---
title: "methylKit: User Guide v`r packageVersion('methylKit')`"
author: "Altuna Akalin^[Author of the vignette. See [Acknowledgements](#acknowledgements) for a list of contributors.] 

altuna.akalin@mdc-berlin.de"
date: "`r Sys.Date()`"
output: 
      html_document:
        toc: true
        toc_float: true
        number_sections: true
        toc_depth: 2

      
bibliography: Vignette_methylKit.bib
vignette: >
  %\VignetteIndexEntry{methylKit: User Guide v`r packageVersion('methylKit')`}
  %\VignetteEngine{knitr::rmarkdown}
  %\VignetteEncoding{UTF-8}
---

```{r setup, include=FALSE}
knitr::opts_chunk$set(dpi = 75)
knitr::opts_chunk$set(cache = FALSE)
```

```{r ,eval=TRUE,echo=FALSE,warning=FALSE,message=FALSE}
#devtools::load_all(".")
```

# Introduction

In this manual, we will show how to use the methylKit package. methylKit is an 
R package for analysis and annotation of DNA methylation information obtained 
by high-throughput bisulfite sequencing. The package is designed to deal with 
sequencing data from RRBS and its variants. But, it can potentially handle 
whole-genome bisulfite sequencing data if proper input format is provided. 

## DNA methylation

DNA methylation in vertebrates typically occurs at CpG dinucleotides, however
non-CpG Cs are also methylated in certain tissues such as embryonic stem cells.
DNA methylation can act as an epigenetic control mechanism for gene regulation.
Methylation can hinder binding of transcription factors and/or methylated bases
can be bound by methyl-binding-domain proteins which can recruit chromatin
remodeling factors. In both cases, the transcription of the regulated gene will
be effected. In addition, aberrant DNA methylation patterns have been associated
with many human malignancies and can be used in a predictive manner. In
malignant tissues, DNA is either hypo-methylated or hyper-methylated compared to
the normal tissue. The location of hyper- and hypo-methylated sites gives a
distinct signature to many diseases. Traditionally, hypo-methylation is
associated with gene transcription (if it is on a regulatory region such as
promoters) and hyper-methylation is associated with gene repression.

## High-throughput bisulfite sequencing

Bisulfite sequencing is a technique that can determine DNA methylation 
patterns. The major difference from regular sequencing experiments is that, in 
bisulfite sequencing DNA is treated with bisulfite which converts cytosine 
residues to uracil, but leaves 5-methylcytosine residues unaffected. By 
sequencing and aligning those converted DNA fragments it is possible to call 
methylation status of a base. Usually, the methylation status of a base 
determined by a high-throughput bisulfite sequencing will not be a binary 
score, but it will be a percentage. The percentage simply determines how many 
of the bases that are aligning to a given cytosine location in the genome have 
actual C bases in the reads. Since bisulfite treatment leaves methylated Cs 
intact, that percentage will give us percent methylation score on that base. 
The reasons why we will not get a binary response are:

*  the probable sequencing errors in high-throughput sequencing experiments 
*  incomplete bisulfite conversion 
*  (and a more likely scenario) is heterogeneity of samples and heterogeneity of
paired chromosomes from the same sample

# Basics

## Reading the methylation call files

We start by reading in the methylation call data from bisulfite sequencing with
`methRead` function. Reading in the data this way will return a `methylRawList`
object which stores methylation information per sample for each covered base. By
default `methRead` requires a minimum coverage of 10 reads per base to ensure
good quality of the data and a high confidence methylation percentage.

The methylation call files are basically text files that contain percent
methylation score per base. Such input files may be obtained from 
[AMP pipeline](http://code.google.com/p/amp-errbs/)
developed for aligning RRBS reads or from `processBismarkAln` function.
However, "cytosineReport" and "coverage" files from 
[Bismark aligner](http://www.bioinformatics.bbsrc.ac.uk/projects/bismark/) can
be read in to methylKit as well.

A typical methylation call file looks like this:

```{r, eval=TRUE, echo=FALSE}
tab <- read.table( system.file("extdata", "test1.myCpG.txt", package = "methylKit"),
                   header=TRUE, nrows=5)
tab
#knitr::kable(tab)
```

Most of the time bisulfite sequencing experiments have test and control 
samples. The test samples can be from a disease tissue while the control 
samples can be from a healthy tissue. You can read a set of methylation call 
files that have test/control conditions giving `treatment` vector option. For 
sake of subsequent analysis, file.list, sample.id and treatment option should 
have the same order. In the following example, first two files have the 
sample ids "test1" and "test2" and as determined by treatment vector they 
belong to the same group. The third and fourth files have sample ids "ctrl1" 
and "ctrl2" and they belong to the same group as indicated by the treatment 
vector.


```{r,message=FALSE}
library(methylKit)
file.list=list( system.file("extdata", 
                            "test1.myCpG.txt", package = "methylKit"),
                system.file("extdata",
                            "test2.myCpG.txt", package = "methylKit"),
                system.file("extdata", 
                            "control1.myCpG.txt", package = "methylKit"),
                system.file("extdata", 
                            "control2.myCpG.txt", package = "methylKit") )


# read the files to a methylRawList object: myobj
myobj=methRead(file.list,
           sample.id=list("test1","test2","ctrl1","ctrl2"),
           assembly="hg18",
           treatment=c(1,1,0,0),
           context="CpG",
           mincov = 10
           )
```

In addition to the options we mentioned above, any tab separated text file with
a generic format can be read in using methylKit, such as methylation ratio files
from [BSMAP](http://code.google.com/p/bsmap/). See
[here](http://zvfak.blogspot.com/2012/10/how-to-read-bsmap-methylation-ratio.html)
for an example.

##  Reading the methylation call files and store them as flat file database

Sometimes, when dealing with multiple samples and increased sample sizes coming
from genome wide bisulfite sequencing experiments, the memory of your  computer
might not be sufficient enough.

Therefore methylKit offers a new group of classes, that are basically pendants 
to the original methylKit classes with one important difference: The 
methylation information, which normally is internally stored as data.frame, is 
stored in an external bgzipped file and is indexed by tabix [@Li2011], to 
enable fast retrieval of records or regions. This group contains 
`methylRawListDB`, `methylRawDB`, `methylBaseDB` and `methylDiffDB`, let us 
call them  **methylDB** objects.

We can now create a `methylRawListDB` object, which stores the same content as
*myobj* from above. But the single `methylRaw` objects retrieve their data from
the tabix-file linked under `dbpath`.

```{r, message=FALSE,warning=FALSE}
library(methylKit)
file.list=list( system.file("extdata", "test1.myCpG.txt", package = "methylKit"),
                system.file("extdata", "test2.myCpG.txt", package = "methylKit"),
                system.file("extdata", "control1.myCpG.txt", package = "methylKit"),
                system.file("extdata", "control2.myCpG.txt", package = "methylKit") )


# read the files to a methylRawListDB object: myobjDB 
# and save in databases in folder methylDB
myobjDB=methRead(file.list,
           sample.id=list("test1","test2","ctrl1","ctrl2"),
           assembly="hg18",
           treatment=c(1,1,0,0),
           context="CpG",
           dbtype = "tabix",
           dbdir = "methylDB"
           )

print(myobjDB[[1]]@dbpath)


```

Most if not all functions in this package will work with methylDB objects the 
same way as it does with normal methylKit objects. 
Functions that return methylKit objects, will return a methylDB object if 
provided, 
but there are a few exceptions such as the `select`, the `[` and the 
`selectByOverlap` functions.



## Reading the methylation calls from sorted  Bismark alignments

Alternatively, methylation percentage calls can be calculated from
sorted SAM or BAM file(s) from Bismark aligner and read-in to the memory. 
Bismark is a
popular aligner for bisulfite sequencing reads, available 
[here](http://www.bioinformatics.bbsrc.ac.uk/projects/bismark/) [@Krueger2011]. 
`processBismarkAln` function is designed to read-in Bismark SAM/BAM files as 
`methylRaw` or `methylRawList` objects which store per base methylation calls. 
SAM files must be sorted by chromosome and read position columns, using 'sort' 
command in unix-like machines will accomplish such a sort easily. BAM files 
should be sorted and indexed. This
could be achieved with samtools (http://www.htslib.org/doc/samtools.html).

The following command reads a sorted SAM file and creates a `methylRaw` object
for CpG methylation. The user has the option to save the methylation call files
to a folder given by `save.folder` option. The saved files can be read-in using
the `methRead` function when needed.

```{r, eval=FALSE}
my.methRaw=processBismarkAln( location = 
                                system.file("extdata",
                                                "test.fastq_bismark.sorted.min.sam", 
	                                              package = "methylKit"),
                         sample.id="test1", assembly="hg18", 
                         read.context="CpG", save.folder=getwd())
```


It is also possible to read multiple SAM files at the same time, 
check `processBismarkAln` documentation.

## Descriptive statistics on samples

Since we read the methylation data now, we can check the basic stats about the
methylation data such as coverage and percent  methylation. We now have a
`methylRawList` object which contains methylation information per sample. The
following command prints out percent methylation statistics for second sample:
"test2"

```{r}
getMethylationStats(myobj[[2]],plot=FALSE,both.strands=FALSE)
```

The following command plots the histogram for percent methylation
distribution.The figure below is the histogram and numbers on bars denote what
percentage of locations are contained in that bin. Typically, percent
methylation histogram should have two peaks on both ends. In any given cell, any
given base are either methylated or not. Therefore, looking at many cells should
yield a similar pattern where we see lots of locations with high methylation and
lots of locations with low methylation.

```{r} 
getMethylationStats(myobj[[2]],plot=TRUE,both.strands=FALSE)
```

We can also plot the read coverage per base information in a similar way, again
numbers on bars denote what percentage of locations are contained in that bin.
Experiments that are highly suffering from PCR duplication bias will have a
secondary peak towards the right hand side of the histogram.

```{r}
getCoverageStats(myobj[[2]],plot=TRUE,both.strands=FALSE)
```

## Filtering samples based on read coverage

It might be useful to filter samples based on coverage. Particularly, if our
samples are suffering from PCR bias it would be useful to discard bases with
very high read coverage. Furthermore, we would also like to discard bases that
have low read coverage, a high enough read coverage will increase the power of
the statistical tests. The code below filters a `methylRawList` and discards
bases that have coverage below 10X and also discards the bases that have more
than 99.9th percentile of coverage in each sample.

```{r}
filtered.myobj=filterByCoverage(myobj,lo.count=10,lo.perc=NULL,
                                      hi.count=NULL,hi.perc=99.9)
```


# Comparative analysis
## Merging samples

In order to do further analysis, we will need to get the bases covered in all
samples. The following function will merge all samples to one object for
base-pair locations that are covered in all samples. Setting `destrand=TRUE`
(the default is FALSE) will merge reads on both strands of a CpG dinucleotide.
This provides better coverage, but only advised when looking at CpG methylation
(for CpH methylation this will cause wrong results in subsequent analyses). In
addition, setting `destrand=TRUE` will only work when operating on base-pair
resolution, otherwise setting this option TRUE will have no effect. The
`unite()` function will return a `methylBase` object which will be our main
object for all comparative analysis. The `methylBase` object contains
methylation information for regions/bases that are covered in all samples.

```{r}
meth=unite(myobj, destrand=FALSE)
```

Let us take a look at the data content of methylBase object:

```{r}
head(meth)
```

By default, `unite` function produces bases/regions covered in all samples. That
requirement can be relaxed using "min.per.group" option in `unite` function.

```{r,eval=FALSE}
# creates a methylBase object, 
# where only CpGs covered with at least 1 sample per group will be returned

# there were two groups defined by the treatment vector, 
# given during the creation of myobj: treatment=c(1,1,0,0)
meth.min=unite(myobj,min.per.group=1L)
```

## Sample Correlation

We can check the correlation between samples using `getCorrelation`. This
function will either plot scatter plot and correlation coefficients or just
print a correlation matrix.


```{r}
getCorrelation(meth,plot=TRUE)
```

## Clustering samples

We can cluster the samples based on the similarity of their methylation
profiles. The following function will cluster the samples and draw a dendrogram.

```{r}
clusterSamples(meth, dist="correlation", method="ward", plot=TRUE)
```

Setting the `plot=FALSE` will return a dendrogram object which can be
manipulated by users or fed in to other user functions that can work with
dendrograms.

```{r,message=FALSE}
hc = clusterSamples(meth, dist="correlation", method="ward", plot=FALSE)
```

We can also do a PCA analysis on our samples. The following function will plot a
scree plot for importance of components.

```{r}
PCASamples(meth, screeplot=TRUE)
```

We can also plot PC1 and PC2 axis and a scatter plot of our samples on those
axis which will reveal how they cluster.

```{r}
PCASamples(meth)
```

## Batch effects

We have implemented some rudimentary functionality for batch effect control. You
can check which one of the principal components are statistically associated
with the potential batch effects such as batch processing dates, age of
subjects, sex of subjects using `assocComp`. The function gets principal
components from the percent methylation matrix derived from the input
`methylBase` object, and checks for association. The tests for association are
either via Kruskal-Wallis test or Wilcoxon test for categorical attributes and
correlation test for numerical attributes for samples such as age. If you are
convinced that some principal components are accounting for batch effects, you
can remove those principal components from your data using `removeComp`.

```{r}
# make some batch data frame
# this is a bogus data frame
# we don't have batch information
# for the example data
sampleAnnotation=data.frame(batch_id=c("a","a","b","b"),
                            age=c(19,34,23,40))

as=assocComp(mBase=meth,sampleAnnotation)
as

# construct a new object by removing the first pricipal component
# from percent methylation value matrix
newObj=removeComp(meth,comp=1)
```

In addition to the methods described above, if you have used other ways to
correct for batch effects and obtained a corrected percent methylation matrix,
you can use `reconstruct` function to reconstruct a corrected `methylBase`
object. Users have to supply a corrected percent methylation matrix and
`methylBase` object (where the uncorrected percent methylation matrix obtained
from) to the `reconstruct` function. Corrected percent methylation matrix should
have the same row and column order as the original percent methylation matrix.
All of these functions described in this section work on a `methylBase` object
that does not have missing values (that means all bases in methylBase object
should have coverage in all samples).

```{r}
mat=percMethylation(meth)

# do some changes in the matrix
# this is just a toy example
# ideally you want to correct the matrix
# for batch effects
mat[mat==100]=80
 
# reconstruct the methylBase from the corrected matrix
newobj=reconstruct(mat,meth)
```

## Tiling windows analysis

For some situations, it might be desirable to summarize methylation information
over tiling windows rather than doing base-pair resolution analysis. `methylKit`
provides functionality to do such analysis. The function below tiles the genome
with windows of 1000bp length and 1000bp step-size and summarizes the methylation
information on those tiles. In this case, it returns a `methylRawList` object
which can be fed into `unite` and `calculateDiffMeth` functions consecutively to
get differentially methylated regions. The tilling function adds up C and T
counts from each covered cytosine and returns a total C and T count for each
tile.

As mentioned [before](#reading-the-methylation-call-files), `methRead` sets a
minimum coverage threshold of 10 reads per cytosine to ensure good quality for
downstream base-pair resolution analysis. However in the case of tiling window /
regional analysis one might want to set the initial per base coverage threshold
to a lower value and then filter based on the number of bases (cytosines) per
region. [Filtering samples based on read
coverage](#filtering-samples-based-on-read-coverage) might still be appropriate
to remove coverage biases.



```{r,warning=FALSE}
myobj_lowCov = methRead(file.list,
           sample.id=list("test1","test2","ctrl1","ctrl2"),
           assembly="hg18",
           treatment=c(1,1,0,0),
           context="CpG",
           mincov = 3
           )

tiles = tileMethylCounts(myobj_lowCov,win.size=1000,step.size=1000,cov.bases = 10)
head(tiles[[1]],3)
```



## Finding differentially methylated bases or regions

The `calculateDiffMeth()` function is the main function to calculate
differential methylation. Depending on the sample size per each set it will
either use Fisher's exact or logistic regression to calculate P-values. P-values
will be adjusted to Q-values using [SLIM
method](http://www.ncbi.nlm.nih.gov/pubmed/21098430) [@Wang2011a]. If you have
replicates, the function will automatically use logistic regression. You can
force the `calculateDiffMeth()` function to use Fisher's exact test if you
pool the replicates when there is only test and control sample groups. This
can be achieved with `pool()` function, see [FAQ](# Frequently Asked Questions)
for more info.

In its
simplest form ,where there are no covariates, the logistic regression will try
to model the the log odds ratio which is based on methylation proportion of a
CpG, $\pi_i$, using the treatment vector which denotes the sample group
membership for the CpGs in the model. Below, the "Treatment" variable is used
to predict the log-odds ratio of methylation proportions. 

$$
\text{log}\left(\dfrac{\pi_i}{1-\pi_i}\right) =\beta_0 + \beta_1 Treatment_i
$$

The logistic regression model is fitted per CpG or per region and we test if 
treatment vector has
any effect on the outcome variable or not. In other words,
we are testing if $log(\pi_i/(1-\pi_i)) = \beta_0 + \beta_1 Treatment_i$ 
is a "better" model than $log(\pi_i/(1-\pi_i)) = \beta_0$.

The following code snippet tests for differential methylation. Since the example
data has replicates, the logistic regression based modeling and test will 
be used.

```{r}
myDiff=calculateDiffMeth(meth)
```

After q-value calculation, we can select the differentially methylated
regions/bases based on q-value and percent methylation difference cutoffs.
Following bit selects the bases that have q-value<0.01 and percent methylation
difference larger than 25\%. If you specify `type="hyper"` or `type="hypo"`
options, you will get hyper-methylated or hypo-methylated regions/bases.

```{r}
# get hyper methylated bases
myDiff25p.hyper=getMethylDiff(myDiff,difference=25,qvalue=0.01,type="hyper")
#
# get hypo methylated bases
myDiff25p.hypo=getMethylDiff(myDiff,difference=25,qvalue=0.01,type="hypo")
#
#
# get all differentially methylated bases
myDiff25p=getMethylDiff(myDiff,difference=25,qvalue=0.01)
```

We can also visualize the distribution of hypo/hyper-methylated bases/regions
per chromosome using the following function. In this case, the example set
includes only one chromosome. The `list` shows percentages of hypo/hyper
methylated bases over all the covered bases in a given chromosome.

```{r}
diffMethPerChr(myDiff,plot=FALSE,qvalue.cutoff=0.01, meth.cutoff=25)
```

## Correcting for overdispersion

Overdispersion occurs when there is more variability in the data than assumed by
the distribution. In the logistic regression model, the response variable
$meth_i$ (number of methylated CpGs) is expected to have a binomial
distribution: $$meth_i \sim Bin(n_i, \pi_i)$$ Therefore, the methylated CpGs
will have the variance $n_i \pi_i(1-\pi_i)$ and mean $\mu_i=n_i \pi_i$. $n_i$ is
the coverage for the CpG or a region and $\pi_i$ is the underlying methylation
proportion.

Overdispersion occurs when the variance of $meth_i$ is greater than 
$n_i\hat{\pi_i}(1-\hat{\pi_i})$, where $\hat{\pi_i}$ is the estimated methylation
proportion from the model. This can be corrected by calculating a scaling 
parameter $\phi$ and adjusting the variance as 
$\phi n_i \hat{\pi_i}(1-\hat{\pi_i})$. `calculateDiffMeth` can calculate that 
scaling parameter and use it in statistical tests to correct for overdispersion.
The parameter is calculated as proposed by [@McCullagh1989] as follows:
$\hat{\phi}=X^2/(N-P)$, where $X$ is Pearson goodness-of-fit statistic, $N$ is
the number of samples, and $P$ is the number of parameters. This scaling
parameter also effects the statistical tests and if there is overdispersion
correction the tests will be more stringent in general.

By default,this overdispersion correction is not applied. This can be achieved
by setting `overdispersion="MN"`. The Chisq-test is used by default only when no
overdispersion correction is applied.
If overdispersion correction is applied, the function automatically switches 
to the F-test. The Chisq-test can be manually chosen in this case as well, 
but the F-test only works with overdispersion correction switched on. In both
cases, the procedure tests if the full model (the model where treatment is
included as an explanatory variable) explains the data better than the null
model (the model with no treatment, just intercept). If there is no effect based
on samples being from different groups adding a treatment vector for sample
groupings will be no better than not adding the treatment vector. Below, we
simulate methylation data and use overdispersion correction for the logistic
regression model.

```{r,eval=FALSE}

sim.methylBase1<-dataSim(replicates=6,sites=1000,
                         treatment=c(rep(1,3),rep(0,3)),
                        sample.ids=c(paste0("test",1:3),paste0("ctrl",1:3))
                        )

my.diffMeth<-calculateDiffMeth(sim.methylBase1[1:,],
                                overdispersion="MN",test="Chisq",mc.cores=1)
```


## Accounting for covariates 

Covariates can be included in the analysis. The function will then try to
separate the influence of the covariates from the treatment effect via the
logistic regression model. In this case, we will test if full model (model with
treatment and covariates) is better than the model with the covariates only. If
there is no effect due to the treatment (sample groups), the full model will not
explain the data better than the model with covariates only. In
`calculateDiffMeth`, this is achieved by supplying the `covariates` argument in
the format of a `data.frame`. Below, we simulate methylation data and add make a
`data.frame` for the age. The data frame can include more columns, and those
columns can also be `factor` variables. The row order of the data.frame should
match the order of samples in the `methylBase` object.

```{r,eval=FALSE}

covariates=data.frame(age=c(30,80,34,30,80,40))
sim.methylBase<-dataSim(replicates=6,sites=1000,
                        treatment=c(rep(1,3),rep(0,3)),
                        covariates=covariates,
                        sample.ids=c(paste0("test",1:3),paste0("ctrl",1:3))
                        )
my.diffMeth3<-calculateDiffMeth(sim.methylBase,
                                covariates=covariates,
                                overdispersion="MN",test="Chisq",mc.cores=1)
```

## Finding differentially methylated bases using multiple-cores

The differential methylation calculation speed can be increased substantially by
utilizing multiple-cores in a machine if available. Both Fisher's Exact test and
logistic regression based test are able to use multiple-core option.

The following piece of code will run differential methylation calculation using
2 cores.

```{r, eval=FALSE}
myDiff=calculateDiffMeth(meth,mc.cores=2)
```


# Annotating differentially methylated bases or regions

We can annotate our differentially methylated regions/bases based on gene
annotation using
[genomation](https://bioconductor.org/packages/release/bioc/html/genomation.html)
package. In this example, we read the gene annotation from a BED file and
annotate our differentially methylated regions with that information using
genomation functions. Note that these functions operate on `GRanges` objects ,so
we first coerce methylKit objects to GRanges. This annotation operation will
tell us what percentage of our differentially methylated regions are on
promoters/introns/exons/intergenic region. In this case we read annotation from
a BED file, similar gene annotation information can be fetched using
`GenomicFeatures` package or other packages available from Bioconductor.org.

```{r}
library(genomation)

# read the gene BED file
gene.obj=readTranscriptFeatures(system.file("extdata", "refseq.hg18.bed.txt", 
                                           package = "methylKit"))
#
# annotate differentially methylated CpGs with 
# promoter/exon/intron using annotation data
#
annotateWithGeneParts(as(myDiff25p,"GRanges"),gene.obj)
```

Similarly, we can read the CpG island annotation and annotate our differentially
methylated bases/regions with them.

```{r}
# read the shores and flanking regions and name the flanks as shores 
# and CpG islands as CpGi
cpg.obj=readFeatureFlank(system.file("extdata", "cpgi.hg18.bed.txt", 
                                        package = "methylKit"),
                           feature.flank.name=c("CpGi","shores"))
#
# convert methylDiff object to GRanges and annotate
diffCpGann=annotateWithFeatureFlank(as(myDiff25p,"GRanges"),
                                    cpg.obj$CpGi,cpg.obj$shores,
                         feature.name="CpGi",flank.name="shores")
```

## Regional analysis

We can also summarize methylation information over a set of defined regions such
as promoters or CpG islands. The function below summarizes the methylation
information over a given set of promoter regions and outputs a `methylRaw` or
`methylRawList` object depending on the input. We are using the output of
genomation functions used above to provide the locations of promoters. For
regional summary  functions, we need to provide regions of interest as GRanges
object.

```{r}
promoters=regionCounts(myobj,gene.obj$promoters)

head(promoters[[1]])
```

## Convenience functions for annotation objects

After getting the annotation of differentially methylated regions, we can get
the distance to TSS and nearest gene name using the `getAssociationWithTSS`
function from genomation package.

```{r,}
diffAnn=annotateWithGeneParts(as(myDiff25p,"GRanges"),gene.obj)

# target.row is the row number in myDiff25p
head(getAssociationWithTSS(diffAnn))
```

It is also desirable to get percentage/number of differentially methylated
regions that overlap with intron/exon/promoters

```{r}
getTargetAnnotationStats(diffAnn,percentage=TRUE,precedence=TRUE)
```

We can also plot the percentage of differentially methylated bases overlapping
with exon/intron/promoters

```{r}
plotTargetAnnotation(diffAnn,precedence=TRUE,
    main="differential methylation annotation")
```

We can also plot the CpG island annotation the same way. The plot below shows
what percentage of differentially methylated bases are on CpG islands, CpG
island shores and other regions.

```{r}
plotTargetAnnotation(diffCpGann,col=c("green","gray","white"),
       main="differential methylation annotation")
```

It might be also useful to get percentage of intron/exon/promoters that overlap
with differentially methylated bases.

```{r}
getFeatsWithTargetsStats(diffAnn,percentage=TRUE)
```

# methylKit convenience functions

## Coercing methylKit objects to GRanges

Most `methylKit` objects (methylRaw,methylBase and methylDiff), including
methylDB objects (methylRawDB,methylBaseDB and methylDiffDB) can be coerced to
`GRanges` objects from `GenomicRanges` package. Coercing methylKit objects to
`GRanges` will give users additional flexibility when customizing their
analyses.

```{r}
class(meth)
as(meth,"GRanges")
class(myDiff)
as(myDiff,"GRanges")
```


## Converting methylKit objects to methylDB objects and vice versa

**methylDB** objects (`methylRawDB`, `methylBaseDB` and `methylDiffDB`) can be
coerced to normal `methylKit` objects. This might speed up the analysis if
sufficient computing resources are available. This can be done via "as()"
function.

```{r}
class(myobjDB[[1]])
```

```{r,eval=FALSE}
as(myobjDB[[1]],"methylRaw")
```

You can also convert methylDB objects to their in-memory equivalents. Since
that requires an additional parameter (the directory where the files will be
located), we have a different function, named `makeMethylDB` to achieve this 
goal. Below, we convert a methylBase object to `methylBaseDB` and saving it 
at "exMethylDB" directory.

```{r,eval=FALSE}
data(methylKit)
 
objDB=makeMethylDB(methylBase.obj,"exMethylDB")

```

## Loading methylDB objects from tabix files

Since version 1.13.1 of methylKit the underlying tabix file of **methylDB**
objects (`methylRawDB`, `methylBaseDB` and `methylDiffDB`) include a header
which stores the corresponding metadata of the object. Thus you can recreate the
object with just the tabix file, which allows easy sharing of methylDB objects
accross sessions or users.

```{r, }
data(methylKit)
baseDB.obj <- makeMethylDB(methylBase.obj,"my/path")
mydbpath <- getDBPath(baseDB.obj)
rm(baseDB.obj)

methylKit:::checkTabixHeader(mydbpath)
readMethylDB(mydbpath)
```

## Selection: subsetting methylKit Objects

We can also select rows from `methylRaw`, `methylBase` and `methylDiff`
objects and methylDB pendants with `select` function. An appropriate methylKit 
object will be returned as a result of `select` function. Or you can use the 
`'['` notation to subset the methylKit objects.

```{r}
select(meth,1:5) # get first 10 rows of a methylBase object
myDiff[21:25,] # get 5 rows of a methylDiff object
```

**Important:** Using `select` or `'['` on methylDB objects will return its 
normal `methylKit` pendant, to avoid overhead of database operations.

### selectByOverlap

We can select rows from any methylKit object, that lie inside the ranges of a 
`GRanges` object from `GenomicRanges` package with `selectByOverlap`
 function. An appropriate methylKit object will be returned as a result of 
 `selectByOverlap` function.
 
```{r,message=FALSE,warning=FALSE,eval=FALSE}
library(GenomicRanges)
my.win=GRanges(seqnames="chr21",
               ranges=IRanges(start=seq(from=9764513,by=10000,length.out=20),width=5000) )
 
# selects the records that lie inside the regions
selectByOverlap(myobj[[1]],my.win)
```

**Important:** Using `selectByOverlap` on methylDB objects will return its
normal `methylKit` pendant, to avoid overhead of database operations.

## reorganize(): reorganizing samples and treatment vector within methylKit objects

The `methylBase` and `methylRawList`, as well as methylDB pendants can be 
reorganized by `reorganize` function. The function can subset the objects 
based on provided sample ids, it also creates a new treatment vector 
determining which samples belong to which group. Order of sample ids should 
match the treatment vector order.

```{r,eval=FALSE}
# creates a new methylRawList object
myobj2=reorganize(myobj,sample.ids=c("test1","ctrl2"),treatment=c(1,0) )
# creates a new methylBase object
meth2 =reorganize(meth,sample.ids=c("test1","ctrl2"),treatment=c(1,0) )
```


## percMethylation(): Getting percent methylation matrix from methylBase objects

Percent methylation values can be extracted from `methylBase` object by using
`percMethylation` function.

```{r, eval=FALSE}
# creates a matrix containing percent methylation values
perc.meth=percMethylation(meth)
```

## methSeg(): segmentation of methylation or differential methylation profiles
Methylation or differential methylation profiles can be segmented to sections
that contain similar CpGs with respect to their methylation profiles. This 
kind of segmentation could help us find interesting regions. For example, 
segmentation analysis will usually reveal high or low methylated regions, where
low methylated regions could be interesting for gene regulation. The algorithm
first finds segments that have CpGs with similar methylation levels, then those
segments are classified to segment groups based on their mean methylation levels.
This enables us to group segments with similar methylation levels to the 
same class. 

See more at
http://zvfak.blogspot.de/2015/06/segmentation-of-methylation-profiles.html

```{r, eval=FALSE}
 download.file("https://raw.githubusercontent.com/BIMSBbioinfo/compgen2018/master/day3_diffMeth/data/H1.chr21.chr22.rds",
               destfile="H1.chr21.chr22.rds",method="curl")

 mbw=readRDS("H1.chr21.chr22.rds")

 # it finds the optimal number of componets as 6
 res=methSeg(mbw,diagnostic.plot=TRUE,maxInt=100,minSeg=10)

 # however the BIC stabilizes after 4, we can also try 4 componets
 res=methSeg(mbw,diagnostic.plot=TRUE,maxInt=100,minSeg=10,G=1:4)

 # get segments to BED file
 methSeg2bed(res,filename="H1.chr21.chr22.trial.seg.bed")


```

# Frequently Asked Questions

Detailed answers to some of the frequently asked questions and various HOW-TO's
can be found at http://zvfak.blogspot.com/search/label/methylKit. In addition,
http://code.google.com/p/methylkit/ has online documentation and links to
tutorials and other related material. You can also check methylKit Q\&A forum
for answers https://groups.google.com/forum/&#35;!forum/methylkit_discussion.

Apart from those here are some of the frequently asked questions.

### How can I select certain regions/bases from `methylRaw` or `methylBase` objects ?

See `?select` or `help("[", package = "methylKit")`

### How can I find if my regions of interest overlap with
exon/intron/promoter/CpG island etc.?

Currently, we will be able to tell you if your regions/bases overlap with the
genomic features or not. See `?getMembers`.

### How can I find the nearest TSS associated with my CpGs ?

See `?genomation::getAssociationWithTSS`

### How do you define promoters and CpG island shores ? 

Promoters are defined by options at `genomation::readTranscriptFeatures`
function. The default option is to take -1000,+1000bp around the TSS and you can
change that. Same goes for CpG islands when reading them in via
`genomation::readFeatureFlank` function. Default is to take 2000bp flanking
regions on each side of the CpG island as shores. But you can change that as
well.

### What does Bismark SAM output look like, where can I get more info ?

Check the Bismark [@Krueger2011]
[website](http://www.bioinformatics.bbsrc.ac.uk/projects/bismark/) and there are
also example files that ship with the package. Look at their formats and try to
run different variations of `processBismarkAln()` command on the example files.

### How can I reorder or remove samples at/from  `methylRawList` or `methylBase`
objects ?

See `?reorganize`

### Should I normalize my data ?

`methylKit` comes with a simple `normalizeCoverage()` function to normalize read
coverage distributions between samples. Ideally, you should first filter bases
with extreme coverage to account for PCR bias using `filterByCoverage()`
function, then run `normalizeCoverage()` function to normalize coverage between
samples. These two functions will help reduce the bias in the statistical tests
that might occur due to systematic over-sampling of reads in certain samples.


### How can I force methylKit to use Fisher's exact test ? 

`methylKit` decides which test to use based on number of samples per group. In
order to use Fisher's exact there must be one sample in each of the test and
control groups. So if you have multiple samples for group, the package will
employ Logistic Regression based test. However, you can use `pool()` function to
pool samples in each group so that you have one representative sample per group.
`pool()` function will sum up number of Cs and Ts in each group. We recommend
using `filterByCoverage()` and `normalizeCoverage()` functions prior to using
`pool()`. See `?pool`

### Can use data from other aligners than Bismark in methylKit ?

Yes, you can. methylKit can read any generic methylation percentage/ratio file
as long as that text file contains columns for chromosome, start, end, strand, 
coverage and number of methylated cytosines. However, methylKit can only 
process SAM files from Bismark. For other aligners, you need to get a text file
containing the minimal information described above. Some aligners will come with
scripts or built-in tools to provide such files.
See http://zvfak.blogspot.com/2012/10/how-to-read-bsmap-methylation-ratio.html 
for how to read methylation ratio files from BSMAP [@Xi2009] aligner.

### Can I transform an methylKit object into an methylDB object ?

Yes, you can. Many functions of the analysis workflow provide an `save.db`
argument, which allows you to save the output as methylDB object. For example
see `?unite` and also check the `...` argument section for further details.

You can also use the `makeMethylDB()` function to export your in-memory object 
to flat-file database.

### How could I share methylKit objects ?

Starting from version 1.13.1, when generating tabix files we are storing all 
required metadata in the header of the created tabix file. The function 
`readMethylDB()` can be used to load supported tabix files only from the file 
path. Supported tabix files are created during normal tabix-based workflow or 
exported with `makeMethylDB()` function whenever using methylKit versions > 1.13.1. 

### Where do I find the flatfile database underlying a methylDB?

You can easily find the underlying flatfile database (aka tabix file) using the `getDBPath()`
function which prints the absolute location. Please note that
starting  is the generated when you decide to set a db.

### Why does my methylBaseDB flatfile database has a different name now ?

In prior version the filename was just generated by comining sample-IDs, but
this lead to unexpected errors. Starting from version 1.3.2 of methylKit we
changed the filename pattern of the `methylBaseDB` and `methylDiffDB` database
files to "methylBase_suffix.txt.bgz"/"methylDiff_suffix.txt.bgz", where suffix
is either a self-defined string given by the `suffix` argument or a
random-string.

### How can I make a bigwig file from methylKit result?

You can use the rtacklayer package, it should be able to convert GRanges objects to bigWig. 

### My data comes from MIRA-seq, can I use methylKit to perform the differential
methylation analysis and its annotation?
 
The package methylKit is designed for analysing methylation data from bisulfite
sequencing (such as WGBS or RRBS) and as such not designed for affinity based
method (like MIRA-Seq, MeDIP), wich produce other type of signal, more like that
of ChiP-Seq. The Developers of MIRA-Seq protocol suggest the 
[MEDIPS](https://bioconductor.org/packages/release/bioc/html/MEDIPS.html) 
package to analyse their data.

### My data comes from Methylation arrays, can I use methylKit to analyse my data ?

The package methylKit is designed for analysing methylation data from bisulfite
sequencing (such as WGBS or RRBS) and as such does not provide any preprocessing
methods required for array based methods (like Illumina Methylation arrays 
(27K, 450k or EPIC (850k))), please check Bioconductor
(https://bioconductor.org/packages/release/BiocViews.html#___MethylationArray)
for more suitable package to perform these steps. You could theoretically use
methylKit to perform downstream analysis but this would require constructing a
table that mimics our expected count based format and is not officially
supported.

### How can I analyze data generated from a local alignment ?

You cannot use the function processBismarkAln() to extract methylation calls,
but you have to use [methylDackel](https://github.com/dpryan79/MethylDackel) or [Bismark methylation extractor](https://github.com/FelixKrueger/Bismark/tree/master/Docs#iv-running-bismark_methylation_extractor) to generate
input files for methylKit.

The reason why we were not dealing with this directly is described here: 
https://sequencing.qcfail.com/articles/soft-clipping

### How can I analyze data generated from a spliced alignment ?

We currently do not fully support spliced alignments generate with Bismarks's HISAT2 mode, but you can extract methylation calls with [methylDackel](https://github.com/dpryan79/MethylDackel) or [Bismark methylation extractor](https://github.com/FelixKrueger/Bismark/tree/master/Docs#iv-running-bismark_methylation_extractor) to generate
input files for methylKit.



### Why does the regionCount function not keep the input region order?

The given regions (Granges/GrangesList object) will be orderd based on
chromosome and position before searching for overlaps, so the resulting
methylKit object might have a different ording than expected. We are doing
this is to ensure that resulting output is consistent for in-memory and
database based objects, as database based objects always have to be sorted to
enable tabix indexing and providing fast random access.

If you to still want get a custom ordering of the output regions you can
order the single regions in any object by providing your indices to the
`select` or `extract` functions.

```{r}
## methylDiff object sorted by chromosome and position 
myDiff
## can be ordered by decreasing absolute methylation difference
myDiff[order(-abs(myDiff$meth.diff))]
```



# Acknowledgements

This package is initially developed at Weill Cornell Medical College by 
Altuna Akalin with important code contributions from 
Matthias Kormaksson(mk375@cornell.edu) 
and Sheng Li (shl2018@med.cornell.edu). 
We wish to thank especially Maria E. Figueroa, Francine Garret-Bakelman, 
Christopher Mason and Ari Melnick for their contribution of ideas, data and 
support. Their support and discussions lead to development of methylKit.

## Full list of contributors

* Altuna Akalin (main design and development)
* Matthias Kormaksson (initial differential methylation tests)
* Sheng Li (adding PCA and clustering)
* Adrian Bierling (methylation simulation, covariate and over-dispersion correction)
* Alexander Gosdschan (C++ based BAM parsing and tabix based classes )
* Arsene Webo (methylation segmentation)

# R session info

```{r}
sessionInfo() 
```


# References

```{r,eval=TRUE,echo=FALSE}
# tidy up                  
rm(myobjDB)              
unlink(list.files(pattern = "methylDB",full.names = TRUE),recursive = TRUE)
```
