along the evolution, can we find orthologs related to the time plastids remain active?

We tried to help to answer the three questions sequencing a novel transcriptome from a cosmopolitan species present along the European Atlantic shore, Elysia viridis (Montagu, 1804) (Jensen 2007) and comparing it with other species of sea slugs. The sample collection and the methodology used to find the answers are described below. Although we report new findings, we are sure that further studies will be required to find a clear answer to the questions. We here describe the full pipeline of our analysis.

@article{10.1093/mollus/eyad001,
    author = {Mendoza, Manuel and Rocha, Sara and Troncoso, Jesús and Posada, David and Canchaya, Carlos},
    title = "{Transcriptomic landscape of the kleptoplastic sea slug Elysia viridis}",
    journal = {Journal of Molluscan Studies},
    volume = {89},
    number = {1},
    year = {2023},
    month = {01},
    issn = {0260-1230},
    doi = {10.1093/mollus/eyad001},
    url = {https://doi.org/10.1093/mollus/eyad001},
    note = {eyad001},
    eprint = {https://academic.oup.com/mollus/article-pdf/89/1/eyad001/48945866/eyad001.pdf},
}

Working environment set up

In our analysis we used miniconda3 v4.11.0. This analysis was done using a high-performance computer (CESGA Finisterrae II) using the queue system SLURM, so we added some SLURM-specific options in the different chunks.

# Crete the environment
conda create --yes --name elvira_env

# Add the channels to the list to download the required tools
conda config --add channels conda-forge 
conda config --add channels bioconda
conda config --add channels r

# Install all the tools required for the analysis
conda install --yes --name elvira_env python=3 r-base=4 fastp trinity transrate transdecoder busco blast hmmer fastqc

Reference generation

STEP 1: Reads quality assessment. We checked the quality of our reads using the modules in FastQC.

# Reads quality assessment 
fastqc \
  --extract \
  --nogroup \
  --threads $SLURM_NTASKS \
  --outdir qc_dir \
  sample_1.fq.gz sample_2.fq.gz

STEP 2: Reads trimming using fastp (Chen et al. 2018). We removed remaining sequencing adapters (detected by reads-pairs overlapping), poly-X tails (we did not allow more than 15bp consecutive position with the nucleotide), and low complexity reads (reads with many repetitions). After we trimmed the low-quality positions, requiring a mean quality of 30 phred-score. The final length required after trimming was 70bp.

# Reads quality control
fastp \
  --thread $SLURM_NTASKS \
  --in1 sample_1.fq.gz \
  --in2 sample_2.fq.gz \
  --out1 sample_1.trim.fq.gz \
  --out2 sample_2.trim.fq.gz \
  --json sample.trim.json\
  --html sample.trim.html \
  --detect_adapter_for_pe \
  --low_complexity_filter \
  --complexity_threshold 50 \
  --cut_right \
  --cut_window_size 10 \
  --cut_mean_quality 30 \
  --qualified_quality_phred 30 \
  --unqualified_percent_limit 25 \
  --average_qual 30 \
  --length_required 70 \
  --correction \
  --overrepresentation_analysis \
  --overrepresentation_sampling 5

STEP 3: Transcriptome de novo assembly. We used the clean reads obtained in the previous step to reconstruct the transcripts using Trinity (Haas et al. 2013).

# Transcriptome assembly
Trinity \
  --CPU $SLURM_NTASKS \
  --max_memory 64G \
  --seqType fq \
  --min_contig_length 300 \
  --KMER_SIZE 20 \
  --min_glue 10 \
  --min_per_id_same_path 84 \
  --max_diffs_same_path 16 \
  --left sample_1.trim.fq.gz \
  --right sample_2.trim.fq.gz \
  --output sample-Trinity \
  --full_cleanup

STEP 4: Transcriptome assembly evaluation. We checked the number of molluscan orthologs assembled using BUSCO (Manni et al. 2021) (transcriptome completeness); and we checked the number of transcripts that were assembled correctly using TransRate (Smith-Unna et al. 2016) (transcriptome correctness).

# Check the transcriptome completeness 
busco \
  --force \
  --cpu $SLURM_NTASKS \
  --evalue 1e-6 \
  --in sample_transcripts.fna \
  --out mollusca_ort \
  --mode transcriptome \
  --lineage_dataset mollusca_odb10  

# Check the transcriptome correctness 
transrate \
  --threads $SLURM_NTASKS \
  --assembly sample_transcripts.fna \
  --left sample_1.trim.fq.gz \
  --right sample_1.trim.fq.gz \
  --output sample_cor

STEP 5: Protein-coding sequences identification. We extracted the protein coding sequences from the transcript assembled correctly using TransDecoder. After that, we removed the redundant sequences using seqkit (Shen et al. 2016).

# Create the transcript to gene map
${TRINITY_HOME}/util/support_scripts/get_Trinity_gene_to_trans_map.pl \
  sample.good.fasta > sample.good.gtm

# Extract the protein-coding sequences
TransDecoder.LongOrfs \
  -t sample.good.fasta \
  --gene_trans_map sample.good.gtm \
  --output_dir sample.good-cds

TransDecoder.Predict \
  --single_best_only \
  -t sample.good.fasta \
  --output_dir sample.good-cds

# Remove redundant sequences
seqkit rmdup \
  --threads $SLURM_NTASKS \
  --ignore-case \
  --by-seq \
  --out-file sample.good.rmdup.faa \
  sample.good.faa

STEP 6: Possible biological contamination removal. After removing the possible miss-assemblies, we pulled the potential contaminants from other organisms (bacteria, algae, etc.). We aligned the reads to the NCBI non-redundant protein database and from that we extracted the taxonomic information from these matches using the taxonomizr R package. We only kept the sequences that matched with a molluscan protein from the genera Elysia, Aplysia and Plakobranchus. Previously to define the filtering condition, we explored the taxonomy of all the matches to find the most appropriate limits.

# Local alignment to identify the product
blastp \
  -num_threads $SLURM_NTASKS \ 
  -task blastp-fast \
  -evalue 1e-3 \
  -max_hsps 1 \
  -max_target_seqs 1 \
  -outfmt "6 qseqid sseqid pident length mismatch gapopen qstart qend sstart send evalue bitscore qlen slen qcovs" \
  -db nr \
  -query sample.good.rmdup.faa \
  -out sample.good.rmdup.nr.tsv
# Attach the packages
library(taxonomizr)
library(Biostrings)
library(stringr)
library(readr)
library(dplyr)

# Prepare the database (do only the 1st time)
getNamesAndNodes()
getAccession2taxid(types = c("nucl_wgs", "nucl_gb", "prot"))
read.names.sql("names.dmp", "accessionTaxa.sql")
read.nodes.sql("nodes.dmp", "accessionTaxa.sql")
read.accession2taxid(list.files(".", "accession2taxid.gz$"), "accessionTaxa.sql")

# Load the transcripts sequences and the output from STEP 5A
prot_good <- readAAStringSet("sample.good.rmdup.faa")
blast_out <- read_delim(file = "sample.good.rmdup.nr.tsv", col_names = FALSE) %>%
  select("X1", "X2") %>%
  rename("tx_name" = "X1", "nr_accs" = "X2")

# Extract the taxonomic information from the proteins ID
prot_taxa <- tibble(
  "nr_accs" = unique(sort(blast_out %>% pull("nr_accs"))),
  "nr_egid" = accessionToTaxa(nr_accs, "accessionTaxa.sql")
  ) %>%
  bind_cols(getTaxonomy(nr_accs %>% pull(nr_egid), "accessionTaxa.sql"))

# Filter by Genus to keep only sea slugs
prot_filt <- prot_taxa %>% 
  filter(genus %in% c("Aplysia", "Elysia", "Plakobranchus")) %>%
  inner_join(blast_out)
prot_filt <- prot_good[prot_filt %>% pull(tx_name)]

# Rename the final transcripts to handle simple names
new_sqaccs <- paste0("SPNAME", str_pad(1:length(prot_good), width = nchar(length(prot_good)), pad = "0"))
old_sqaccs <- names(prot_filt)
accs_convr <- tibble("qseqid" = old_sqaccs, "qseqid_new" = new_sqaccs)
names(prot_filt) <- new_sqaccs

# Change the sequence accession in the alignment
col_names <- c("qseqid", "sseqid", "pident", "length", "mismatch", "gapopen", "qstart", "qend", "sstart", "send", "evalue", "bitscore", "qlen", "slen", "qcovs")
res_blast <- read_delim(file = "sample.good.rmdup.nr.tsv", col_names = col_names) %>%
  inner_join(accs_convr) %>%
  select(!qseqid) %>%
  rename("qseqid" = "qseqid_new")

# Export the final transcriptome
writeXStringSet(x = prot_filt, filepath = "sample.good.rmdup.slugs.faa", append = FALSE)
write_delim(x = res_blast, file = "sample.good.rmdup.slugs.nr.tsv", delim = "\t", col_names = FALSE)

STEP 7: Protein homology prediction. We tried to predict the product of the transcripts by local alignment using BLASTP (Altschul et al. 1990; shiryev2007improved?; Camacho et al. 2009). We annotated the transcriptome using four databases: NCBI Nr, NCBI RefSeq Protein (Sayers et al. 2021), UniProt TrEMBL and UniProt TrEMBL limited to molluscan entries (UniProt Consortium 2021).

# Identify the homologous proteins 
blastp \
  -num_threads $SLURM_NTASKS \
  -task blastp \
  -evalue 1e-6 \
  -max_hsps 1 \
  -max_target_seqs 1 \
  -outfmt "6 qseqid sseqid pident length mismatch gapopen qstart qend sstart send evalue bitscore qlen slen qcovs" \
  -db dbname \
  -query sample.good.rmdup.slugs.faa \
  -out sample.good.rmdup.slugs.dbname.tsv

STEP 8: Protein domain identification. We identified the different protein domains from the filtered transcripts using HMMER (Eddy 2011) and the database Pfam (Mistry et al. 2021).

# Identify the different protein domains
hmmsearch \
  --cpu $SLURM_NTASKS \
  --tblout sample.good.rmdup.slugs.seqdom.tsv \
  --domtblout sample.good.rmdup.slugs.ptrdom.tsv \
  -E 1e-6 \
  --domE 1e-6 \
  --incE 1e-6 \
  --incdomE 1e-6 \
  pfam \
  sample.good.rmdup.slugs.faa

STEP 9: Gene Ontology annotation. We predicted the GO associated with each transcript using the homologous proteins (STEP 7 using TrEMBL DB) and the protein domains (STEP 8). Additionally, we required an extra file containing the conversion between protein accession and the GO IDs; this information can be obtained using the ID mapping tool.

# Extract the protein accessions to convert into GO IDs
awk '{print $1}' sample.good.rmdup.slugs.trembl.tsv | sort -u > sample.good.rmdup.slugs.prot2go.tsv
# Attach the packages
library(elvira)

# Add GO annotations to the transcripts 
txann <- go_annotation( 
  trans_blast = "sample.good.rmdup.slugs.trembl.tsv", 
  trans_hmm   = "sample.good.rmdup.slugs.seqdom.tsv", 
  unip_goid   = "sample.good.rmdup.slugs.prot2go.tsv"
  )

# Export the annotation
write_delim(txann, file = "sample.good.rmdup.slugs.trans2go.tsv", delim = "\t", col_names = FALSE)

STEP 10: Additional functional annotation using an orthologs database. After filtering the sequences and obtaining the final transcriptome (sample.good.rmdup.slugs.faa) we sent it for functional annotation using the eggNOG webportal (Huerta-Cepas et al. 2019; Cantalapiedra et al. 2021) with the following options:

  • protein sequences
  • minimum hit e-value = 1e-6
  • percentage identity = 60
  • minimum % of query coverage = 50
  • Gene Ontology evidence = Transfer all annotations
  • PFAM refinement = realign queries to the whole PFAM DB
  • SMART annotation = Perform SMART annotation.

The other options were set by default.

Additional steps

Over-represented sequences analysis: We extracted the overrepresented sequences identified using FastQC and aligned them to the Nucleotide database. The result is showed in the Table S2.

# Attach the packages
library(fastqcr)
library(dplyr)
library(Biostrings)

# Extract the overrepresented sequences and their abundance
overseq_tbl <- full_join(
  qc_plot(qc_read("sample_1_fastqc.zip"), "Overrepresented sequences") %>% select(Sequence, Count) %>% rename("frcts" = Count),
  qc_plot(qc_read("sample_2_fastqc.zip"), "Overrepresented sequences") %>% select(Sequence, Count) %>% rename("rvcts" = Count)
  )

# Export overrepresented sequences
overseq <- DNAStringSet(overseq_tbl %>% pull(Sequence))
names(overseq) <- paste0("ELVIRA_OVERSEQ-", 1:nrow(overseq_tbl))
writeXStringSet(x = overseq, filepath = "sample.overseq.fna", append = FALSE)
# Align the overrepresented sequences to the Nucleotide database 
blastn \
  -num_threads $SLURM_NTASKS \
  -task blastn-short \
  -db nt \
  -query sample.overseq.fna
  -out sample.overseq.nt.tsv \
  -evalue 1e-3 \
  -outfmt 6 \
  -perc_identity 75 \
  -max_target_seqs 1 \
  -max_hsps 1

Transcriptome fragmentation: We checked if the transcript were assembled completely and the proteins coverage (we required the alignment obtained in the STEP 7).

# Calculate fragmentation and protein coverage
trans_frag <- check_completeness(
  prot_seqs  = "sample.good.rmdup.slugs.faa",
  prot_blast = "sample.good.rmdup.slugs.nr.tsv"
)

# Export the result
write_delim(trans_frag, file = "sample.fragmentation.tsv", delim = "\t", append = FALSE, col_names = TRUE)

Orthogroups detection: We detected the different orthogroups using OrthoFinder (Emms and Kelly 2019). After, these sequences were aligned using MAFFT (Katoh et al. 2002). OrthoFinder is not reporting the final species tree correctly (Issue #732)[davidemms/OrthoFinder#732] so, we had to build it using an alternaltive approach.

# Create a dump directory to store the different transcriptomes
mkdir ref_sequences

# Run OrthoFinder
orthofinder \
  -f ref_sequences \
  -a $SLURM_NTASKS \
  -M msa \
  -A mafft \
  -T raxml-ng \
  -o slugs_ortphy

Building the species tree:

# Estimate the substitution model
modeltest-ng \
  --force \
  --processes $SLURM_NTASKS \ 
  --datatype aa \
  --input slugs_ortphy/*/MultipleSequenceAlignments/SpeciesTreeAlignment.fa \
  --output SpeciesTreeAlignment.model \
  --topology ml \
  --frequencies e \
  --model-het f \
  --template raxml

# Build the ML tree
raxml-ng \
  --redo \
  --threads $SLURM_NTASKS \
  --all \
  --check \
  --msa slugs_ortphy/*/MultipleSequenceAlignments/SpeciesTreeAlignment.fa \
  --model MODEL \
  --blopt nr_safe \
  --bs-trees 10000

Orthogroups gene-ontology enrichment

# Attach the libraries
library(topGO)
library(readr)
library(dplyr)
library(stringr)

# Load the Orthogroups information
cnames      <- c("Orthogroup", "ACA", "ECH", "ECO", "ECR", "EOR", "ETI", "EVI", "OVI", "POC")
orthogroups <- read_delim(file = "orthofinder_dir/Orthogroups.tsv", delim = "\t", col_names = cnames, skip = 1) 

# Load ELVIRA annotation
txannotation <- readMappings(file = "sample.good.rmdup.slugs.trans2go.tsv", sep = "\t", IDsep = ";")  
# Pick up the genes of interest
# KLEPTOPLASTY
txsubset <- orthogroups %>% 
  filter(is.na(ACA), is.na(OVI), !is.na(ECO), !is.na(EOR), !is.na(ECR), !is.na(ETI), !is.na(ECH), !is.na(EVI), !is.na(POC)) %>%
  pull(EVI) 

# LONG-TERM RETAINERS
txsubset <- orthogroups %>% 
  filter(is.na(ACA), is.na(OVI), is.na(ECO), is.na(EOR), !is.na(ECR), !is.na(ETI), !is.na(ECH), !is.na(EVI), !is.na(POC)) %>%
  pull(EVI) 

# LTR ULVOPHYCEAE-FEEDER
txsubset <- orthogroups %>% 
  filter(is.na(ACA), is.na(OVI), is.na(ECO), is.na(EOR), !is.na(ECR), !is.na(ETI), is.na(ECH), !is.na(EVI), !is.na(POC)) %>%
  pull(EVI) 

# Select the genes of interest 
txsubset <- unlist(str_split(string = txsubset, pattern = ", "))
txsubset <- factor(as.integer(names(txannotation) %in% txsubset))
names(txsubset) <- names(txannotation)
# Perform GO-term enrichment
# Biological Process
bp_godata <- new("topGOdata", ontology = "BP", allGenes = txsubset, annot = annFUN.gene2GO, gene2GO = txannotation)
bp_enrichment <- runTest(object = bp_godata, algorithm = "weight01", statistic = "t")
bp_enrichment <- GenTable(object = bp_godata, pvalue = bp_enrichment, topNodes = 2583)

# Cellular Component
cc_godata <- new("topGOdata", ontology = "CC", allGenes = txsubset, annot = annFUN.gene2GO, gene2GO = txannotation)
cc_enrichment <- runTest(object = cc_godata, algorithm = "weight01", statistic = "t")
cc_enrichment <- GenTable(object = cc_godata, pvalue = cc_enrichment, topNodes = 683)

# Molecular Function
mf_godata <- new("topGOdata", ontology = "MF", allGenes = txsubset, annot = annFUN.gene2GO, gene2GO = txannotation)
mf_enrichment <- runTest(object = mf_godata, algorithm = "weight01", statistic = "t")
mf_enrichment <- GenTable(object = mf_godata, pvalue = mf_enrichment, topNodes = 1606)

# Binding enrichment result
go_enrichment <- tibble(bind_rows(
  bp_enrichment %>% mutate("go_class" = "BP"),
  cc_enrichment %>% mutate("go_class" = "CC"),
  mf_enrichment %>% mutate("go_class" = "MF")
)) %>%
  mutate(pvalue   = str_replace(string = pvalue, pattern = "< ", replacement = ""),
         pvalue   = as.numeric(pvalue),
         go_class = factor(go_class, levels = c("BP", "CC", "MF")))

# Export the result
write_delim(x = go_enrichment, file = "go_enrichment.tsv", delim = "\t", append = FALSE, col_names = TRUE)

References

Altschul, Stephen F, Warren Gish, Webb Miller, Eugene W Myers, and David J Lipman. 1990. “Basic Local Alignment Search Tool.” Journal of Molecular Biology 215 (3): 403–10.

Camacho, Christiam, George Coulouris, Vahram Avagyan, Ning Ma, Jason Papadopoulos, Kevin Bealer, and Thomas L Madden. 2009. “BLAST+: Architecture and Applications.” BMC Bioinformatics 10 (1): 1–9.

Cantalapiedra, Carlos P, Ana Hernández-Plaza, Ivica Letunic, Peer Bork, and Jaime Huerta-Cepas. 2021. “eggNOG-Mapper V2: Functional Annotation, Orthology Assignments, and Domain Prediction at the Metagenomic Scale.” Molecular Biology and Evolution 38 (12): 5825–29.

Chen, Shifu, Yanqing Zhou, Yaru Chen, and Jia Gu. 2018. “Fastp: An Ultra-Fast All-in-One FASTQ Preprocessor.” Bioinformatics 34 (17): i884–90.

de Vries, Jan, Gregor Christa, and Sven B Gould. 2014. “Plastid Survival in the Cytosol of Animal Cells.” Trends in Plant Science 19 (6): 347–50.

de Vries, Jan, Cessa Rauch, Gregor Christa, and Sven B Gould. 2014. “A Sea Slug’s Guide to Plastid Symbiosis.” Acta Societatis Botanicorum Poloniae 83 (4).

Eddy, Sean R. 2011. “Accelerated Profile HMM Searches.” PLoS Computational Biology 7 (10): e1002195.

Emms, David M, and Steven Kelly. 2019. “OrthoFinder: Phylogenetic Orthology Inference for Comparative Genomics.” Genome Biology 20 (1): 1–14.

Haas, Brian J, Alexie Papanicolaou, Moran Yassour, Manfred Grabherr, Philip D Blood, Joshua Bowden, Matthew Brian Couger, et al. 2013. “De Novo Transcript Sequence Reconstruction from RNA-Seq Using the Trinity Platform for Reference Generation and Analysis.” Nature Protocols 8 (8): 1494–1512.

Händeler, Katharina, Yvonne P Grzymbowski, Patrick J Krug, and Heike Wägele. 2009. “Functional Chloroplasts in Metazoan Cells-a Unique Evolutionary Strategy in Animal Life.” Frontiers in Zoology 6 (1): 1–18.

Huerta-Cepas, Jaime, Damian Szklarczyk, Davide Heller, Ana Hernández-Plaza, Sofia K Forslund, Helen Cook, Daniel R Mende, et al. 2019. “eggNOG 5.0: A Hierarchical, Functionally and Phylogenetically Annotated Orthology Resource Based on 5090 Organisms and 2502 Viruses.” Nucleic Acids Research 47 (D1): D309–14.

Jensen, Kathe R. 2007. “Biogeography of the Sacoglossa (Mollusca, Opisthobranchia).” Bonner Zoologische Beiträge 55 (3/4): 255–81.

Katoh, Kazutaka, Kazuharu Misawa, Kei-ichi Kuma, and Takashi Miyata. 2002. “MAFFT: A Novel Method for Rapid Multiple Sequence Alignment Based on Fast Fourier Transform.” Nucleic Acids Research 30 (14): 3059–66.

Manni, Mosè, Matthew R Berkeley, Mathieu Seppey, Felipe A Simão, and Evgeny M Zdobnov. 2021. “BUSCO Update: Novel and Streamlined Workflows Along with Broader and Deeper Phylogenetic Coverage for Scoring of Eukaryotic, Prokaryotic, and Viral Genomes.” Molecular Biology and Evolution 38 (10): 4647–54.

Mistry, Jaina, Sara Chuguransky, Lowri Williams, Matloob Qureshi, Gustavo A Salazar, Erik LL Sonnhammer, Silvio CE Tosatto, et al. 2021. “Pfam: The Protein Families Database in 2021.” Nucleic Acids Research 49 (D1): D412–19.

Sayers, Eric W, Jeffrey Beck, Evan E Bolton, Devon Bourexis, James R Brister, Kathi Canese, Donald C Comeau, et al. 2021. “Database Resources of the National Center for Biotechnology Information.” Nucleic Acids Research 49 (D1): D10.

Smith-Unna, Richard, Chris Boursnell, Rob Patro, Julian M Hibberd, and Steven Kelly. 2016. “TransRate: Reference-Free Quality Assessment of de Novo Transcriptome Assemblies.” Genome Research 26 (8): 1134–44.

UniProt Consortium. 2021. “UniProt: The Universal Protein Knowledgebase in 2021.” Nucleic Acids Research 49 (D1): D480–89.