,
Tian Wang [aut] ,
John Platig [aut],
Marieke Kuijjer [aut] ,
Megha Padi [aut] ,
Rebekka Burkholz [aut],
Des Weighill [aut] ,
Kate Shutta [aut] | Title: | Unified methods for the inference and analysis of gene regulatory networks |
|---|---|
| Description: | netZooR unifies the implementations of several Network Zoo methods (netzoo, netzoo.github.io) into a single package by creating interfaces between network inference and network analysis methods. Currently, the package has 3 methods for network inference including PANDA and its optimized implementation OTTER (network reconstruction using mutliple lines of biological evidence), LIONESS (single-sample network inference), and EGRET (genotype-specific networks). Network analysis methods include CONDOR (community detection), ALPACA (differential community detection), CRANE (significance estimation of differential modules), MONSTER (estimation of network transition states). In addition, YARN allows to process gene expresssion data for tissue-specific analyses and SAMBAR infers missing mutation data based on pathway information. |
| Authors: | Marouen Ben Guebila [aut, cre]
,
Tian Wang [aut] ,
John Platig [aut],
Marieke Kuijjer [aut] ,
Megha Padi [aut] ,
Rebekka Burkholz [aut],
Des Weighill [aut] ,
Kate Shutta [aut] |
| Maintainer: | Marouen Ben Guebila <[email protected]> |
| License: | GPL-3 |
| Version: | 1.9.0 |
| Built: | 2024-09-28 07:01:59 UTC |
| Source: | https://github.com/bioc/netZooR |
converts adjacency matrix to edge list
adjMatToElist(adj_mat)adjMatToElist(adj_mat)
adj_mat |
adjacency matrix |
edge list
This function compares two networks and finds the sets of nodes that best characterize the change in modular structure
alpaca(net.table, file.stem, verbose = FALSE)alpaca(net.table, file.stem, verbose = FALSE)
net.table |
A table of edges, with the first column representing the TFs ("from" nodes) and the second column representing the targets ("to" nodes). The third column contains the edge weights corresponding to the control or healthy network, and the fourth column contains the edge weights for the disease network or network of interest. |
file.stem |
The folder location and title under which all results will be stored. |
verbose |
Indicates whether the full differential modularity matrix should also be written to a file. Defaults to FALSE. modularity |
List where first element is the membership vector and second element is the contribution score of each node to its module's total differential modularity
example_path <- system.file("extdata", "Example_2comm.txt", package = "netZooR", mustWork = TRUE) simp.mat <- read.table(example_path,header=TRUE) simp.alp <- alpaca(simp.mat,NULL,verbose=FALSE)example_path <- system.file("extdata", "Example_2comm.txt", package = "netZooR", mustWork = TRUE) simp.mat <- read.table(example_path,header=TRUE) simp.alp <- alpaca(simp.mat,NULL,verbose=FALSE)
This function uses the pseudo-inverse to find the optimal linear transformation mapping the community structures of two networks, then ranks nodes in the network by how much they deviate from the linear mapping.
alpacaCommunityStructureRotation(net1.memb, net2.memb)alpacaCommunityStructureRotation(net1.memb, net2.memb)
net1.memb |
The community membership for Network 1. |
net2.memb |
The community membership for Network 2. |
A ranked list of nodes.
a <- 1 #place holdera <- 1 #place holder
This functions takes the precomputed differential modularity matrix and the genLouvain membership to compute the differential modularity score.
alpacaComputeDifferentialScoreFromDWBM(dwbm, louv.memb)alpacaComputeDifferentialScoreFromDWBM(dwbm, louv.memb)
dwbm |
differential modularity matrix |
louv.memb |
louvain community membership |
Vector of differntial modularity score
This function computes the differential modularity matrix for weighted bipartite networks. The community structure of the healthy network is rescaled by the ratio of m (the total edge weight) of each network.
alpacaComputeDWBMmatmScale(edge.mat, ctrl.memb)alpacaComputeDWBMmatmScale(edge.mat, ctrl.memb)
edge.mat |
A table of edges, with the first column representing the TFs ("from" nodes) and the second column representing the targets ("to" nodes). The third column contains the edge weights corresponding to the control or healthy network, and the fourth column contains the edge weights for the disease network or network of interest. |
ctrl.memb |
The community membership for the control (healthy) network. |
The differential modularity matrix, with rows representing "from" nodes and columns representing "to" nodes.
a <- 1 # place holdera <- 1 # place holder
This function computes the modularity matrix for a weighted bipartite network.
alpacaComputeWBMmat(edge.mat)alpacaComputeWBMmat(edge.mat)
edge.mat |
A table of edges, with the first column representing the TFs ("from" nodes) and the second column representing the targets ("to" nodes). The third column contains the edge weights corresponding to the network of interest. |
Modularity matrix with rows representing TFs ("from" nodes) and columns repesenting targets ("to" nodes)
a <- 1 # example place holdera <- 1 # example place holder
Find the robust nodes in ALPACA community using CRANE
alpacaCrane(input, alp, alpha = 0.1, beta = 0, iteration = 30, isParallel = F)alpacaCrane(input, alp, alpha = 0.1, beta = 0, iteration = 30, isParallel = F)
input |
same input for alpaca: first column TF, second column Genes, third column edge weights from baseline condition, fourth column edge weights from disease condition. |
alp |
alpca object in list format (output from alpaca package) |
alpha |
alpha paramter perturbs each edge weights |
beta |
beta parameter perturbs the strength of each node. Set this to 0 if you want nodes to have node strength identical to the orignal network. |
iteration |
Number of CRANE distributions to create. Higher value leads to better ranking but longer runtime. |
isParallel |
TRUE = use Multithread / FALSE = do not use Multithread |
list of data frames
## Not run: input=cbind(nonAng,ang[,3]) alp=alpaca(input,NULL,verbose = F) alpListObject=alpacaCrane(input, alp, isParallel = T) ## End(Not run)## Not run: input=cbind(nonAng,ang[,3]) alp=alpaca(input,NULL,verbose = F) alpListObject=alpacaCrane(input, alp, isParallel = T) ## End(Not run)
Takes two networks, subtracts edges individually, and then clusters the subtracted network using CONDOR.
alpacaDeltaZAnalysis(net.table, file.stem)alpacaDeltaZAnalysis(net.table, file.stem)
net.table |
A table of edges, with the first column representing the TFs ("from" nodes) and the second column representing the targets ("to" nodes). The third column contains the edge weights corresponding to the control or healthy network, and the fourth column contains the edge weights for the disease network or network of interest. |
file.stem |
The folder location and title under which all results will be stored. |
List where first element is the membership vector and second element is the contribution score of each node to its community's modularity in the final edge-subtracted network
a <- 1 # example place holdera <- 1 # example place holder
Takes two networks, subtracts edges individually, and then clusters the subtracted network using Louvain method.
alpacaDeltaZAnalysisLouvain(net.table, file.stem)alpacaDeltaZAnalysisLouvain(net.table, file.stem)
net.table |
A table of edges, with the first column representing the TFs ("from" nodes) and the second column representing the targets ("to" nodes). The third column contains the edge weights corresponding to the control or healthy network, and the fourth column contains the edge weights for the disease network or network of interest. |
file.stem |
The folder location and title under which all results will be stored. |
List where first element is the membership vector and second element is the contribution score of each node to its community's modularity in the final edge-subtracted network
a <- 1 # example place holdera <- 1 # example place holder
This function outputs the top target genes in each module, ranked by their contribution to the differential modularity of the particular module in which they belong.
alpacaExtractTopGenes(module.result, set.lengths)alpacaExtractTopGenes(module.result, set.lengths)
module.result |
A table of edges, with the first column representing the TFs ("from" nodes) and the second column representing the targets ("to" nodes). The third column contains the edge weights corresponding to the control or healthy network, and the fourth column contains the edge weights for the disease network or network of interest. |
set.lengths |
The desired lengths of the top gene lists. |
List with two elements. First element is a list of the top target genes in each cluster. Second element is a vector with the names of the gene sets. The names are in the format "number_length", where number is the module number label and length is the length of the gene set.
example_path <- system.file("extdata", "Example_2comm.txt", package = "netZooR", mustWork = TRUE) simp.mat <- read.table(example_path,header=TRUE) simp.alp <- alpaca(simp.mat,NULL,verbose=FALSE) alpacaExtractTopGenes(simp.alp, set.lengths=c(2,2))example_path <- system.file("extdata", "Example_2comm.txt", package = "netZooR", mustWork = TRUE) simp.mat <- read.table(example_path,header=TRUE) simp.alp <- alpaca(simp.mat,NULL,verbose=FALSE) alpacaExtractTopGenes(simp.alp, set.lengths=c(2,2))
This function implements the Louvain optimization scheme on a general symmetric matrix. First, nodes are all placed in separate communities, and merged iteratively according to which merge moves result in the greatest increase in the modularity sum. Note that nodes are iterated in the order of the input matrix (not randomly) so that all results are reproducible. Second, the final community membership is used to form a alpacaMetaNetwork whose nodes represent communities from the prevous step, and which are connected by effective edge weights. The merging process is then repeated on the alpacaMetaNetwork. These two steps are repeated until the modularity sum does not increase more than a very small tolerance factor. New
alpacaGenLouvain(B)alpacaGenLouvain(B)
B |
Symmetric modularity matrix |
The community membership vector
a <- 1 # example place holdera <- 1 # example place holder
get the member vector from alpaca object
alpacaGetMember(alp, target = "all")alpacaGetMember(alp, target = "all")
alp |
alpaca object |
target |
tf, gene, or all |
member vector
Get all the genes in the top-scoring lists which are annotated with the enriched GO terms. Only GO terms with at least 3 genes in the overlap are included.
alpacaGOtabtogenes(go.result, dm.top)alpacaGOtabtogenes(go.result, dm.top)
go.result |
The result of the GO term analysis (alpacaListToGo) |
dm.top |
The result of extracting the top genes of the differential modules (dm.top) |
A vector with strings representing gene lists, each element of the vector has the genes in that GO term and community pasted together with spaces in between.
a <- 1 # example place holdera <- 1 # example place holder
This function extracts all the gene symbols associated with a GO term and its descendants. (v1)
alpacaGoToGenes(go.term)alpacaGoToGenes(go.term)
go.term |
The GO Biological Process ID (string). |
A vector of all gene symbols associated with the GO term.
a <- 1 # example place holdera <- 1 # example place holder
GO term enrichment is run using the GOstats package, and corrected for multiple testing using the Benjamini-Hochberg method.
alpacaListToGo(gene.list, univ.vec, comm.nums)alpacaListToGo(gene.list, univ.vec, comm.nums)
gene.list |
A list consisting of vectors of genes; genes must be identified by their official gene symbols. |
univ.vec |
A vector of all gene symbols that were present in the original network. This set is used as the universe for running the hypergeometric test in GOstats. |
comm.nums |
A vector of names for the gene sets in the input parameter "gene.list". These are used to create the table of final results. |
A table whose rows represent enriched GO terms (p_adj<0.05) and columns describe useful properties, like the name of the GO term, the label of the gene set which is enriched in that GO term, the adjusted p-value and Odds Ratio.
a <- 1 # example place holdera <- 1 # example place holder
Computes the "effective" adjacency matrix of a alpacaMetaNetwork whose nodes represent communities in the larger input matrix.
alpacaMetaNetwork(J, S)alpacaMetaNetwork(J, S)
J |
The modularity matrix |
S |
The community membership vector from the previous round of agglomeration. |
The differential modularity matrix, with rows representing "from" nodes and columns representing "to" nodes.
a <- 1 # example place holdera <- 1 # example place holder
In gene regulatory networks, transcription factors can act as both "from" nodes (regulators) and "to" nodes (target genes), so the network analysis functions automatically tag the two columns to differentiate them. This function removes those tags from the gene identifiers.
alpacaNodeToGene(x)alpacaNodeToGene(x)
x |
Tagged node identifier |
Untagged node name
a <- 1 # example place holdera <- 1 # example place holder
Converts alpaca output into list of data frames
alpacaObjectToDfList(alp)alpacaObjectToDfList(alp)
alp |
alpaca object |
list of data frames
Takes two networks, finds community structure of each one individually using CONDOR, and then ranks the nodes that show the biggest difference in their community membership.
alpacaRotationAnalysis(net.table)alpacaRotationAnalysis(net.table)
net.table |
A table of edges, with the first column representing the TFs ("from" nodes) and the second column representing the targets ("to" nodes). The third column contains the edge weights corresponding to the control or healthy network, and the fourth column contains the edge weights for the disease network or network of interest. |
Vector of nodes ordered by how much they change their community membership between the two networks.
a <- 1 # example place holdera <- 1 # example place holder
Takes two networks, finds community structure of each one individually using a generalization of the Louvain method, and then ranks the nodes that show the biggest difference in their community membership.
alpacaRotationAnalysisLouvain(net.table)alpacaRotationAnalysisLouvain(net.table)
net.table |
A table of edges, with the first column representing the TFs ("from" nodes) and the second column representing the targets ("to" nodes). The third column contains the edge weights corresponding to the control or healthy network, and the fourth column contains the edge weights for the disease network or network of interest. |
Vector of nodes ordered by how much they change their community membership between the two networks.
a <- 1 # example place holdera <- 1 # example place holder
This function creates a pair of networks given user-defined parameters for the modular structure of the first (healthy) network and the type of added module in the second (disease) network.
alpacaSimulateNetwork( comm.sizes, edge.mat, num.module, size.module, dens.module )alpacaSimulateNetwork( comm.sizes, edge.mat, num.module, size.module, dens.module )
comm.sizes |
A two-column matrix indicating the number of "from" nodes (left column) and number of "to" nodes (right column) in each community (row). |
edge.mat |
A matrix indicating the number of edges from the TFs in community i (rows) to target genes in community j (columns). |
num.module |
The number of modules that will be added to simulate the disease network. |
size.module |
A two-column matrix indicating the number of "from" and "to" nodes in each new module (row) that will be added to simulate the disease network. |
dens.module |
A vector of length num.module, indicating the edge density of each added module. |
A list with two elements. The first element is a four-column edge table of the same form that is input into the differential modularity function. The second element is a list of all the new nodes in the modules that were added to create the disease network.
a <- 1 # example place holdera <- 1 # example place holder
This function computes the enrichment of selected nodes in a ranked list, using Wilcoxon, Kolmogorov-Smirnov, and Fisher exact tests.
alpacaTestNodeRank(node.ordered, true.pos)alpacaTestNodeRank(node.ordered, true.pos)
node.ordered |
An ordered list of nodes (high-scoring to low-scoring). |
true.pos |
The selected set of nodes being tested for enrichment among the ranked list. |
A vector of 4 values. 1) Wilcoxon p-value, 2) KS p-value, 3) Fisher p-value, 4) Fisher odds ratio.
a <- 1 # example place holdera <- 1 # example place holder
This is a helper function alpacaGenLouvain. It re-numbers the communities so that they run from 1 to N increasing through the vector.
alpacaTidyConfig(S)alpacaTidyConfig(S)
S |
The community membership vector derived from the previous round of agglomeration. |
The renumbered membership vector.
a <- 1 # example place holdera <- 1 # example place holder
Takes a list of gene sets named using gene identifiers and converts them to a list of symbols given a user-defined annotation table.
alpacaTopEnsembltoTopSym(mod.top, annot.vec)alpacaTopEnsembltoTopSym(mod.top, annot.vec)
mod.top |
A list of gene sets (gene identifiers) |
annot.vec |
A vector of gene symbols with gene identifiers as the names of the vector, that defines the translation between annotations. |
A list of sets of gene symbols.
a <- 1 # example place holdera <- 1 # example place holder
This function implements a generalized form of the Louvain method for weighted bipartite networks.
alpacaWBMlouvain(net.frame)alpacaWBMlouvain(net.frame)
net.frame |
A table of edges, with the first column representing the TFs ("from" nodes) and the second column representing the targets ("to" nodes). The third column contains the edge weights corresponding to the network of interest. |
List where first element is the community membership vector and second element is the contribution score of each node to its community's portion of the bipartite modularity.
a <- 1 # example place holdera <- 1 # example place holder
This function performs community structure clustering using
the bipartite modularity described in
condorModularityMax. This function uses a standard
(non-bipartite) community structure clustering of the uni-partite,
weighted projection of the original bipartite graph as an initial
guess for the bipartite modularity.
condorCluster( condor.object, cs.method = "LCS", project = TRUE, low.memory = FALSE, deltaQmin = "default" )condorCluster( condor.object, cs.method = "LCS", project = TRUE, low.memory = FALSE, deltaQmin = "default" )
condor.object |
Output of make.condor.object. This function uses
|
cs.method |
is a string to specify which unipartite community
structure algorithm should be used for the seed clustering.
Options are |
project |
Provides options for initial seeding of the bipartite
modularity maximization.
If TRUE, the nodes in the first column of |
low.memory |
If TRUE, uses |
deltaQmin |
convergence parameter determining the minimum required increase
in the modularity for each iteration. Default is min(10^-4,1/(number of edges)),
with number of edges determined by |
condor.object with condorModularityMax output
included.
r = c(1,1,1,2,2,2,3,3,3,4,4); b = c(1,2,3,1,2,4,2,3,4,3,4); reds <- c("Alice","Sue","Janine","Mary") blues <- c("Bob","John","Ed","Hank") elist <- data.frame(red=reds[r],blue=blues[b]) condor.object <- createCondorObject(elist) condor.object <- condorCluster(condor.object)r = c(1,1,1,2,2,2,3,3,3,4,4); b = c(1,2,3,1,2,4,2,3,4,3,4); reds <- c("Alice","Sue","Janine","Mary") blues <- c("Bob","John","Ed","Hank") elist <- data.frame(red=reds[r],blue=blues[b]) condor.object <- createCondorObject(elist) condor.object <- condorCluster(condor.object)
Compute one-sided KS and wilcox tests to determine if a subset of nodes has a stochastically larger qscore distribution.
condorCoreEnrich(test_nodes, q, perm = FALSE, plot.hist = FALSE, nsamp = 1000)condorCoreEnrich(test_nodes, q, perm = FALSE, plot.hist = FALSE, nsamp = 1000)
test_nodes |
is a list containing the subset of nodes (of one node class –blue or red–only) to be tested |
q |
is a two column data frame containing the node names in the first column and the q-scores in the second column. |
perm |
if TRUE, run permutation tests. Else, run
|
plot.hist |
if TRUE, produces two histograms of test statistics from permutation tests, one for KS and one for wilcoxon and a red dot for true labeling. Only works if perm=TRUE. |
nsamp |
Number of permutation tests to run |
if perm=FALSE, the analytical p-values from
ks.test and wilcox.test
if perm=TRUE, the permutation p-values are provided in
addition to the analytical values.
ks.test and wilcox.test
will throw warnings due to the presence of ties, so the p-values will be
approximate. See those functions for further details.
r = c(1,1,1,2,2,2,3,3,3,4,4); b = c(1,2,3,1,2,4,2,3,4,3,4); reds <- c("Alice","Sue","Janine","Mary") blues <- c("Bob","John","Ed","Hank") elist <- data.frame(red=reds[r],blue=blues[b]) condor.object <- createCondorObject(elist) condor.object <- condorCluster(condor.object) condor.object <- condorQscore(condor.object) q_in <- condor.object$qscores$red.qscore out <- condorCoreEnrich(c("Alice","Mary"),q=q_in,perm=TRUE,plot.hist=TRUE)r = c(1,1,1,2,2,2,3,3,3,4,4); b = c(1,2,3,1,2,4,2,3,4,3,4); reds <- c("Alice","Sue","Janine","Mary") blues <- c("Bob","John","Ed","Hank") elist <- data.frame(red=reds[r],blue=blues[b]) condor.object <- createCondorObject(elist) condor.object <- condorCluster(condor.object) condor.object <- condorQscore(condor.object) q_in <- condor.object$qscores$red.qscore out <- condorCoreEnrich(c("Alice","Mary"),q=q_in,perm=TRUE,plot.hist=TRUE)
creates condor object
condorCreateObject(elist)condorCreateObject(elist)
elist |
edge list |
condor object
This function is based on the bipartite modularity
as defined in "Modularity and community detection in bipartite networks"
by Michael J. Barber, Phys. Rev. E 76, 066102 (2007)
This function uses a slightly different implementation from the paper. It
does not use the "adaptive BRIM" method for identifying the number of
modules. Rather, it simply continues to iterate until the difference in
modularity between iterations is less that 10^-4. Starting from a random
initial condition, this could take some time. Use
condorCluster for quicker runtimes and likely better
clustering, it initializes the blue
node memberships by projecting the blue nodes into a unipartite "blue"
network and then identify communities in that network using a standard
unipartite community detection algorithm run on the projected network.
See condorCluster for more details on that.
This function loads the entire adjacency matrix in memory, so if your
network has more than ~50,000 nodes, you may want to use
condorModularityMax, which is slower, but does not store
the matrices in memory. Or, of course, you could move to a larger machine.
condorMatrixModularity( condor.object, T0 = cbind(seq_len(q), rep(1, q)), weights = 1, deltaQmin = "default" )condorMatrixModularity( condor.object, T0 = cbind(seq_len(q), rep(1, q)), weights = 1, deltaQmin = "default" )
condor.object |
is a list created by
|
T0 |
is a two column data.frame with the initial community assignment for each "blue" node, assuming there are more reds than blues, though this is not strictly necessary. The first column contains the node name, the second column the community assignment. |
weights |
edgeweights for each edge in |
deltaQmin |
convergence parameter determining the minimum required increase
in the modularity for each iteration. Default is min(10^-4,1/(number of edges)),
with number of edges determined by |
Qcoms data.frame with modularity of each community.
modularity modularity value after each iteration.
red.memb community membership of the red nodes
blue.memb community membership of the blue.nodes
r = c(1,1,1,2,2,2,3,3,3,4,4); b = c(1,2,3,1,2,4,2,3,4,3,4); reds <- c("Alice","Sue","Janine","Mary") blues <- c("Bob","John","Ed","Hank") elist <- data.frame(red=reds[r],blue=blues[b]) condor.object <- createCondorObject(elist) #randomly assign blues to their own community T0 <- data.frame(nodes=blues,coms=seq_len(4)) condor.object <- condorMatrixModularity(condor.object,T0=T0)r = c(1,1,1,2,2,2,3,3,3,4,4); b = c(1,2,3,1,2,4,2,3,4,3,4); reds <- c("Alice","Sue","Janine","Mary") blues <- c("Bob","John","Ed","Hank") elist <- data.frame(red=reds[r],blue=blues[b]) condor.object <- createCondorObject(elist) #randomly assign blues to their own community T0 <- data.frame(nodes=blues,coms=seq_len(4)) condor.object <- condorMatrixModularity(condor.object,T0=T0)
This function is based on the bipartite modularity
as defined in "Modularity and community detection in bipartite networks"
by Michael J. Barber, Phys. Rev. E 76, 066102 (2007)
This function uses a slightly different implementation from the paper. It
does not use the "adaptive BRIM" method for identifying the number of
modules. Rather, it simply continues to iterate until the difference in
modularity between iterations is less that 10^-4. Starting from a random
initial condition, this could take some time. Use
condorCluster for quicker runtimes and likely better
clustering, it initializes the blue
node memberships by projecting the blue nodes into a unipartite "blue"
network and then identify communities in that network using a standard
unipartite community detection algorithm run on the projected network.
See condorCluster for more details that.
condorModularityMax( condor.object, T0 = cbind(seq_len(q), rep(1, q)), weights = 1, deltaQmin = "default" )condorModularityMax( condor.object, T0 = cbind(seq_len(q), rep(1, q)), weights = 1, deltaQmin = "default" )
condor.object |
is a list created by
|
T0 |
is a two column data.frame with the initial community assignment for each "blue" node, assuming there are more reds than blues, though this is not strictly necessary. The first column contains the node name, the second column the community assignment. |
weights |
edgeweights for each edge in |
deltaQmin |
convergence parameter determining the minimum required increase
in the modularity for each iteration. Default is min(10^-4,1/(number of edges)),
with number of edges determined by |
Qcoms data.frame with modularity of each community.
modularity modularity value after each iteration.
red.memb community membership of the red nodes
blue.memb community membership of the blue.nodes
r = c(1,1,1,2,2,2,3,3,3,4,4); b = c(1,2,3,1,2,4,2,3,4,3,4); reds <- c("Alice","Sue","Janine","Mary") blues <- c("Bob","John","Ed","Hank") elist <- data.frame(red=reds[r],blue=blues[b]) condor.object <- createCondorObject(elist) #randomly assign blues to their own community T0 <- data.frame(nodes=blues,coms=1) condor.object <- condorModularityMax(condor.object,T0=T0)r = c(1,1,1,2,2,2,3,3,3,4,4); b = c(1,2,3,1,2,4,2,3,4,3,4); reds <- c("Alice","Sue","Janine","Mary") blues <- c("Bob","John","Ed","Hank") elist <- data.frame(red=reds[r],blue=blues[b]) condor.object <- createCondorObject(elist) #randomly assign blues to their own community T0 <- data.frame(nodes=blues,coms=1) condor.object <- condorModularityMax(condor.object,T0=T0)
This function will generate the network link 'heatmap' with colored dots representing within-community links and black dots between-community links
condorPlotCommunities( condor.object, color_list, point.size = 0.01, xlab = "SNP", ylab = "Gene" )condorPlotCommunities( condor.object, color_list, point.size = 0.01, xlab = "SNP", ylab = "Gene" )
condor.object |
output of either |
color_list |
vector of colors accepted by |
point.size |
passed to |
xlab |
x axis label |
ylab |
y axis label |
produces a plot output.
For the condor paper http://arxiv.org/abs/1509.02816, I used 35 colors from the "Tarnish" palette with "hard" clustering
http://tools.medialab.sciences-po.fr/iwanthue/ for a nice color generator at
r = c(1,1,1,2,2,2,3,3,3,4,4); b = c(1,2,3,1,2,4,2,3,4,3,4); reds <- c("Alice","Sue","Janine","Mary") blues <- c("Bob","John","Ed","Hank") elist <- data.frame(red=reds[r],blue=blues[b]) condor.object <- createCondorObject(elist) condor.object <- condorCluster(condor.object) condorPlotCommunities(condor.object, color_list=c("darkgreen","darkorange"),point.size=2, xlab="Women",ylab="Men")r = c(1,1,1,2,2,2,3,3,3,4,4); b = c(1,2,3,1,2,4,2,3,4,3,4); reds <- c("Alice","Sue","Janine","Mary") blues <- c("Bob","John","Ed","Hank") elist <- data.frame(red=reds[r],blue=blues[b]) condor.object <- createCondorObject(elist) condor.object <- condorCluster(condor.object) condorPlotCommunities(condor.object, color_list=c("darkgreen","darkorange"),point.size=2, xlab="Women",ylab="Men")
This function will generate the network link 'heatmap' for a weighted network
condorPlotHeatmap(condor.object, main = "", xlab = "blues", ylab = "reds")condorPlotHeatmap(condor.object, main = "", xlab = "blues", ylab = "reds")
condor.object |
output of either |
main |
plot title |
xlab |
x axis label |
ylab |
y axis label |
produces a plot output.
data(small1976) condor.object <- createCondorObject(small1976) condor.object <- condorCluster(condor.object, project=FALSE) condorPlotHeatmap(condor.object)data(small1976) condor.object <- createCondorObject(small1976) condor.object <- condorCluster(condor.object, project=FALSE) condorPlotHeatmap(condor.object)
Qscore is designed to calculate the fraction of the modularity contributed by each node to its community's modularity
condorQscore(condor.object)condorQscore(condor.object)
condor.object |
output of |
condor.object list has condor.object$qscores added to it.
this includes two data.frames, blue.qscore and red.qscore
which have the qscore for each red and blue node.
r = c(1,1,1,2,2,2,3,3,3,4,4); b = c(1,2,3,1,2,4,2,3,4,3,4); reds <- c("Alice","Sue","Janine","Mary") blues <- c("Bob","John","Ed","Hank") elist <- data.frame(red=reds[r],blue=blues[b]) condor.object <- createCondorObject(elist) condor.object <- condorCluster(condor.object) condor.object <- condorQscore(condor.object)r = c(1,1,1,2,2,2,3,3,3,4,4); b = c(1,2,3,1,2,4,2,3,4,3,4); reds <- c("Alice","Sue","Janine","Mary") blues <- c("Bob","John","Ed","Hank") elist <- data.frame(red=reds[r],blue=blues[b]) condor.object <- createCondorObject(elist) condor.object <- condorCluster(condor.object) condor.object <- condorQscore(condor.object)
Run CONDOR clustering
condorRun(elist, qscore = F)condorRun(elist, qscore = F)
elist |
edge list |
qscore |
TRUE = output qscore / FALSE = do not output qscore |
condor object
Pertrubs the bipartite network with fixed node strength
craneBipartite(df, alpha = 0.1, beta = 0, getAdj = F, randomStart = F)craneBipartite(df, alpha = 0.1, beta = 0, getAdj = F, randomStart = F)
df |
Adjacency Matrix or Edge list |
alpha |
alpha paramter perturbs each edge weights |
beta |
beta parameter perturbs the strength of each node. Set this to 0 if you want nodes to have node strength identical to the orignal network. |
getAdj |
TRUE = this will return adjacency matrix instead of edge list |
randomStart |
FALSE = initialize the first row with completely random edge weights. |
edge list
## Not run: # Using Edge list as input elist=craneBipartite(nonAng) elist=craneBipartite(nonAng,alpha=0.3) # Using Edge list as input and Adjcency Matrix as output adjMatrix=craneBipartite(nonAng,alpha=0.1,getAdj=T) # Using Edge list as input and Adjcency Matrix as output A=elistToAdjMat(nonAng) elist=craneBipartite(A) ## End(Not run)## Not run: # Using Edge list as input elist=craneBipartite(nonAng) elist=craneBipartite(nonAng,alpha=0.3) # Using Edge list as input and Adjcency Matrix as output adjMatrix=craneBipartite(nonAng,alpha=0.1,getAdj=T) # Using Edge list as input and Adjcency Matrix as output A=elistToAdjMat(nonAng) elist=craneBipartite(A) ## End(Not run)
Pertrubs the unipartite network with fixed node strength from adjacency matrix
craneUnipartite(A, alpha = 0.1, isSelfLoop = F)craneUnipartite(A, alpha = 0.1, isSelfLoop = F)
A |
Adjacency Matrix |
alpha |
alpha paramter perturbs each edge weights |
isSelfLoop |
TRUE/FALSE if self loop exists. co-expression matrix will have a self-loop of 1. Thus TRUE |
adjacency matrix
condor package.Converts an edge list into a list which is then an input for
other functions in the condor package.
createCondorObject(edgelist, return.gcc = TRUE)createCondorObject(edgelist, return.gcc = TRUE)
edgelist |
a data.frame with 'red' nodes in the first column and 'blue' nodes in the second column, representing links from the node in the first column to the node in the second column. There must be more unique 'red' nodes than 'blue' nodes. Optionally, a third column may be provided to create a weighted network. |
return.gcc |
if TRUE, returns the giant connected component |
G is an igraph graph object with a 'color' attribute based on the colnames of edgelist. This can be accessed via V(g)$color, which returns a vector indicating red/blue. Use V(g)$name with V(g)$color to identify red/blue node names
edges corresponding to graph G. If return.gcc=TRUE, includes only those edges in the giant connected component.
Qcoms output from condorCluster or
condorModularityMax
modularity NULL output from condorCluster
or condorModularityMax
red.memb NULL output from condorCluster
or condorModularityMax
blue.memb NULL output from condorCluster
or condorModularityMax
qscores NULL output from condorQscore
r = c(1,1,1,2,2,2,3,3,3,4,4); b = c(1,2,3,1,2,4,2,3,4,3,4); reds <- c("Alice","Sue","Janine","Mary") blues <- c("Bob","John","Ed","Hank") elist <- data.frame(red=reds[r],blue=blues[b]) condor.object <- createCondorObject(elist)r = c(1,1,1,2,2,2,3,3,3,4,4); b = c(1,2,3,1,2,4,2,3,4,3,4); reds <- c("Alice","Sue","Janine","Mary") blues <- c("Bob","John","Ed","Hank") elist <- data.frame(red=reds[r],blue=blues[b]) condor.object <- createCondorObject(elist)
This function is able to create a Cytoscape visual style for any PANDA network output.
createPandaStyle(style_name = "PandaStyle")createPandaStyle(style_name = "PandaStyle")
style_name |
Character string indicating the style name. Defaults to "PandaStyle" |
A visual style in Cytoscape Control Panel under "Style" button.
# Here we will load a customized visual style for our network, in which TF # nodes are orange circles, target gene nodes are blue squares, and edges # shade and width are the edge weight (likelyhood of regulatory interaction # between the TF and gene). You can further customize the network style # directly from Cytoscape. createPandaStyle(style_name="PandaStyle")# Here we will load a customized visual style for our network, in which TF # nodes are orange circles, target gene nodes are blue squares, and edges # shade and width are the edge weight (likelyhood of regulatory interaction # between the TF and gene). You can further customize the network style # directly from Cytoscape. createPandaStyle(style_name="PandaStyle")
Function to adjust the degree so that the hub nodes are not penalized in z-score transformation
degreeAdjust(A)degreeAdjust(A)
A |
Input adjacency matrix |
Description: Estimates a multi-omic Gaussian graphical model for two input layers of paired omic data.
dragon( layer1, layer2, pval = FALSE, gradient = "finite_difference", verbose = FALSE )dragon( layer1, layer2, pval = FALSE, gradient = "finite_difference", verbose = FALSE )
layer1 |
: first layer of omics data; rows: samples (order must match layer2), columns: variables |
layer2 |
: second layer of omics data; rows: samples (order must match layer1), columns: variables. |
pval |
: calculate p-values for network edges. Not yet implemented in R; available in netZooPy. |
gradient |
: method for estimating parameters of p-value distribution, applies only if p-val == TRUE. default = "finite_difference"; other option = "exact" |
verbose |
: verbosity level (TRUE/FALSE) |
A list of model results. cov : the shrunken covariance matrix
cov the shrunken covariance matrix
prec the shrunken precision matrix
ggm the shrunken Gaussian graphical model; matrix of partial correlations. Self-edges (diagonal elements) are set to zero.
lambdas Vector of omics-specific tuning parameters (lambda1, lambda2) for layer1 and layer2
gammas Reparameterized tuning parameters; gamma = 1 - lambda^2
risk_grid Risk grid, for assessing optimization. Grid boundaries are in terms of gamma.
Adds "_A" to first column and "_B" to second column
elistAddTags(elist)elistAddTags(elist)
elist |
edge list |
edge list
check if first two columns are identical
elistIsEdgeOrderEqual(elist1, elist2)elistIsEdgeOrderEqual(elist1, elist2)
elist1 |
edge list |
elist2 |
edge list |
boolean
undo elistAddTags
elistRemoveTags(elist)elistRemoveTags(elist)
elist |
edge list |
edge list
Sorts the edge list based on first two columns in alphabetical order
elistSort(elist)elistSort(elist)
elist |
edge list |
edge list
Converts edge list to adjacency matrix
elistToAdjMat(elist, isBipartite = F)elistToAdjMat(elist, isBipartite = F)
elist |
edge list |
isBipartite |
TRUE = for bipartite / FALSE = for unipartite |
Adjcency Matrix
A vector of gene lengths. This will be used to normalize the gene mutation scores by the gene's length. This example is based on hg19 gene symbols. The gene length is based on the number of non-overlapping exons. Data were downloaded and pre-processed as described in Kuijjer et al.
This data is a toy example data for SAMBAR, it contains length of Exons.
This data is a toy example data for SAMBAR, it contains gene annotations
data(exon.size) data(exon.size) data(genes)data(exon.size) data(exon.size) data(genes)
A integer vector of size 23459, with gene symbols as names
A list containing Exon sizes for 23459 genes
A vector containing names of 23459 genes
A list of length 1
A vector of length 23459
Kuijjer, Marieke Lydia, et al. "Cancer subtype identification using somatic mutation data." British journal of cancer 118.11 (2018): 1492-1501.
Kuijjer, Marieke Lydia, et al. "Cancer subtype identification using somatic mutation data." British journal of cancer 118.11 (2018): 1492-1501.
List of cancer-associated genes to subset the mutation data to, as described in Kuijjer et al.
data(genes)data(genes)
A character vector of length 2352
Check if data frame is an edge list
isElist(df)isElist(df)
df |
some data frame |
Boolean
CRANE Beta perturbation function. This function will add noice to the node strength sequence.
jutterDegree(nodeD, beta, beta_slope = T)jutterDegree(nodeD, beta, beta_slope = T)
nodeD |
Vector of node strength |
beta |
beta |
beta_slope |
TRUE=use predetermined slope to add noise / FALSE = use constant value for noise |
vector with new strength distribution
Compute LIONESS (Linear Interpolation to Obtain Network Estimates for Single Samples)
lioness( expr, motif = NULL, ppi = NULL, network.inference.method = "panda", ncores = 1, ... )lioness( expr, motif = NULL, ppi = NULL, network.inference.method = "panda", ncores = 1, ... )
expr |
A mandatory expression dataset, as a genes (rows) by samples (columns) data.frame |
motif |
A motif dataset, a data.frame, matrix or exprSet containing 3 columns. Each row describes an motif associated with a transcription factor (column 1) a gene (column 2) and a score (column 3) for the motif. |
ppi |
A Protein-Protein interaction dataset, a data.frame containing 3 columns. Each row describes a protein-protein interaction between transcription factor 1(column 1), transcription factor 2 (column 2) and a score (column 3) for the interaction. |
network.inference.method |
String specifying choice of network inference method. Default is "panda". Options include "pearson". |
ncores |
int specifying the number of cores to be used. Default is 1. (Note: constructing panda networks can be memory-intensive, and the number of cores should take into consideration available memory.) |
... |
additional arguments for panda analysis |
A list of length N, containing objects of class "panda"
corresponding to each of the N samples in the expression data set.
"regNet" is the regulatory network
"coregNet" is the coregulatory network
"coopNet" is the cooperative network
Kuijjer, M.L., Tung, M., Yuan, G., Quackenbush, J. and Glass, K., 2015. Estimating sample-specific regulatory networks. arXiv preprint arXiv:1505.06440. Kuijjer, M.L., Hsieh, PH., Quackenbush, J. et al. lionessR: single sample network inference in R. BMC Cancer 19, 1003 (2019). https://doi.org/10.1186/s12885-019-6235-7
data(pandaToyData) lionessRes <- lioness(expr = pandaToyData$expression[,1:3], motif = pandaToyData$motif, ppi = pandaToyData$ppi,hamming=1,progress=FALSE)data(pandaToyData) lionessRes <- lioness(expr = pandaToyData$expression[,1:3], motif = pandaToyData$motif, ppi = pandaToyData$ppi,hamming=1,progress=FALSE)
LIONESS(Linear Interpolation to Obtain Network Estimates for Single Samples) is a method to estimate sample-specific regulatory networks. [(LIONESS publication)]).
lionessPy( expr_file, motif_file = NULL, ppi_file = NULL, computing = "cpu", precision = "double", save_tmp = TRUE, modeProcess = "union", remove_missing = FALSE, start_sample = 1, end_sample = "None", save_single_network = FALSE, save_dir = "lioness_output", save_fmt = "npy" )lionessPy( expr_file, motif_file = NULL, ppi_file = NULL, computing = "cpu", precision = "double", save_tmp = TRUE, modeProcess = "union", remove_missing = FALSE, start_sample = 1, end_sample = "None", save_single_network = FALSE, save_dir = "lioness_output", save_fmt = "npy" )
expr_file |
Character string indicating the file path of expression values file, with each gene(in rows) across samples(in columns). |
motif_file |
An optional character string indicating the file path of a prior transcription factor binding motifs dataset. When this argument is not provided, analysis will continue with Pearson correlation matrix. |
ppi_file |
An optional character string indicating the file path of protein-protein interaction edge dataset.
Also, this can be generated with a list of proteins of interest by |
computing |
'cpu' uses Central Processing Unit (CPU) to run PANDA; 'gpu' use the Graphical Processing Unit (GPU) to run PANDA. The default value is "cpu". |
precision |
'double' computes the regulatory network in double precision (15 decimal digits); 'single' computes the regulatory network in single precision (7 decimal digits) which is fastaer, requires half the memory but less accurate. The default value is 'double'. |
save_tmp |
'TRUE' saves middle data like expression matrix and normalized networks; 'FALSE' deletes the middle data. The default value is 'TURE'. |
modeProcess |
'legacy' refers to the processing mode in netZooPy<=0.5, 'union': takes the union of all TFs and genes across priors and fills the missing genes in the priors with zeros; 'intersection': intersects the input genes and TFs across priors and removes the missing TFs/genes. Default values is 'union'. |
remove_missing |
Only when modeProcess='legacy': remove_missing='TRUE' removes all unmatched TF and genes; remove_missing='FALSE' keeps all tf and genes. The default value is FALSE. |
start_sample |
Numeric indicating the start sample number, The default value is 1. |
end_sample |
Numeric indicating the end sample number. The default value is 'None' meaning no end sample, i.e. print out all samples. |
save_single_network |
Boolean vector, "TRUE" wirtes out the single network in npy/txt/mat formats, directory and format are specifics by params "save_dir" and "save_fmt". The default value is 'FALSE' |
save_dir |
Character string indicating the folder name of output lioness networks for each sample by defined. The default is a folder named "lioness_output" under current working directory. This paramter is valid only when save_single_network = TRUE. |
save_fmt |
Character string indicating the format of lioness network of each sample. The dafault is "npy". The option is txt, npy, or mat. This paramter is valid only when save_single_network = TRUE. |
A data frame with columns representing each sample, rows representing the regulator-target pair in PANDA network generated by pandaPy.
Each cell filled with the related score, representing the estimated contribution of a sample to the aggregate network.
# refer to the input datasets files of control in inst/extdat as example control_expression_file_path <- system.file("extdata", "expr10_reduced.txt", package = "netZooR", mustWork = TRUE) motif_file_path <- system.file("extdata", "chip_reduced.txt", package = "netZooR", mustWork = TRUE) ppi_file_path <- system.file("extdata", "ppi_reduced.txt", package = "netZooR", mustWork = TRUE) # Run LIONESS algorithm control_lioness_result <- lionessPy(expr_file = control_expression_file_path, motif_file = motif_file_path, ppi_file = ppi_file_path, modeProcess="union",start_sample=1, end_sample=1, precision="single")# refer to the input datasets files of control in inst/extdat as example control_expression_file_path <- system.file("extdata", "expr10_reduced.txt", package = "netZooR", mustWork = TRUE) motif_file_path <- system.file("extdata", "chip_reduced.txt", package = "netZooR", mustWork = TRUE) ppi_file_path <- system.file("extdata", "ppi_reduced.txt", package = "netZooR", mustWork = TRUE) # Run LIONESS algorithm control_lioness_result <- lionessPy(expr_file = control_expression_file_path, motif_file = motif_file_path, ppi_file = ppi_file_path, modeProcess="union",start_sample=1, end_sample=1, precision="single")
This function runs the MONSTER algorithm. Biological states are characterized by distinct patterns of gene expression that reflect each phenotype's active cellular processes. Driving these phenotypes are gene regulatory networks in which transcriptions factors control when and to what degree individual genes are expressed. Phenotypic transitions, such as those that occur when disease arises from healthy tissue, are associated with changes in these networks. MONSTER is an approach to understanding these transitions. MONSTER models phenotypic-specific regulatory networks and then estimates a "transition matrix" that converts one state to another. By examining the properties of the transition matrix, we can gain insight into regulatory changes associated with phenotypic state transition. Important note: the direct regulatory network observed from gene expression is currently implemented as a regular correlation as opposed to the partial correlation described in the paper. Citation: Schlauch, Daniel, et al. "Estimating drivers of cell state transitions using gene regulatory network models." BMC systems biology 11.1 (2017): 139. https://doi.org/10.1186/s12918-017-0517-y
monster( expr, design, motif, nullPerms = 100, ni_method = "BERE", ni.coefficient.cutoff = NA, numMaxCores = 1, outputDir = NA, alphaw = 0.5, mode = "buildNet" )monster( expr, design, motif, nullPerms = 100, ni_method = "BERE", ni.coefficient.cutoff = NA, numMaxCores = 1, outputDir = NA, alphaw = 0.5, mode = "buildNet" )
expr |
Gene Expression dataset, can be matrix or data.frame of expression values or ExpressionSet. |
design |
Binary vector indicating case control partition. 1 for case and 0 for control. |
motif |
Regulatory data.frame consisting of three columns. For each row, a transcription factor (column 1) regulates a gene (column 2) with a defined strength (column 3), usually taken to be 0 or 1 |
nullPerms |
number of random permutations to run (default 100). Set to 0 to only calculate observed transition matrix. When mode is is 'buildNet' it randomly permutes the case and control expression samples, if mode is 'regNet' it will randomly permute the case and control networks. |
ni_method |
String to indicate algorithm method. Must be one of "bere","pearson","cd","lda", or "wcd". Default is "bere" |
ni.coefficient.cutoff |
numeric to specify a p-value cutoff at the network inference step. Default is NA, indicating inclusion of all coefficients. |
numMaxCores |
requires doParallel, foreach. Runs MONSTER in parallel computing environment. Set to 1 to avoid parallelization, NA will take the default parallel pool in the computer. |
outputDir |
character vector specifying a directory or path in which which to save MONSTER results, default is NA and results are not saved. |
alphaw |
A weight parameter between 0 and 1 specifying proportion of weight to give to indirect compared to direct evidence. The default is 0.5 to give an equal weight to direct and indirect evidence. |
mode |
A parameter telling whether to build the regulatory networks ('buildNet') or to use provided regulatory networks ('regNet'). If set to 'regNet', then the parameters motif, ni_method, ni.coefficient.cutoff, and alphaw will be set to NA. |
An object of class "monsterAnalysis" containing results
# Example with the network reconstruction step data(yeast) design <- c(rep(0,20),rep(NA,10),rep(1,20)) yeast$exp.cc[is.na(yeast$exp.cc)] <- mean(as.matrix(yeast$exp.cc),na.rm=TRUE) #monsterRes <- monster(yeast$exp.cc[1:500,], design, yeast$motif, nullPerms=10, numMaxCores=1) # Example with provided networks pandaResult <- panda(pandaToyData$motif, pandaToyData$expression, pandaToyData$ppi) case=getRegNet(pandaResult) nelemReg=dim(getRegNet(pandaResult))[1]*dim(getRegNet(pandaResult))[2] nGenes=length(colnames(getRegNet(pandaResult))) control=matrix(rexp(nelemReg, rate=.1), ncol=nGenes) colnames(control) = colnames(case) rownames(control) = rownames(case) expr = as.data.frame(cbind(control,case)) design=c(rep(0,nGenes),rep(1, nGenes)) monsterRes <- monster(expr, design, motif=NA, nullPerms=10, numMaxCores=1, mode='regNet')# Example with the network reconstruction step data(yeast) design <- c(rep(0,20),rep(NA,10),rep(1,20)) yeast$exp.cc[is.na(yeast$exp.cc)] <- mean(as.matrix(yeast$exp.cc),na.rm=TRUE) #monsterRes <- monster(yeast$exp.cc[1:500,], design, yeast$motif, nullPerms=10, numMaxCores=1) # Example with provided networks pandaResult <- panda(pandaToyData$motif, pandaToyData$expression, pandaToyData$ppi) case=getRegNet(pandaResult) nelemReg=dim(getRegNet(pandaResult))[1]*dim(getRegNet(pandaResult))[2] nGenes=length(colnames(getRegNet(pandaResult))) control=matrix(rexp(nelemReg, rate=.1), ncol=nGenes) colnames(control) = colnames(case) rownames(control) = rownames(case) expr = as.data.frame(cbind(control,case)) design=c(rep(0,nGenes),rep(1, nGenes)) monsterRes <- monster(expr, design, motif=NA, nullPerms=10, numMaxCores=1, mode='regNet')
This function generates a complete bipartite network from gene expression data and sequence motif data. This NI method serves as a default method for inferring bipartite networks in MONSTER. Running monsterBereFull can generate these networks independently from the larger MONSTER method.
monsterBereFull( motif.data, expr.data, alpha = 0.5, lambda = 10, score = "motifincluded" )monsterBereFull( motif.data, expr.data, alpha = 0.5, lambda = 10, score = "motifincluded" )
motif.data |
A motif dataset, a data.frame, matrix or exprSet containing 3 columns. Each row describes an motif associated with a transcription factor (column 1) a gene (column 2) and a score (column 3) for the motif. |
expr.data |
An expression dataset, as a genes (rows) by samples (columns) data.frame |
alpha |
A weight parameter specifying proportion of weight to give to indirect compared to direct evidence. See documentation. |
lambda |
if using penalized, the lambda parameter in the penalized logistic regression |
score |
String to indicate whether motif information will be readded upon completion of the algorithm |
An matrix or data.frame
data(yeast) monsterRes <- monsterBereFull(yeast$motif, yeast$exp.cc, alpha=.5)data(yeast) monsterRes <- monsterBereFull(yeast$motif, yeast$exp.cc, alpha=.5)
This function calculates the significance of an observed transition matrix given a set of null transition matrices
monsterCalculateTmPValues(monsterObj, method = "z-score")monsterCalculateTmPValues(monsterObj, method = "z-score")
monsterObj |
monsterAnalysis Object |
method |
one of 'z-score' or 'non-parametric' |
vector of p-values for each transcription factor
# data(yeast) # design <- c(rep(0,20),rep(NA,10),rep(1,20)) # yeast$exp.cc[is.na(yeast$exp.cc)] <- mean(as.matrix(yeast$exp.cc),na.rm=TRUE) # monsterRes <- monster(yeast$exp.cc, design, yeast$motif, nullPerms=100, numMaxCores=4) data(monsterRes) monsterCalculateTmPValues(monsterRes)# data(yeast) # design <- c(rep(0,20),rep(NA,10),rep(1,20)) # yeast$exp.cc[is.na(yeast$exp.cc)] <- mean(as.matrix(yeast$exp.cc),na.rm=TRUE) # monsterRes <- monster(yeast$exp.cc, design, yeast$motif, nullPerms=100, numMaxCores=4) data(monsterRes) monsterCalculateTmPValues(monsterRes)
Checks that data is something MONSTER can handle
monsterCheckDataType(expr)monsterCheckDataType(expr)
expr |
Gene Expression dataset |
expr Gene Expression dataset in the proper form (may be the same as input)
expr.matrix <- matrix(rnorm(2000),ncol=20) monsterCheckDataType(expr.matrix) #TRUE data(yeast) class(yeast$exp.cc) monsterCheckDataType(yeast$exp.cc) #TRUEexpr.matrix <- matrix(rnorm(2000),ncol=20) monsterCheckDataType(expr.matrix) #TRUE data(yeast) class(yeast$exp.cc) monsterCheckDataType(yeast$exp.cc) #TRUE
This function plots the Off diagonal mass of an observed Transition Matrix compared to a set of null TMs
monsterdTFIPlot( monsterObj, rescale = "none", plot.title = NA, highlight.tfs = NA, nTFs = -1 )monsterdTFIPlot( monsterObj, rescale = "none", plot.title = NA, highlight.tfs = NA, nTFs = -1 )
monsterObj |
monsterAnalysis Object |
rescale |
string indicating whether to reorder transcription factors according to their statistical significance and to rescale the values observed to be standardized by the null distribution ('significance'), to reorder transcription factors according to the largest dTFIs ('magnitude') with the TF x axis labels proportional to their significance , or finally without ordering them ('none'). When rescale is set to 'significance', the results can be different between two MONSTER runs if the number of permutations is not large enough to sample the null, that is why it is the seed should be set prior to calling MONSTER to get reproducible results. If rescale is set to another value such as 'magnitude' or 'none', it will produce deterministic results between two identical MONSTER runs. |
plot.title |
String specifying the plot title |
highlight.tfs |
vector specifying a set of transcription factors to highlight in the plot |
nTFs |
number of TFs to plot in x axis. -1 takes all TFs. |
ggplot2 object for transition matrix comparing observed distribution to that estimated under the null
# data(yeast) # yeast$exp.cc[is.na(yeast$exp.cc)] <- mean(as.matrix(yeast$exp.cc),na.rm=TRUE) # design <- c(rep(0,20),rep(NA,10),rep(1,20)) # monsterRes <- monster(yeast$exp.cc, design, yeast$motif, nullPerms=100, numMaxCores=4)#' data(monsterRes) monsterdTFIPlot(monsterRes)# data(yeast) # yeast$exp.cc[is.na(yeast$exp.cc)] <- mean(as.matrix(yeast$exp.cc),na.rm=TRUE) # design <- c(rep(0,20),rep(NA,10),rep(1,20)) # monsterRes <- monster(yeast$exp.cc, design, yeast$motif, nullPerms=100, numMaxCores=4)#' data(monsterRes) monsterdTFIPlot(monsterRes)
acessor for the transition matrix in MONSTER object
monsterGetTm(x)monsterGetTm(x)
x |
an object of class "monsterAnalysis" |
Transition matrix
data(monsterRes) tm <- monsterGetTm(monsterRes)data(monsterRes) tm <- monsterGetTm(monsterRes)
This function plots a hierachically clustered heatmap and corresponding dendrogram of a transaction matrix
monsterHclHeatmapPlot(monsterObj, method = "pearson")monsterHclHeatmapPlot(monsterObj, method = "pearson")
monsterObj |
monsterAnalysis Object |
method |
distance metric for hierarchical clustering. Default is "Pearson correlation" |
ggplot2 object for transition matrix heatmap
# data(yeast) # design <- c(rep(0,20),rep(NA,10),rep(1,20)) # yeast$exp.cc[is.na(yeast$exp.cc)] <- mean(as.matrix(yeast$exp.cc),na.rm=TRUE) # monsterRes <- monster(yeast$exp.cc, design, yeast$motif, nullPerms=10, numMaxCores=1) data(monsterRes) monsterHclHeatmapPlot(monsterRes)# data(yeast) # design <- c(rep(0,20),rep(NA,10),rep(1,20)) # yeast$exp.cc[is.na(yeast$exp.cc)] <- mean(as.matrix(yeast$exp.cc),na.rm=TRUE) # monsterRes <- monster(yeast$exp.cc, design, yeast$motif, nullPerms=10, numMaxCores=1) data(monsterRes) monsterHclHeatmapPlot(monsterRes)
This function generates a complete bipartite network from gene expression data and sequence motif data
monsterMonsterNI( motif.data, expr.data, verbose = FALSE, randomize = "none", method = "bere", ni.coefficient.cutoff = NA, alphaw = 1, regularization = "none", score = "motifincluded", cpp = FALSE )monsterMonsterNI( motif.data, expr.data, verbose = FALSE, randomize = "none", method = "bere", ni.coefficient.cutoff = NA, alphaw = 1, regularization = "none", score = "motifincluded", cpp = FALSE )
motif.data |
A motif dataset, a data.frame, matrix or exprSet containing 3 columns. Each row describes an motif associated with a transcription factor (column 1) a gene (column 2) and a score (column 3) for the motif. |
expr.data |
An expression dataset, as a genes (rows) by samples (columns) |
verbose |
logical to indicate printing of output for algorithm progress. |
randomize |
logical indicating randomization by genes, within genes or none |
method |
String to indicate algorithm method. Must be one of "bere","pearson","cd","lda", or "wcd". Default is "bere". Important note: the direct regulatory network observed from gene expression is currently implemented as a regular correlation as opposed to the partial correlation described in the paper (please see Schlauch et al., 2017, https://doi.org/10.1186/s12918-017-0517-y) |
ni.coefficient.cutoff |
numeric to specify a p-value cutoff at the network inference step. Default is NA, indicating inclusion of all coefficients. |
alphaw |
A weight parameter between 0 and 1 specifying proportion of weight to give to indirect compared to direct evidence. The default is 0.5 to give an equal weight to direct and indirect evidence. |
regularization |
String parameter indicating one of "none", "L1", "L2" |
score |
String to indicate whether motif information will be readded upon completion of the algorithm to give to indirect compared to direct evidence. See documentation. |
cpp |
logical use C++ for maximum speed, set to false if unable to run. |
matrix for inferred network between TFs and genes
data(yeast) cc.net <- monsterMonsterNI(yeast$motif,yeast$exp.cc)data(yeast) cc.net <- monsterMonsterNI(yeast$motif,yeast$exp.cc)
plots the sum of squares of off diagonal mass (differential TF Involvement)
monsterPlotMonsterAnalysis(x, ...)monsterPlotMonsterAnalysis(x, ...)
x |
an object of class "monsterAnalysis" |
... |
further arguments passed to or from other methods. |
Plot of the dTFI for each TF against null distribution
data(yeast) yeast$exp.cc[is.na(yeast$exp.cc)] <- mean(as.matrix(yeast$exp.cc),na.rm=TRUE) design <- c(rep(1,25),rep(0,10),rep(NA,15)) #monsterRes <- monster(yeast$exp.cc, design, #yeast$motif, nullPerms=10, numMaxCores=1) #monsterPlotMonsterAnalysis(monsterRes)data(yeast) yeast$exp.cc[is.na(yeast$exp.cc)] <- mean(as.matrix(yeast$exp.cc),na.rm=TRUE) design <- c(rep(1,25),rep(0,10),rep(NA,15)) #monsterRes <- monster(yeast$exp.cc, design, #yeast$motif, nullPerms=10, numMaxCores=1) #monsterPlotMonsterAnalysis(monsterRes)
summarizes the results of a MONSTER analysis
monsterPrintMonsterAnalysis(x, ...)monsterPrintMonsterAnalysis(x, ...)
x |
an object of class "monster" |
... |
further arguments passed to or from other methods. |
Description of transition matrices in object
data(yeast) yeast$exp.cc[is.na(yeast$exp.cc)] <- mean(as.matrix(yeast$exp.cc),na.rm=TRUE) design <- c(rep(1,25),rep(0,10),rep(NA,15)) #monster(yeast$exp.cc,design,yeast$motif, nullPerms=10, numMaxCores=1)data(yeast) yeast$exp.cc[is.na(yeast$exp.cc)] <- mean(as.matrix(yeast$exp.cc),na.rm=TRUE) design <- c(rep(1,25),rep(0,10),rep(NA,15)) #monster(yeast$exp.cc,design,yeast$motif, nullPerms=10, numMaxCores=1)
This data contains the MONSTER result from analysis of Yeast Cell cycle, included in data(yeast). This result arbitrarily takes the first 20 gene expression samples in yeast$cc to be the baseline condition, and the final 20 samples to be the final condition.
data(monsterRes)data(monsterRes)
MONSTER obj #' @references Schlauch, Daniel, et al. "Estimating drivers of cell state transitions using gene regulatory network models." BMC systems biology 11.1 (2017): 1-10.
This function analyzes a bi-partite network.
monsterTransformationMatrix( network.1, network.2, by.tfs = TRUE, standardize = FALSE, remove.diagonal = TRUE, method = "ols" )monsterTransformationMatrix( network.1, network.2, by.tfs = TRUE, standardize = FALSE, remove.diagonal = TRUE, method = "ols" )
network.1 |
starting network, a genes by transcription factors data.frame with scores for the existence of edges between |
network.2 |
final network, a genes by transcription factors data.frame with scores for the existence of edges between |
by.tfs |
logical indicating a transcription factor based transformation. If false, gives gene by gene transformation matrix |
standardize |
logical indicating whether to standardize the rows and columns |
remove.diagonal |
logical for returning a result containing 0s across the diagonal |
method |
character specifying which algorithm to use, default='ols' |
matrix object corresponding to transition matrix
data(yeast) cc.net.1 <- monsterMonsterNI(yeast$motif,yeast$exp.cc[1:1000,1:20]) cc.net.2 <- monsterMonsterNI(yeast$motif,yeast$exp.cc[1:1000,31:50]) monsterTransformationMatrix(cc.net.1, cc.net.2)data(yeast) cc.net.1 <- monsterMonsterNI(yeast$motif,yeast$exp.cc[1:1000,1:20]) cc.net.2 <- monsterMonsterNI(yeast$motif,yeast$exp.cc[1:1000,31:50]) monsterTransformationMatrix(cc.net.1, cc.net.2)
This function uses igraph to plot the transition matrix (directed graph) as a network. The edges in the network should be read as A 'positively/negatively contributes to' the targeting of B in the target state.
monsterTransitionNetworkPlot( monsterObj, numEdges = 100, numTopTFs = 10, rescale = "significance" )monsterTransitionNetworkPlot( monsterObj, numEdges = 100, numTopTFs = 10, rescale = "significance" )
monsterObj |
monsterAnalysis Object |
numEdges |
The number of edges to display |
numTopTFs |
The number of TFs to display, only when rescale='significance' |
rescale |
string to specify the order of edges. If set to 'significance', the TFs with the largest dTFI significance (smallest dTFI p-values) will be filtered first before plotting the edges with the largest magnitude in the transition matrix. Otherwise the filtering step will be skipped and the edges with the largest transitions will be plotted. The plotted graph represents the top numEdges edges between the numTopTFs if rescale=='significance' and top numEdges edges otherwise. The edge weight represents the observed transition edges standardized by the null and the node size in the graph is proportional to the p-values of the dTFIs of each TF. When rescale is set to 'significance', the results can be different between two MONSTER runs if the number of permutations is not large enough to sample the null, that is why it is the seed should be set prior to calling MONSTER to get reproducible results. If rescale is set to another value such as 'none', it will produce deterministic results between two identical MONSTER runs. |
plot the transition matrix (directed graph) as a network.
# data(yeast) # yeast$exp.cc[is.na(yeast$exp.cc)] <- mean(as.matrix(yeast$exp.cc),na.rm=TRUE) # design <- c(rep(0,20),rep(NA,10),rep(1,20)) # monsterRes <- monster(yeast$exp.cc, design, yeast$motif, nullPerms=100, numMaxCores=4)#' data(monsterRes) monsterTransitionNetworkPlot(monsterRes, rescale='significance') monsterTransitionNetworkPlot(monsterRes, rescale='none')# data(yeast) # yeast$exp.cc[is.na(yeast$exp.cc)] <- mean(as.matrix(yeast$exp.cc),na.rm=TRUE) # design <- c(rep(0,20),rep(NA,10),rep(1,20)) # monsterRes <- monster(yeast$exp.cc, design, yeast$motif, nullPerms=100, numMaxCores=4)#' data(monsterRes) monsterTransitionNetworkPlot(monsterRes, rescale='significance') monsterTransitionNetworkPlot(monsterRes, rescale='none')
This function plots the first two principal components for a transaction matrix
monsterTransitionPCAPlot( monsterObj, title = "PCA Plot of Transition", clusters = 1, alpha = 1 )monsterTransitionPCAPlot( monsterObj, title = "PCA Plot of Transition", clusters = 1, alpha = 1 )
monsterObj |
a monsterAnalysis object resulting from a monster analysis |
title |
The title of the plot |
clusters |
A vector indicating the number of clusters to compute |
alpha |
A vector indicating the level of transparency to be plotted |
ggplot2 object for transition matrix PCA
# data(yeast) # design <- c(rep(0,20),rep(NA,10),rep(1,20)) # yeast$exp.cc[is.na(yeast$exp.cc)] <- mean(as.matrix(yeast$exp.cc),na.rm=TRUE) # monsterRes <- monster(yeast$exp.cc, design, yeast$motif, nullPerms=100, numMaxCores=4)#' data(monsterRes) # Color the nodes according to cluster membership clusters <- kmeans(monsterGetTm(monsterRes),3)$cluster monsterTransitionPCAPlot(monsterRes, title="PCA Plot of Transition - Cell Cycle vs Stress Response", clusters=clusters)# data(yeast) # design <- c(rep(0,20),rep(NA,10),rep(1,20)) # yeast$exp.cc[is.na(yeast$exp.cc)] <- mean(as.matrix(yeast$exp.cc),na.rm=TRUE) # monsterRes <- monster(yeast$exp.cc, design, yeast$motif, nullPerms=100, numMaxCores=4)#' data(monsterRes) # Color the nodes according to cluster membership clusters <- kmeans(monsterGetTm(monsterRes),3)$cluster monsterTransitionPCAPlot(monsterRes, title="PCA Plot of Transition - Cell Cycle vs Stress Response", clusters=clusters)
Somatic mutations of Uterine Corpus Endometrial Carcinoma from The Cancer Genome Atlas. Data were downloaded and pre-processed as described in Kuijjer et al.
This data is a toy example data for SAMBAR, it contains gene annotations
data(mut.ucec) data(mut.ucec)data(mut.ucec) data(mut.ucec)
A table with 248 rows and 19754 columns
A binary dataframe where 1 indicates a mutation and 0 otherwise.
A table of 19754 genes by 248 samples
Kuijjer, Marieke Lydia, et al. "Cancer subtype identification using somatic mutation data." British journal of cancer 118.11 (2018): 1492-1501.
Description: OTTER infers gene regulatory networks using TF DNA binding motif (W), TF PPI (P), and gene coexpression (C) through minimzing the following objective: min f(W) with f(W) = (1-lambda)*||WW' - P||^2 + lambda*||W'W - C||^2 + (gamma/2)*||W||^2
otter(W, P, C, lambda = 0.035, gamma = 0.335, Iter = 60, eta = 1e-05, bexp = 1)otter(W, P, C, lambda = 0.035, gamma = 0.335, Iter = 60, eta = 1e-05, bexp = 1)
W |
: TF-gene regulatory network based on TF motifs as a matrix of size (t,g), g=number of genes, t=number of TFs |
P |
: TF-TF protein interaction network as a matrix of size (t,t) |
C |
: gene coexpression as a matrix of size (g,g) |
lambda |
: tuning parameter in [0,1] (higher gives more weight to C) |
gamma |
: regularization parameter |
Iter |
: number of iterations of the algorithm |
eta |
: learning rate |
bexp |
: exponent influencing learning rate (higher means smaller) Outputs: |
Inputs:
W : Predicted TF-gene complete regulatory network as an adjacency matrix of size (t,g).
W=matrix(rexp(100, rate=.1), ncol=10) C=matrix(rexp(100, rate=.1), ncol=10) P=matrix(rexp(100, rate=.1), ncol=10) # Run OTTER algorithm W <- otter(W, P, C)W=matrix(rexp(100, rate=.1), ncol=10) C=matrix(rexp(100, rate=.1), ncol=10) P=matrix(rexp(100, rate=.1), ncol=10) # Run OTTER algorithm W <- otter(W, P, C)
To determine the probability that an edge is "different" between the networks, we first subtracted the z-score weight values estimated by PANDA for the two networks and then determined the value of the inverse cumulative distribution for this difference. The product of these two probabilities represents the probability than an edge is both "supported" and "different." We select edges for which this combined probability is greater than a threshold probability (default value is 0.8).
pandaDiffEdges( panda.net1, panda.net2, threshold = 0.8, condition_name = "cond.1" )pandaDiffEdges( panda.net1, panda.net2, threshold = 0.8, condition_name = "cond.1" )
panda.net1 |
vector indicating the PANDA networks of one condition or phenotype. |
panda.net2 |
vector indicating the PANDA networks of another compared condition orphenotype. |
threshold |
numerical vector indicating a threshold probability to select select edges. |
condition_name |
string vector indicating the condition name of net1 |
a data.frame with five columns: tf, gene, motif, Score and defined condition name(the row with "T" in this column means this egde belongs to first condition or phenotype, "F" means this edge belongs to the second condition or phenotype)
# refer to four input datasets files in inst/extdat treated_expression_file_path <- system.file("extdata", "expr4_matched.txt", package = "netZooR", mustWork = TRUE) control_expression_file_path <- system.file("extdata", "expr10_matched.txt", package = "netZooR", mustWork = TRUE) motif_file_path <- system.file("extdata", "chip_matched.txt", package = "netZooR", mustWork = TRUE) ppi_file_path <- system.file("extdata", "ppi_matched.txt", package = "netZooR", mustWork = TRUE) # Run PANDA for treated and control network #treated_all_panda_result <- pandaPy(expr_file = treated_expression_file_path, #motif_file= motif_file_path, ppi_file = ppi_file_path, modeProcess="legacy", remove_missing = TRUE ) #control_all_panda_result <- pandaPy(expr_file = control_expression_file_path, #motif_file= motif_file_path, ppi_file= ppi_file_path, modeProcess="legacy", remove_missing = TRUE ) # access PANDA regulatory network #treated_net <- treated_all_panda_result$panda #control_net <- control_all_panda_result$panda #merged.panda <- pandaDiffEdges(treated_net, control_net, condition_name="treated")# refer to four input datasets files in inst/extdat treated_expression_file_path <- system.file("extdata", "expr4_matched.txt", package = "netZooR", mustWork = TRUE) control_expression_file_path <- system.file("extdata", "expr10_matched.txt", package = "netZooR", mustWork = TRUE) motif_file_path <- system.file("extdata", "chip_matched.txt", package = "netZooR", mustWork = TRUE) ppi_file_path <- system.file("extdata", "ppi_matched.txt", package = "netZooR", mustWork = TRUE) # Run PANDA for treated and control network #treated_all_panda_result <- pandaPy(expr_file = treated_expression_file_path, #motif_file= motif_file_path, ppi_file = ppi_file_path, modeProcess="legacy", remove_missing = TRUE ) #control_all_panda_result <- pandaPy(expr_file = control_expression_file_path, #motif_file= motif_file_path, ppi_file= ppi_file_path, modeProcess="legacy", remove_missing = TRUE ) # access PANDA regulatory network #treated_net <- treated_all_panda_result$panda #control_net <- control_all_panda_result$panda #merged.panda <- pandaDiffEdges(treated_net, control_net, condition_name="treated")
PANDA(Passing Attributes between Networks for Data Assimilation) is a message-passing model to reconstruct gene regulatory network, which integrates multiple sources of biological data-including protein-protein interaction data, gene expression data, and transcription factor binding motifs data to reconstruct genome-wide, condition-specific regulatory networks. [(Glass et al. 2013)]) This function is designed to run the a derived PANDA implementation in Python Library "netZooPy" netZooPy.
pandaPy( expr_file, motif_file = NULL, ppi_file = NULL, computing = "cpu", precision = "double", save_memory = FALSE, save_tmp = TRUE, keep_expression_matrix = FALSE, modeProcess = "union", remove_missing = FALSE, with_header = FALSE )pandaPy( expr_file, motif_file = NULL, ppi_file = NULL, computing = "cpu", precision = "double", save_memory = FALSE, save_tmp = TRUE, keep_expression_matrix = FALSE, modeProcess = "union", remove_missing = FALSE, with_header = FALSE )
expr_file |
Character string indicating the file path of expression values file, with each gene(in rows) across samples(in columns). |
motif_file |
An optional character string indicating the file path of a prior transcription factor binding motifs dataset. When this argument is not provided, analysis will continue with Pearson correlation matrix. |
ppi_file |
An optional character string indicating the file path of protein-protein interaction edge dataset.
Also, this can be generated with a list of proteins of interest by |
computing |
'cpu' uses Central Processing Unit (CPU) to run PANDA; 'gpu' use the Graphical Processing Unit (GPU) to run PANDA. The default value is "cpu". |
precision |
'double' computes the regulatory network in double precision (15 decimal digits); 'single' computes the regulatory network in single precision (7 decimal digits) which is fastaer, requires half the memory but less accurate. The default value is 'double'. |
save_memory |
'TRUE' removes temporary results from memory. The result network is weighted adjacency matrix of size (nTFs, nGenes); 'FALSE' keeps the temporary files in memory. The result network has 4 columns in the form gene - TF - weight in motif prior - PANDA edge. PANDA indegree/outdegree of panda network, only if save_memory = FALSE. The default value is 'FALSE'. |
save_tmp |
'TRUE' saves middle data like expression matrix and normalized networks; 'FALSE' deletes the middle data. The default value is 'TURE'. |
keep_expression_matrix |
'TRUE' keeps the input expression matrix as an attribute in the result Panda object.'FALSE' deletes the expression matrix attribute in the Panda object. The default value is 'FALSE'. |
modeProcess |
'legacy' refers to the processing mode in netZooPy<=0.5, 'union': takes the union of all TFs and genes across priors and fills the missing genes in the priors with zeros; 'intersection': intersects the input genes and TFs across priors and removes the missing TFs/genes. Default values is 'union'. |
remove_missing |
Only when modeProcess='legacy': remove_missing='TRUE' removes all unmatched TF and genes; remove_missing='FALSE' keeps all tf and genes. The default value is 'FALSE'. |
with_header |
if TRUE reads header of expression matrix |
When save_memory=FALSE(default), this function will return a list of three items:
Use $panda to access the standard output of PANDA as data frame, which consists of four columns:
"TF", "Gene", "Motif" using 0 or 1 to indicate if this edge belongs to prior motif dataset, and "Score".
Use $indegree to access the indegree of PANDA network as data frame, which consists of two columns: "Gene", "Score".
Use $outdegree to access the outdegree of PANDA network as data frame, which consists of two columns: "TF", "Score".
When save_memory=TRUE, this function will return a weigheted adjacency matirx of size (nTFs, nGenes), use $WAMpanda to access.
# take the treated TB dataset as example here. # refer to the datasets files path in inst/extdat treated_expression_file_path <- system.file("extdata", "expr4_matched.txt", package = "netZooR", mustWork = TRUE) treated_expression_file_path <- system.file("extdata", "expr4_matched.txt", package = "netZooR", mustWork = TRUE) motif_file_path <- system.file("extdata", "chip_matched.txt", package = "netZooR", mustWork = TRUE) ppi_file_path <- system.file("extdata", "ppi_matched.txt", package = "netZooR", mustWork = TRUE) # Run PANDA for treated and control network treated_all_panda_result <- pandaPy(expr_file = treated_expression_file_path, motif_file = motif_file_path, ppi_file = ppi_file_path, modeProcess="legacy", remove_missing = TRUE ) # access PANDA regulatory network treated_net <- treated_all_panda_result$panda # access PANDA regulatory indegree network. indegree_net <- treated_all_panda_result$indegree # access PANDA regulatory outdegree networks outdegree_net <- treated_all_panda_result$outdegree# take the treated TB dataset as example here. # refer to the datasets files path in inst/extdat treated_expression_file_path <- system.file("extdata", "expr4_matched.txt", package = "netZooR", mustWork = TRUE) treated_expression_file_path <- system.file("extdata", "expr4_matched.txt", package = "netZooR", mustWork = TRUE) motif_file_path <- system.file("extdata", "chip_matched.txt", package = "netZooR", mustWork = TRUE) ppi_file_path <- system.file("extdata", "ppi_matched.txt", package = "netZooR", mustWork = TRUE) # Run PANDA for treated and control network treated_all_panda_result <- pandaPy(expr_file = treated_expression_file_path, motif_file = motif_file_path, ppi_file = ppi_file_path, modeProcess="legacy", remove_missing = TRUE ) # access PANDA regulatory network treated_net <- treated_all_panda_result$panda # access PANDA regulatory indegree network. indegree_net <- treated_all_panda_result$indegree # access PANDA regulatory outdegree networks outdegree_net <- treated_all_panda_result$outdegree
ALPACA(ALtered Partitions Across Community Architectures) is a method for comparing two genome-scale networks derived from different phenotypic states to identify condition-specific modules.
[(Padi and Quackenbush 2018)])
This function compares two networks generate by pandaPy in this package and finds the sets of nodes that best characterize the change in modular structure.
pandaToAlpaca(panda.net1, panda.net2, file.stem = "./alpaca", verbose = FALSE)pandaToAlpaca(panda.net1, panda.net2, file.stem = "./alpaca", verbose = FALSE)
panda.net1 |
data.frame indicating an complete network of one condition generated by |
panda.net2 |
data.frame indicating an complete network of another condition generated by |
file.stem |
String indicating the folder path and prefix of result files, where all results will be stored. |
verbose |
Boolean vector indicating whether the full differential modularity matrix should also be written to a file. The default values is 'FALSE'. |
A string message showing the location of output file if file.stem is given, and a List where the first element is the membership vector and second element is the contribution score of each node to its module's total differential modularity
# refer to four input datasets files in inst/extdat treated_expression_file_path <- system.file("extdata", "expr4_matched.txt", package = "netZooR", mustWork = TRUE) control_expression_file_path <- system.file("extdata", "expr10_matched.txt", package = "netZooR", mustWork = TRUE) motif_file_path <- system.file("extdata", "chip_matched.txt", package = "netZooR", mustWork = TRUE) ppi_file_path <- system.file("extdata", "ppi_matched.txt", package = "netZooR", mustWork = TRUE) # Run PANDA for treated and control network treated_panda_net <- pandaPy(expr_file = treated_expression_file_path, motif_file = motif_file_path, ppi_file = ppi_file_path, modeProcess="legacy", remove_missing = TRUE )$panda control_panda_net <- pandaPy(expr_file = control_expression_file_path, motif_file = motif_file_path, ppi_file = ppi_file_path, modeProcess="legacy", remove_missing = TRUE )$panda # Run ALPACA alpaca<- pandaToAlpaca(treated_panda_net, control_panda_net, "./TB", verbose=TRUE)# refer to four input datasets files in inst/extdat treated_expression_file_path <- system.file("extdata", "expr4_matched.txt", package = "netZooR", mustWork = TRUE) control_expression_file_path <- system.file("extdata", "expr10_matched.txt", package = "netZooR", mustWork = TRUE) motif_file_path <- system.file("extdata", "chip_matched.txt", package = "netZooR", mustWork = TRUE) ppi_file_path <- system.file("extdata", "ppi_matched.txt", package = "netZooR", mustWork = TRUE) # Run PANDA for treated and control network treated_panda_net <- pandaPy(expr_file = treated_expression_file_path, motif_file = motif_file_path, ppi_file = ppi_file_path, modeProcess="legacy", remove_missing = TRUE )$panda control_panda_net <- pandaPy(expr_file = control_expression_file_path, motif_file = motif_file_path, ppi_file = ppi_file_path, modeProcess="legacy", remove_missing = TRUE )$panda # Run ALPACA alpaca<- pandaToAlpaca(treated_panda_net, control_panda_net, "./TB", verbose=TRUE)
CONDOR (COmplex Network Description Of Regulators) implements methods for clustering biapartite networks and estimatiing the contribution of each node to its community's modularity, [(Platig et al. 2016)]) This function uses the result of PANDA algorithm as the input dataset to run CONDOR algorithm. More about condor package and usage.
pandaToCondorObject(panda.net, threshold)pandaToCondorObject(panda.net, threshold)
panda.net |
Data Frame indicating the result of PANDA regulatory network, created by |
threshold |
Numeric vector of the customered threshold to select edges. Default value is the the midpoint between the median edge-weight of prior ( 3rd column "Motif" is 1.0) edges and the median edge-weight of non-prior edges (3rd column "Motif" is 0.0) in PANDA network. and the median edge-weight of non-prior edges (3rd column "Motif" is 0.0) in PANDA network. |
a CONDOR object, see createCondorObject.
# refer to three input datasets files in inst/extdat treated_expression_file_path <- system.file("extdata", "expr4_matched.txt", package = "netZooR", mustWork = TRUE) motif_file_path <- system.file("extdata", "chip_matched.txt", package = "netZooR", mustWork = TRUE) ppi_file_path <- system.file("extdata", "ppi_matched.txt", package = "netZooR", mustWork = TRUE) # Run PANDA to construct the treated network treated_all_panda_result <- pandaPy(expr_file = treated_expression_file_path, motif_file= motif_file_path, ppi_file = ppi_file_path, modeProcess="legacy", remove_missing = TRUE ) # access PANDA regulatory network treated_net <- treated_all_panda_result$panda # Obtain the condor.object from PANDA network treated_condor_object <- pandaToCondorObject(treated_net, threshold = 0) # cluster condor.object treated_condor_object <- condorCluster(treated_condor_object, project = FALSE) # package igraph and package viridisLite are already loaded with this package. library(viridisLite) treated_color_num <- max(treated_condor_object$red.memb$com) treated_color <- viridis(treated_color_num, alpha = 1, begin = 0, end = 1, direction = 1, option = "D") condorPlotCommunities(treated_condor_object, color_list=treated_color, point.size=0.04, xlab="Target", ylab="Regulator")# refer to three input datasets files in inst/extdat treated_expression_file_path <- system.file("extdata", "expr4_matched.txt", package = "netZooR", mustWork = TRUE) motif_file_path <- system.file("extdata", "chip_matched.txt", package = "netZooR", mustWork = TRUE) ppi_file_path <- system.file("extdata", "ppi_matched.txt", package = "netZooR", mustWork = TRUE) # Run PANDA to construct the treated network treated_all_panda_result <- pandaPy(expr_file = treated_expression_file_path, motif_file= motif_file_path, ppi_file = ppi_file_path, modeProcess="legacy", remove_missing = TRUE ) # access PANDA regulatory network treated_net <- treated_all_panda_result$panda # Obtain the condor.object from PANDA network treated_condor_object <- pandaToCondorObject(treated_net, threshold = 0) # cluster condor.object treated_condor_object <- condorCluster(treated_condor_object, project = FALSE) # package igraph and package viridisLite are already loaded with this package. library(viridisLite) treated_color_num <- max(treated_condor_object$red.memb$com) treated_color <- viridis(treated_color_num, alpha = 1, begin = 0, end = 1, direction = 1, option = "D") condorPlotCommunities(treated_condor_object, color_list=treated_color, point.size=0.04, xlab="Target", ylab="Regulator")
Description: NOTE: Beta version. EGRET infers individual-specific gene regulatory networks using inidividual level data - a genotype vcf file (v) and QBiC binding predictions (q) - as well as population/reference level data - eQTLs (b), a motif-gene prior (m), PPI network (p), and gene expression (e). An annotation file g is also used to map TF names to their corresponding ensemble ids.
runEgret(b, v, q, m, e, p, g, t)runEgret(b, v, q, m, e, p, g, t)
b |
: Data frame of eQTL data, each row containing an eQTL which exist within motif regions adjacent to the eGene, with columns TF, gene, variant position,variant chromosome, eQTL beta value. |
v |
: Data frame of VCF file containing SNPs of the individual in question |
q |
: Data frame of QBiC predictions of the effect of eQTL variants on TF binding. Each row represents an eQTL variant with a predicted negative (disruptive) effect on the binding of the TF corresponding to the motif in which the eQTL variant resides. Colums are: eQTL variant as chr[chrNum]_position, TF, adjacent eGene, QBiC binding effect size and QBiC binding effect (should be negative) |
m |
: Motif prior data frame. Each row represents an edge in the bipartite motif prior, with columns TF, gene and edge weight. The edge weight should be 1 or 0 based on the presence/absence of the TF motif in the promoter region of the gene. |
e |
: Gene expression data frame in which each row represents a gene and each column represents the expression of that gene in a sample. The first column should contain gene IDs. |
p |
: PPI network data frame. Each row represents an edgem with columns TF, TF and interaction weight. |
g |
: Data frame mapping gene names to gene ids, with columns containing the gene ID the corresponding gene name. |
t |
: A string containing a name for the EGRET run. Output files will be labelled with this tag. Outputs: |
Inputs:
EGRET : Predicted genotye-specific gene regulatory network saved as tag_egret.RData
BASELINE : A Baseline (PANDA) genotype-agnostic gene regulatory network saved as tag_panda.RData
# Run EGRET algorithm toy_qbic_path <- system.file("extdata", "toy_qbic.txt", package = "netZooR", mustWork = TRUE) toy_genotype_path <- system.file("extdata", "toy_genotype.vcf", package = "netZooR", mustWork = TRUE) toy_motif_path <- system.file("extdata", "toy_motif_prior.txt", package = "netZooR", mustWork = TRUE) toy_expr_path <- system.file("extdata", "toy_expr.txt", package = "netZooR", mustWork = TRUE) toy_ppi_path <- system.file("extdata", "toy_ppi_prior.txt", package = "netZooR", mustWork = TRUE) toy_eqtl_path <- system.file("extdata", "toy_eQTL.txt", package = "netZooR", mustWork = TRUE) toy_map_path <- system.file("extdata", "toy_map.txt", package = "netZooR", mustWork = TRUE) qbic <- read.table(file = toy_qbic_path, header = FALSE) vcf <- read.table(toy_genotype_path, header = FALSE, sep = "\t", stringsAsFactors = FALSE, colClasses = c("character", "numeric", "character", "character", "character", "character", "character", "character", "character", "character")) motif <- read.table(toy_motif_path, sep = "\t", header = FALSE) expr <- read.table(toy_expr_path, header = FALSE, sep = "\t", row.names = 1) ppi <- read.table(toy_ppi_path, header = FALSE, sep = "\t") qtl <- read.table(toy_eqtl_path, header = FALSE) nameGeneMap <- read.table(toy_map_path, header = FALSE) tag <- "my_toy_egret_run" runEgret(qtl,vcf,qbic,motif,expr,ppi,nameGeneMap,tag)# Run EGRET algorithm toy_qbic_path <- system.file("extdata", "toy_qbic.txt", package = "netZooR", mustWork = TRUE) toy_genotype_path <- system.file("extdata", "toy_genotype.vcf", package = "netZooR", mustWork = TRUE) toy_motif_path <- system.file("extdata", "toy_motif_prior.txt", package = "netZooR", mustWork = TRUE) toy_expr_path <- system.file("extdata", "toy_expr.txt", package = "netZooR", mustWork = TRUE) toy_ppi_path <- system.file("extdata", "toy_ppi_prior.txt", package = "netZooR", mustWork = TRUE) toy_eqtl_path <- system.file("extdata", "toy_eQTL.txt", package = "netZooR", mustWork = TRUE) toy_map_path <- system.file("extdata", "toy_map.txt", package = "netZooR", mustWork = TRUE) qbic <- read.table(file = toy_qbic_path, header = FALSE) vcf <- read.table(toy_genotype_path, header = FALSE, sep = "\t", stringsAsFactors = FALSE, colClasses = c("character", "numeric", "character", "character", "character", "character", "character", "character", "character", "character")) motif <- read.table(toy_motif_path, sep = "\t", header = FALSE) expr <- read.table(toy_expr_path, header = FALSE, sep = "\t", row.names = 1) ppi <- read.table(toy_ppi_path, header = FALSE, sep = "\t") qtl <- read.table(toy_eqtl_path, header = FALSE) nameGeneMap <- read.table(toy_map_path, header = FALSE) tag <- "my_toy_egret_run" runEgret(qtl,vcf,qbic,motif,expr,ppi,nameGeneMap,tag)
Main SAMBAR function.
sambar( mutdata = mut.ucec, esize = exon.size, signatureset = system.file("extdata", "h.all.v6.1.symbols.gmt", package = "netZooR", mustWork = TRUE), cangenes = genes, kmin = 2, kmax = 4 )sambar( mutdata = mut.ucec, esize = exon.size, signatureset = system.file("extdata", "h.all.v6.1.symbols.gmt", package = "netZooR", mustWork = TRUE), cangenes = genes, kmin = 2, kmax = 4 )
mutdata |
Mutation data in matrix format. The number of mutations should be listed for samples (rows) and genes (columns). |
esize |
A integer vector of gene lengths, with gene symbols as names. |
signatureset |
A file containing gene sets (signatures) in .gmt format. These gene sets will be used to de-sparsify the gene-level mutation scores. |
cangenes |
A vector of genes, for example of cancer-associated genes. This will be used to subset the gene-level mutation data to. |
kmin |
The minimum number of subtypes the user wants to assess. Defaults to 2. |
kmax |
The maximum number of subtypes the user wants to assess. Defaults to 4. |
A list of samples and the subtypes to which these samples are assigned, for each k.
data("exon.size") data("mut.ucec") data("genes") sambar(mutdata=mut.ucec, esize=exon.size, signatureset=system.file("extdata", "h.all.v6.1.symbols.gmt", package="netZooR", mustWork=TRUE), cangenes=genes, kmin=2, kmax=4)data("exon.size") data("mut.ucec") data("genes") sambar(mutdata=mut.ucec, esize=exon.size, signatureset=system.file("extdata", "h.all.v6.1.symbols.gmt", package="netZooR", mustWork=TRUE), cangenes=genes, kmin=2, kmax=4)
Convert .gmt files into a binary matrix.
sambarConvertgmt(signature, cagenes)sambarConvertgmt(signature, cagenes)
signature |
A file containing gene sets (signatures) in .gmt format. These gene sets will be used to de-sparsify the gene-level mutation scores. |
cagenes |
A vector of genes, for example of cancer-associated genes. This will be used to subset the gene-level mutation data to. |
A matrix containing gene set mutation scores.
Normalize gene mutation scores by gene length.
sambarCorgenelength(x, cagenes, exonsize)sambarCorgenelength(x, cagenes, exonsize)
x |
Mutation data, in the format of a matrix, including the number of mutations for samples (rows) and genes (columns). |
cagenes |
A vector of genes, for example of cancer-associated genes. This will be used to subset the gene-level mutation data to. |
exonsize |
A vector of gene lengths. This will be used to normalize the gene mutation scores. |
Mutation rate-adjusted gene mutation scores.
De-sparsify gene-level mutation scores into gene set-level mutation scores.
sambarDesparsify(edgx, mutratecorx)sambarDesparsify(edgx, mutratecorx)
edgx |
A binary matrix containing information on which genes belong to which gene sets. Output from the sambarConvertgmt function. |
mutratecorx |
Gene-level mutation scores corrected for the number of gene sets each gene belongs to (from sambar function). |
De-sparsified mutation data.
A dataset containing the number of interactions 34 plants and 13 pollinators. The variables are as follows:
data(small1976)data(small1976)
A data frame with 442 rows and 3 variables
pollinator. Species name of insect pollinator
plant. Species name of plant
interactions. Number of visitors caught on each plant species
https://www.nceas.ucsb.edu/interactionweb/html/small_1976.html
This function uses a list of Transcription Factors (TF) of interest to source the Protein-Protein interactions (PPI) from STRING database using all types of interactions not only the physical subnetwork Important: this function produces a simple unweighted network for tutorial purposes, and does not support weighted PPI edges for the moment. For more complex PPI network modeling, consider pulling the PPI network directly from STRINGdb directly or through their R package.
sourcePPI(TF, STRING.version = "10", species.index, ...)sourcePPI(TF, STRING.version = "10", species.index, ...)
TF |
a data frame with one column indicating the TF of interest |
STRING.version |
a numeric vector indicating the STRING version. Default valuve is 10 |
species.index |
a numeric vector indicating NCBI taxonomy identifiers |
... |
any dditional arguments passed to |
A PPI data.frame which contains three columns: "from" and "to" indicating the direction of protein-protein interaction, and "score" indicating the interaction score between two proteins.
# the example motif file motif_file_path <- system.file("extdata", "chip_matched.txt", package = "netZooR", mustWork = TRUE) motif <- read.table(motif_file_path, sep="\t") # create a TF data frame with one column TF <-data.frame(motif[,1]) # create PPI data frame by searching in STRING version 10 # and specifying specie to "Mycobacterium tuberculosis H37Rv". # STRING verison 11 is only accessible to R 4.0. if(R.Version()$major=="3"){PPI <- sourcePPI(TF, STRING.version="10", species.index=83332, score_threshold=0)} if(R.Version()$major=="4"){PPI <- sourcePPI(TF, STRING.version="11", species.index=83332, score_threshold=0)} # write out locally then can be used in \code{\link{pandaPy}}.# the example motif file motif_file_path <- system.file("extdata", "chip_matched.txt", package = "netZooR", mustWork = TRUE) motif <- read.table(motif_file_path, sep="\t") # create a TF data frame with one column TF <-data.frame(motif[,1]) # create PPI data frame by searching in STRING version 10 # and specifying specie to "Mycobacterium tuberculosis H37Rv". # STRING verison 11 is only accessible to R 4.0. if(R.Version()$major=="3"){PPI <- sourcePPI(TF, STRING.version="10", species.index=83332, score_threshold=0)} if(R.Version()$major=="4"){PPI <- sourcePPI(TF, STRING.version="11", species.index=83332, score_threshold=0)} # write out locally then can be used in \code{\link{pandaPy}}.
This function runs the SPIDER algorithm
spider( motif, expr = NULL, epifilter = NULL, ppi = NULL, alpha = 0.1, hamming = 0.001, iter = NA, output = c("regulatory", "coexpression", "cooperative"), zScale = TRUE, progress = FALSE, randomize = c("None", "within.gene", "by.gene"), cor.method = "pearson", scale.by.present = FALSE, edgelist = FALSE, remove.missing.ppi = FALSE, remove.missing.motif = FALSE, remove.missing.genes = FALSE, mode = "union" )spider( motif, expr = NULL, epifilter = NULL, ppi = NULL, alpha = 0.1, hamming = 0.001, iter = NA, output = c("regulatory", "coexpression", "cooperative"), zScale = TRUE, progress = FALSE, randomize = c("None", "within.gene", "by.gene"), cor.method = "pearson", scale.by.present = FALSE, edgelist = FALSE, remove.missing.ppi = FALSE, remove.missing.motif = FALSE, remove.missing.genes = FALSE, mode = "union" )
motif |
A motif dataset, a data.frame, matrix or exprSet containing 3 columns. Each row describes an motif associated with a transcription factor (column 1) a gene (column 2) and a score (column 3) for the motif. |
expr |
An expression dataset, as a genes (rows) by samples (columns) data.frame |
epifilter |
A binary matrix that is of the same size as motif that will be used as a mask to filter motif for open chromatin region. Motif interactions that fall in open chromatin region will be kept and the others are removed. |
ppi |
A Protein-Protein interaction dataset, a data.frame containing 3 columns. Each row describes a protein-protein interaction between transcription factor 1(column 1), transcription factor 2 (column 2) and a score (column 3) for the interaction. |
alpha |
value to be used for update variable, alpha (default=0.1) |
hamming |
value at which to terminate the process based on hamming distance (default 10^-3) |
iter |
sets the maximum number of iterations SPIDER can run before exiting. |
output |
a vector containing which networks to return. Options include "regulatory", "coregulatory", "cooperative". |
zScale |
Boolean to indicate use of z-scores in output. False will use [0,1] scale. |
progress |
Boolean to indicate printing of output for algorithm progress. |
randomize |
method by which to randomize gene expression matrix. Default "None". Must be one of "None", "within.gene", "by.genes". "within.gene" randomization scrambles each row of the gene expression matrix, "by.gene" scrambles gene labels. |
cor.method |
Correlation method, default is "pearson". |
scale.by.present |
Boolean to indicate scaling of correlations by percentage of positive samples. |
edgelist |
Boolean to indicate if edge lists instead of matrices should be returned. |
remove.missing.ppi |
Boolean to indicate whether TFs in the PPI but not in the motif data should be removed. Only when mode=='legacy'. |
remove.missing.motif |
Boolean to indicate whether genes targeted in the motif data but not the expression data should be removed. Only when mode=='legacy'. |
remove.missing.genes |
Boolean to indicate whether genes in the expression data but lacking information from the motif prior should be removed. Only when mode=='legacy'. |
mode |
The data alignment mode. The mode 'union' takes the union of the genes in the expression matrix and the motif and the union of TFs in the ppi and motif and fills the matrics with zeros for nonintersecting TFs and gens, 'intersection' takes the intersection of genes and TFs and removes nonintersecting sets, 'legacy' is the old behavior with PANDAR version 1.19.3. #' Parameters remove.missing.ppi, remove.missingmotif, remove.missing.genes work only with mode=='legacy'. |
An object of class "panda" containing matrices describing networks achieved by convergence
with SPIDER algorithm.
"regNet" is the regulatory network
"coregNet" is the coregulatory network
"coopNet" is the cooperative network
Sonawane, Abhijeet Rajendra, et al. "Constructing gene regulatory networks using epigenetic data." npj Systems Biology and Applications 7.1 (2021): 1-13.
data(pandaToyData) pandaToyData$epifilter = pandaToyData$motif nind=floor(runif(5000, min=1, max=dim(pandaToyData$epifilter)[1])) pandaToyData$epifilter[nind,3] = 0 #spiderRes <- spider(pandaToyData$motif,pandaToyData$expression, # pandaToyData$epifilter,pandaToyData$ppi,hamming=.1,progress=TRUE)data(pandaToyData) pandaToyData$epifilter = pandaToyData$motif nind=floor(runif(5000, min=1, max=dim(pandaToyData$epifilter)[1])) pandaToyData$epifilter[nind,3] = 0 #spiderRes <- spider(pandaToyData$motif,pandaToyData$expression, # pandaToyData$epifilter,pandaToyData$ppi,hamming=.1,progress=TRUE)
This function is able to modify PANDA network and plot in Cytoscape. Please make sure that Cytoscape is installed and open it before calling this function.
visPandaInCytoscape(panda.net, network_name = "PANDA")visPandaInCytoscape(panda.net, network_name = "PANDA")
panda.net |
Character string indicating the input PANDA network in data frame structure type. |
network_name |
Character string indicating the name of Cytoscape network. |
PANDA network in Cytoscape
# refer to the input datasets files of control TB dataset in inst/extdat as example control_expression_file_path <- system.file("extdata", "expr10_matched.txt", package = "netZooR", mustWork = TRUE) motif_file_path <- system.file("extdata", "chip_matched.txt", package = "netZooR", mustWork = TRUE) ppi_file_path <- system.file("extdata", "ppi_matched.txt", package = "netZooR", mustWork = TRUE) # Run PANDA algorithm control_all_panda_result <- panda.py(expr = control_expression_file_path, motif = motif_file_path, ppi = ppi_file_path, mode_process="legacy", rm_missing = TRUE ) # access PANDA regulatory network control_net <- control_all_panda_result$panda # select top 1000 edges in PANDA network by edge weight. panda.net <- head(control_net[order(control_net$force,decreasing = TRUE),], 1000) # run this function to create a network in Cytoscape. visPandaInCytoscape(panda.net, network.name="PANDA")# refer to the input datasets files of control TB dataset in inst/extdat as example control_expression_file_path <- system.file("extdata", "expr10_matched.txt", package = "netZooR", mustWork = TRUE) motif_file_path <- system.file("extdata", "chip_matched.txt", package = "netZooR", mustWork = TRUE) ppi_file_path <- system.file("extdata", "ppi_matched.txt", package = "netZooR", mustWork = TRUE) # Run PANDA algorithm control_all_panda_result <- panda.py(expr = control_expression_file_path, motif = motif_file_path, ppi = ppi_file_path, mode_process="legacy", rm_missing = TRUE ) # access PANDA regulatory network control_net <- control_all_panda_result$panda # select top 1000 edges in PANDA network by edge weight. panda.net <- head(control_net[order(control_net$force,decreasing = TRUE),], 1000) # run this function to create a network in Cytoscape. visPandaInCytoscape(panda.net, network.name="PANDA")
This data is a list containing gene expression data from three separate yeast studies along with data mapping yeast transcription factors with genes based on the presence of a sequence binding motif for each transcription factor in the vicinity of each gene. The motif data.frame, yeast$motif, describes a set of pairwise connections where a specific known sequence motif of a transcription factor was found upstream of the corresponding gene. The expression data, yeast$exp.ko, yeast$exp.cc, and yeast$exp.sr, are three gene expression datasets measured in conditions of gene knockout, cell cycle, and stress response, respectively.
data(yeast)data(yeast)
A list containing 4 data.frames
A list of length 4
Glass K, Huttenhower C, Quackenbush J, Yuan GC. Passing Messages Between Biological Networks to Refine Predicted Interactions. PLoS One. 2013 May 31;8(5):e64832.