
%the following has to be kept in comments !!
%\VignetteIndexEntry{arrayMagic: two-colour DNA array quality control and preprocessing}
%\VignetteDepends{Biobase, vsn, limma}
%\VignetteKeywords{quality control, two colour microarray data, normalisation}
%\VignettePackage{arrayMagic}

% possibly use tempdir() instead of
% the default savePath, i.e. ''.''
% (at this point not very important)

% notes on further improvement
% 'pastel' colours red and green instead of darkred and darkgreen ?! (and blue)

\documentclass[a4paper, 12pt]{article}

%\usepackage{times}
\usepackage{a4wide}
\usepackage[latin1]{inputenc}

\title{arrayMagic: two-colour DNA array quality control and preprocessing}
\author{Andreas Buneß}


\newcommand{\Rfunction}[1]{{\texttt{#1}}}
\newcommand{\Robject}[1]{{\texttt{#1}}}
\newcommand{\Rpackage}[1]{{\textit{#1}}}
\newcommand{\Rmethod}[1]{{\texttt{#1}}}
\newcommand{\Rfunarg}[1]{{\texttt{#1}}}
\newcommand{\Rclass}[1]{{\textit{#1}}}

\setcounter{secnumdepth}{0}

\begin{document}

% should avoid additional generation of
% encapsulated postscript graphics which
% even may have side effects if the code
% contains lines like this: i <- i + 1
\SweaveOpts{eps=false}

\maketitle
\tableofcontents


%% Wolfgang: 
%% www.bioconductor.org/develPage/guidelines/programming/performance-issues.pdf%%
%% has to be placed behind \maketitle and \tableofcontents ??
%% eval=FALSE section are excecuted in a second run
%% and will be blocked with the following statement
%% BUT this might be desired for testing of all code presented !!
<<noexectwice,eval=FALSE,echo=FALSE,results=hide>>=
if( length(grep(
      "/home/buness/bunessFileserver/R/Rpacks/arrayMagic", getwd())) > 0 |
   length(grep(
      "/home/buness/R/Rpacks/arrayMagic", getwd())) > 0                   ){
  ## process a second time 
}else{
  q(save="no") 
}
@


% change the line width in R and
% possibly also change the prompt
% via 
% options(prompt="MyR>")
%
<<setup,echo=FALSE,results=hide>>= 
  options(width=70)
@


\section{Abstract}

This document explains an efficient and
automated way to load data from two colour microarray 
image quantification result files into R and Bioconductor. 
The data are normalised and several quality diagnostic plots are
generated on the fly. 

%% \section{Workflow Overview}

%% The workflow can be summarized as follows:

%% \begin{enumerate}
%%   \item create and load description of the experiment
%%   \item read image quantification result files
%%   \item normalisation of the data
%%   \item quality diagnostics and visualisation
%%   \item export of the data
%%   \item follow-up analysis
%% \end{enumerate}


\section{Preliminaries}  To go through this document, 
  you need to have installed R 1.9.0, 
  the Bioconductor libraries
  \Rpackage{Biobase, limma} >=1.2.0, \Rpackage{vsn} >=1.4.9 and 
  \Rpackage{arrayMagic} >= 1.4.5, which contains part 
  of the lymphoma data set which is used as example
  (cf. http://llmpp.nih.gov/lymphoma/).
<<libraries,echo=TRUE,results=hide>>= 
  library(Biobase)
  library(vsn)
  library(limma)
  library(arrayMagic)
@


\section{Workflow}

%%%%%%%%%%%

\subsection{Create and load description of the experiment}
  The starting point is a description file which comprises the experiment. 
  The description file must contain the file names of all
  image analysis quantification results and should contain all other 
  analysis relevant information. For the example data set 
  such a tab-deliminated file is provided as shown below:


<<descriptionFileAccessOnly,echo=FALSE,results=hide>>=
packageDirectory <- system.file(package="arrayMagic")
loadPath <- file.path( packageDirectory, "extdata" )
fileName <-"phenoDataLymphoma.txt"
@ 
<<showDescriptionFile,echo=FALSE>>=
read.delim( file.path(loadPath, fileName) )
@
 
  Relevant information may be as various as
  probe origin, hybridisation day, slide charge,
  tumour type etc. Each line of the description
  file  has to correspond to either a single 
  hybridisation or a single channel of one hybridisation
  depending on the requirements of the experimental design
  (cf. the argument method \Rfunarg{channelColumn} of
   the method \Rmethod{readIntensities}).

  The example description file as well as the image quantification
  result files are accessible on your system. The
  access route is determined as follows. 
  
<<descriptionFile,echo=TRUE>>=
packageDirectory <- system.file(package="arrayMagic")
loadPath <- file.path( packageDirectory, "extdata" )
fileName <-"phenoDataLymphoma.txt"
@ 

  The description is read and stored in a \Rclass{data.frame}
   named \Robject{description}:
 
<<readDescriptionFile,echo=TRUE,results=hide>>=  
description <- readpDataSlides(fileName, loadPath=loadPath)
@ 

%%%%%%%%%

\subsection{Reading image quantification result files}

The \Rfunarg{fileNameColumn} of your experiment description contains
the file names of the image quantification result files. All raw data are
read in and stored in an instance 
of the class \Rclass{arrayData}
named \Robject{aD}.

<<readIntensities,echo=TRUE,results=hide>>=  
aD <- readIntensities(description, fileNameColumn="fileName", 
                      slideNameColumn="slideNumber", 
                      loadPath=loadPath, type="ScanAlyze")
@ 


There is a generic way to deal with different types of 
image quantification result apart from predefined types 
like 'ScanAlyze' and 'GenePix' (cf. the arguments 
\Rfunarg{generic} and \Rfunarg{genericOneFilePerChannel}
of \Rmethod{readIntensities}). 
For 'ScanAlyze' type files the following lines do the same job.

<<readIntensitiesLong,echo=TRUE,eval=FALSE,results=hide>>=  
dataColumns <-  c("CH1I", "CH1B", "CH2I", "CH2B")
names(dataColumns) <- c("greenForeground","greenBackground","redForeground","redBackground")
spotAnnoColumns <- c( "HEADER", "SPOT", "GRID", "ROW", "COL" )
skip <- 0
removePattern <- "^REMARK"
aD <- readIntensities(description, fileNameColumn="fileName",
                      slideNameColumn="slideNumber", loadPath=loadPath, 
                      type="generic", spotAnnoColumns=spotAnnoColumns, 
                      dataColumns=dataColumns, removePattern=removePattern,
                      skip=skip)
@

Some image quantification result files require to change the
\Rfunarg{quote} argument to succeed in reading of the files; 
as first alternative choice you may set 
\Rfunarg{quote="$\backslash$""}.


%%%%%%%%%%%

\subsection{Normalisation of the data}

In general dye, slide and hybridisation effects besides others
make a calibration or normalisation step of the data inevitable.
Moreover, for quality assessment not only the raw data, but 
also the normalised ones have to be considered. Difficulties
in normalisation may indicate low quality hybridisations.
The method \Rfunction{normalise} offers a flexible way to normalise
your data with 'loess', 'vsn' or  'quantile' type normalisations.
Channels, groups of hybridisations and subsets of spots,
e.g. by grid or print-tip, can be normalised separately.

<<normalise,echo=TRUE,results=hide>>=  
eSRG <- normalise(aD, subtractBackground=TRUE, method="vsn", spotIdentifier="SPOT") 
@ 

The method \Rfunction{normalise} returns an object
of class \Rclass{exprSetRG} which contains the normalised
data of both channels. Details on the class are
given below. The experiment description information
has been passed on to the object.
Unique identifiers which have been
supplied with the raw data image quantification result 
files in the column 'SPOT' have been added as 'gene'-names 
to the object. Here, the given unique identifiers correspond 
to a consecutive numbering. The annotation 
information can be obtained as follows.

<<objectAccess,echo=TRUE>>=  
pDataSlide(eSRG)
spotGeneNames <- geneNames(eSRG) 
@ 



%%%%%%%%%%%
\subsection{Quality diagnostics and visualisation}

Several quality and hybridisation characteristics 
are calculated with the help of the function 
\Rfunction{qualityParameters}.
All results are stored in a list object.
The quality scores given per microarray 
can be saved in a tab-deliminated
file if the argument \Rfunarg{resultFileName} is
supplied. Details on all quality measures
can be found on the help page or in the manual.

<<qualityParameters,echo=TRUE>>=  
qPL <- qualityParameters(arrayDataObject = aD, 
                        exprSetRGObject = eSRG,
                        spotIdentifier= "SPOT",
                        slideNameColumn="slideNumber",
                        resultFileName="qualityScores.txt")
@ 

These quality characteristics are utilised by the
function \Rfunction{qualityDiagnostics} which automatically
generates several diagnostic plots. Examples of these
plots are shown in the Figures
\ref{distributionRaw}, \ref{distributionRawLogRatios}
and
\ref{slideDistances}.
%and \ref{quality}.

<<qualityDiagnostics,echo=TRUE,fig=FALSE,results=hide>>=  
qualityDiagnostics(arrayDataObject = aD,
                   exprSetRGObject = eSRG, 
                   qualityParameters = qPL, 
                   plotOutput="pdf")
@ 


\begin{figure}[htb]
\begin{center}  
  \includegraphics[width=0.4\textwidth]{distributionOfRawDataChannelWise.pdf}
  \includegraphics[width=0.4\textwidth]{distributionOfNormalisedData.pdf}
  \caption{ \label{distributionRaw} 
    The plot on the left hand side
    characterises the distribution of the raw intensity values 
    and on the right
    hand side of the normalised  
    intensity values for each channel green and red
    of all hybridisations.
    Each box characterizes the median and range of 50\% of the data,
    i.e. the 25, 50 and 75 percent quantiles of the data.
  }
 \end{center}
\end{figure}


\begin{figure}[htb]
\begin{center}  
 \includegraphics[width=0.4\textwidth]{distributionOfRawDataLogRatio.pdf}
 \includegraphics[width=0.4\textwidth]{distributionOfNormalisedDataLogRatio.pdf}
  \caption{ \label{distributionRawLogRatios} 
    The plot on the left hand side
    characterises the distribution of the log-ratios 
    of the non-normalised and on the right
    hand side of the normalised data. 
    Each box characterizes the median and range of 50\% of the data,
    i.e. the 25, 50 and 75 percent quantiles of the data.
  }
 \end{center}
\end{figure}


\begin{figure}[htb]
\begin{center}  
  %\includegraphics[width=\textwidth,keepaspectratio=true]{slideDistances.pdf}
  \includegraphics[width=0.5\textwidth]{slideDistances.pdf}
  \caption{ \label{slideDistances} 
    (Dis)similarities between all pairs of hybridisations.
    This may unveil potential technical artifacts 
    like batch effects. Such global view on the data does not
    allow to separate technical and biological variation.
    Here, the blue and yellow 'blocks' 
    characterize the two different tumor types
    'CLL' and 'DLCL'. An ANOVA approach 
    explicitly addressing known technical 
    and biological variation, followed by a subsequent 
    correlation analysis of the residuals 
    may provide further insight into the data.
    % Wolfgang: e.g. via heatmap
  }
 \end{center}
\end{figure}


%% \begin{figure}[htb]
%% \begin{center}  
%%  \includegraphics[width=\textwidth]{visualiseQualityParametersOutput.pdf}
%%   \caption{ \label{quality} 
%%       }
%%  \end{center}
%% \end{figure}


Spatial inhomogeneities and scratches 
can be detected by visual inspection
of the hybridisations. The function
\Rfunction{visualiseHybridisations} re-generates
a two dimensional representation of
the raw or normalised data. The
output of the following code is shown in
Figure \ref{visualisedData}.

%% for faster processing:
%% possibly use eval=FALSE and store the plots beforhand
<<visualiseHybridisations,echo=TRUE,eval=TRUE,fig=FALSE,results=hide>>=  
mappingColumns <- list(Block = "GRID", Column = "COL", Row = "ROW")
visualiseHybridisations(arrayDataObject = aD[,c(2,6)],
                        slideNameColumn = "slideNumber",
                        mappingColumns = mappingColumns)
visualiseHybridisations(arrayDataObject = aD[,6],
                        exprSetRGObject = slideSubset( eSRG, j = 6 ),
                        type= "normalised",
                        slideNameColumn = "slideNumber",
                        mappingColumns = mappingColumns)
@ 


\begin{figure}[htb]
\begin{center}  
 \includegraphics[width=\textwidth]{hybridisation_raw_2.pdf}
 \includegraphics[width=\textwidth]{hybridisation_raw_6.pdf}
 \includegraphics[width=\textwidth]{hybridisation_normalised_6.pdf}
  \caption{ \label{visualisedData} 
    \textit{Top:} 
    visualisation of the raw data of the second hybridisation.
    The foreground and background of the red and green channel
    is shown.
    \textit{Middle:} the raw data and
    \textit{bottom:} normalised data of the sixth hybridisation.
  }
 \end{center}
\end{figure}


Additional graphical checks can be implemented by
means of the R and Bioconductor environment. 

A simple scatterplot is easily generated
as shown below and on the left in Figure 
\ref{scatterplots}.
The spots of the first eight subgrids on the
microarray are coloured in red, all others
in black. The average intensity against
the log ratio is shown on the right of
Figure \ref{scatterplots}.


<<additionalVisualInspectionScatterplot,fig=FALSE,echo=TRUE>>=
green <- exprs(getExprSetGreen(eSRG))
red <- exprs(getExprSetRed(eSRG))

grid <- getSpotAttr(aD)[["GRID"]]
colour <- c("black", "red")[ as.integer(grid %in% 1:8) + 1]

par(mfrow=c(1,2))

plot(green[, 5], red[, 5], pch=".", col=colour)
plot(x=rowMeans(green[, 5, drop=FALSE], red[, 5, drop=FALSE]), 
     y=green[, 5]-red[, 5], pch=".", xlab="A", ylab="M", col=colour)
@

<<additionalVisualInspectionScatterplotII,fig=FALSE,echo=FALSE,results=hide>>=
pdf(width=7, height=3.5, file="scatterplots.pdf")

par(mfrow=c(1,2))

plot(green[, 5], red[, 5], pch=".", col=colour)
plot(x=rowMeans(green[, 5, drop=FALSE], red[, 5, drop=FALSE]), 
     y=green[, 5]-red[, 5], pch=".", xlab="A", ylab="M", col=colour)

dev.off()
@


\begin{figure}[htb]
\begin{center}  
  \includegraphics[height=0.4\textwidth]{scatterplots.pdf}
  \caption{ \label{scatterplots} 
    The green versus the red channel of the fifth hybridisation
    is shown on the left hand side. A different, but similar
    view on the same hybridisation is shown on the right hand
    side, i.e. the average intensity versus its log ratio.
    All spots belonging to the first eight subgrids are 
    coloured in red instead of black.
  }
 \end{center}
\end{figure}




The esitmated density of the log ratios for
each of the sixteen subgrids of the first
hybridisation is shown on the left in Figure
\ref{subgridDensities}.
Similarly, the estimated density of the
first subgrid for each of the eight 
hybridisations is shown on the right.
The within and between hybridisation
variability appears to be comparable.

%% The frequently shown relationship between the average
%% intensity and the log ratio is generated for
%% the fifth hybridisation as follows:
%% <<MAplot,echo=TRUE>>=
%% green <- exprs(getExprSetGreen(eSRG))[,5]
%% red <- exprs(getExprSetRed(eSRG))[,5]
%% plot(x=(red+green), y=(red-green), pch=".") 
%% @ 

%% 1 array: 16 grids containing 576 spots
%% 
%% 16 grids of 8 slides of 7 values returned by density 
%% x <- lapply( unique(grid), function(g) apply( lR[grid==g,], 2, density))

%%   more intuitive 
%% dxHybOne <- sapply( split( lR[,1], grid), function(x) density(x)$x)
%% dyHybOne <- sapply( split( lR[,1], grid), function(x) density(x)$y)
%%   and more efficient code for the subgrids of the first hybridisation
%% dHybOne <- lapply(split( lR[,1], grid), function(x) density(x) )
%% dxHybOne <- cbind( sapply( dHybOne, function(x) x$x))
%% dyHybOne <- cbind( sapply( dHybOne, function(x) x$y))

<<additionalVisualInspectionDensity,fig=FALSE,echo=TRUE>>=
lR <- exprs(getExprSetLogRatio(eSRG))

par(mfrow=c(1,2))

dHybOne <- lapply(split( lR[,1], grid), function(x) density(x) )
dxHybOne <- cbind( sapply( dHybOne, function(x) x$x))
dyHybOne <- cbind( sapply( dHybOne, function(x) x$y))
matplot(dxHybOne, dyHybOne, pch=".", ylim=c(0,1))

dxGridOne <- apply( lR[grid==1,], 2, function(x) density(x)$x)
dyGridOne <- apply( lR[grid==1,], 2, function(x) density(x)$y)
matplot(dxGridOne, dyGridOne, pch=".", ylim=c(0,1))
@ 

<<additionalVisualInspectionDensityII,fig=FALSE,echo=FALSE,results=hide>>=
pdf( width=7, height=3.5, file="subgridDensities.pdf")
par(mfrow=c(1,2))
matplot(dxHybOne, dyHybOne, pch=".", ylim=c(0,1))
matplot(dxGridOne, dyGridOne, pch=".", ylim=c(0,1))
dev.off()
@ 

\begin{figure}[htb]
\begin{center}  
  \includegraphics[height=0.4\textwidth]{subgridDensities.pdf}
  \caption{ \label{subgridDensities} 
    The graphic on the left hand side
    characterises the densities of log ratios for
    each of the sixteen subgrids of the first
    hybridisation. The estimated density of the
    first subgrid for each of the eight 
    hybridisations is shown in the right
    graphic.
  }
 \end{center}
\end{figure}


Following the same lines the distribution
of the intensities before and after the
normalisation can be compared  
separately for each channel. 
 
%% rawGreen <- getIntensities(aD)[,"green",]
%% green <- exprs(getExprSetGreen(eSRG))


%% dens <- function(x){
%%    xx <- apply( x, 2, function(x) density(x)$x)
%%    xy <- apply( x, 2, function(x) density(x)$y)
%%    return(list(x=xx, y=xy))
%% }

%% densRawGreen <- dens(log(rawGreen))
%% densGreen     <- dens(green)

%% par(mfrow=c(1,2))
%% matplot(densRawGreen$x, densRawGreen$y, pch=".")
%% matplot(densGreen$x, densGreen$y, pch=".")




%% other possible extensions:
%%
%% overall equality of the distributions could be
%% checked via quantile - quantile plots 
%%
%% possibly check for the modality of the distributions,
%% e.g. two modal background 
%%



%%%%%%%%%%%%%

\subsection{Export of the data}

The \Rfunction{writeToFile} offers a convenient way
to export processed data to a well-formated 
tab-deliminated text file for any kind of 
subsequent analysis in other tools. The
\Rfunarg{channels} allows to select 
between the two channels and the log-ratios,
as well as among raw and processed data. 

%% possibly use eval=FALSE, but no file will be included in the package
<<exportData,echo=TRUE>>=
writeToFile(arrayDataObject = aD, 
            exprSetRGObject = eSRG, 
            rowSelection = 1:100, 
            slideNameColumn = "slideNumber", 
            channels=c("logRatio"), 
            fileName="normalisedLogRatios.txt", 
            )
@ 


%%%%%%%%%%%
\subsection{Further Automation}

The first three steps of the workflow like the
reading of the image files and the normalisation
are integrated in the function \Rfunction{processArrayData}.
Empty spots may be specified and will excluded before
or after the normalisation step. In our example the 
function could be called as follows: 

%% eval=FALSE to speed-up computation
<<processArrayData,echo=TRUE,eval=FALSE,fig=FALSE,results=hide>>=  
resultList <- processArrayData(slideDescriptionFile=fileName,
                               fileNameColumn="fileName", 
                               slideNameColumn="slideNumber", 
                               loadPath=loadPath, 
                               savePath=tempdir(),
                               type="ScanAlyze",
                               spotIdentifier="SPOT",
                               spotsRemovedBeforeNormalisation=c("empty",""),  
                               subtractBackground=TRUE, 
                               normalisationMethod="vsn", 
                               plotOutput="pdf"
                               )
@ 




%%%%%%%%%%%%%

\subsection{Follow-up analysis}

A simple group comparison is presented as example for a follow-up analysis.
Genes are selected which differ between the two tumour groups
and which belong to the top 4000 highest intensities in the
green channel. The 'difference' is calculated by means of an
univariate t-test with no correction for multiple testing.
The intensities of the green channel are ranked by their 
maximum intensity value to determine the 'highest' ones. 
A ranking based on the average intensity may for example
exclude genes with low or no expression in all but one 
condition. The function \Rfunction{myTTest} is only shown
to demonstrate the usage of the function \Rfunction{esApply}
of the package \Rpackage{Biobase}.

%% possibly use eval=FALSE (here and below)
<<tTest,echo=TRUE>>=  
myTTest <- function(x){
  xs <- split( x, tumortype )
  result <- t.test( x=xs[[1]], y=xs[[2]], var.equal=TRUE)$p.value  
  return(result)  
}

logRatios <- getExprSetLogRatio(eSRG)
pValues <- esApply(logRatios, 1, myTTest)

factorTumor <- factor(pDataSlide(eSRG)$tumortype)
pValuesFast <- rowttests(x=exprs(logRatios), fac=factorTumor)$pvalue
stopifnot( all.equal.numeric(pValuesFast, pValues) )

sampleIntensities <- exprs(getExprSetGreen(eSRG))
maxIntensity <- apply(sampleIntensities, 1, max)
highestOnes <- rank(-maxIntensity) <= 4000
selectedIndexes <- which( pValues < 0.00001  & highestOnes)
selectedGenes <- geneNames(logRatios)[selectedIndexes]
@ 

The selected genes and their p-values are written to a html-file
named 'result.html'.

%% possibly use eval=FALSE, but no file will be included in the package
<<writeResult,echo=TRUE>>=
df <- data.frame(genes=I(selectedGenes),pValues=pValues[selectedIndexes])
write.htmltable(df, "result", sortby="pValues", decreasing=FALSE)
@ 


\section{Details on the classes}

All data are stored in two R classes. The class 
\Rclass{exprSetRG} offers a convienent way to deal with 
normalised two colour microarray data. An instance
of the class stores the normalised data for each channel.
This offers the possibility to retrieve log-ratios and 
single channel intensities from the same instance as
you might need it for filtering and analysis.
It is an extension of the class \Rclass{exprSet} 
which is part of the library \Rclass{Biobase}. 
The class \Rclass{arrayData} is a simple 
class for all raw data information like foreground and
background intensities, spot weights, hybridisation
and spot annotation information.

Important methods offered by the \Rclass{exprSetRG-class} 
are \Rfunction{cbind, slideSubset, pDataSlide, getExprSetLogRatios}
and by the \Rclass{arrayData-class} the subset operator 
\Rfunction{[]} and \Rfunction{cbind}.


%%%%%%%%%%%%%

\section{Example application: different microarray layouts}

Occasionally different types of microarrays have been
used in the same experiment. For example an upgraded
clone library or changing spotting layouts may result
in different types of microarrays. 
If a unique identifier for all spots is 
supplied with the data files it is possible
to extract a subset common to all types
of microarrays. The following lines of code
demonstrate how one might combine two types
of microarrays. This mock example makes use
of the same example data set as before.
Two times the same data are combined. The
approach naturally extends to more than
two types. A separate description file
is required for each set of microarrays
belonging to the same type.


%% eval=FALSE, to speed-up calculation
%% required by chunk slideMerge
<<layout,eval=FALSE,echo=TRUE,results=hide>>=  

SPOTIDENTIFIER <- "SPOT"

rLOne <- processArrayData(
                          slideDescriptionFile = fileName,
                          fileNameColumn       = "fileName",
                          slideNameColumn      = "slideNumber",
                          loadPath             = loadPath, 
                          savePath             = tempdir(),
                          spotIdentifier       = SPOTIDENTIFIER,
                          type                 = "ScanAlyze",
                          normalisationMethod  = "none",
                          plotOutput           = "pdf"
                          )

rLTwo <- processArrayData(
                          slideDescriptionFile = fileName,
                          fileNameColumn       = "fileName",
                          slideNameColumn      = "slideNumber",
                          loadPath             = loadPath, 
                          savePath             = tempdir(),
                          spotIdentifier       = SPOTIDENTIFIER,
                          type                 = "ScanAlyze",
                          normalisationMethod  = "none",
                          plotOutput           = "pdf"
                          )

aDOne <- rLOne$arrayDataObject
aDTwo <- rLTwo$arrayDataObject
    
namesOne <- getSpotAttr(aDOne)[,SPOTIDENTIFIER]
namesTwo <- getSpotAttr(aDTwo)[,SPOTIDENTIFIER]

namesBoth <- intersect(namesOne, namesTwo)

selectionOne <- namesOne %in% namesBoth
selectionTwo <- namesTwo %in% namesBoth

## assertion
stopifnot( ! any(duplicated(namesOne[selectionOne])) )
stopifnot( ! any(duplicated(namesTwo[selectionTwo])) )
    
orderOne <- order(namesOne[selectionOne])
orderTwo <- order(namesTwo[selectionTwo])

aDOne <- aDOne[selectionOne,][orderOne,]
aDTwo <- aDTwo[selectionTwo,][orderTwo,]

aDBoth <- cbind(aDOne, aDTwo)

oneNrExcluded <- sum( !selectionOne )
if( oneNrExcluded > 0 ){
  cat(" excluded ", oneNrExcluded, " items from the first set\n")
}
twoNrExcluded <- sum( !selectionTwo )
if( twoNrExcluded > 0 ){
  cat(" excluded ", twoNrExcluded, " items from the second set\n")
}

rL <- processArrayDataObject(
                             arrayDataObject = aDBoth,
                             spotIdentifier  = SPOTIDENTIFIER,
                             normalisationMethod = "vsn",
                             subtractBackground   = TRUE
                             )
    

@ 

\section{Example application: averaging microarrays}

Technical replicates are very common in microarray
analysis. One might explicitly address such situation
by means of an ANOVA approach. Another approach
could involve the averaging of the technical replicates.
The following example explains how to average
hybridisations in the framework of \Rpackage{arrayMagic}.
The mock example above demonstrating the integration
of different microarray types serves as basis for
this example.
Replication on different levels of the experimental
hierarchy should be treated separately.

%% depends on chunk layout
%% eval=FALSE to speed-up calculations
<<slideMerge,eval=FALSE,echo=TRUE>>=  

eSRGTmp <- slideMerge(exprSetRGObject=rL$exprSetRGObject,
                         slideMergeColumn="slideNumber")
eSRGMerged <- slideMerge(exprSetRGObject=eSRGTmp,
                         slideMergeColumn="sampleid")
@ 


%% \usepackage[...]{tocbibind}
%% \settocbibname{References}
%% tocbibind is a package for adding extra titles (like the
%% bibliography, or index, or List of Figures, or ...) 
%% to the Table of Contents. 
%% \bibliographystyle{plain}

\addcontentsline{toc}{section}{References}
\begin{thebibliography}{}

\bibitem{Buness2004}
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\end{document}

