 Research article
 Open Access
 Published:
Addressing the Challenge of Defining Valid Proteomic Biomarkers and Classifiers
BMC Bioinformatics volume 11, Article number: 594 (2010)
Abstract
Background
The purpose of this manuscript is to provide, based on an extensive analysis of a proteomic data set, suggestions for proper statistical analysis for the discovery of sets of clinically relevant biomarkers. As tractable example we define the measurable proteomic differences between apparently healthy adult males and females. We choose urine as bodyfluid of interest and CEMS, a thoroughly validated platform technology, allowing for routine analysis of a large number of samples. The second urine of the morning was collected from apparently healthy male and female volunteers (aged 2140) in the course of the routine medical checkup before recruitment at the Hannover Medical School.
Results
We found that the Wilcoxontest is best suited for the definition of potential biomarkers. Adjustment for multiple testing is necessary. Sample size estimation can be performed based on a small number of observations via resampling from pilot data. Machine learning algorithms appear ideally suited to generate classifiers. Assessment of any results in an independent testset is essential.
Conclusions
Valid proteomic biomarkers for diagnosis and prognosis only can be defined by applying proper statistical data mining procedures. In particular, a justification of the sample size should be part of the study design.
Background
The field of biomarker discovery or clinical proteomics has raised high hopes generated by reports on potential biomarkers, which in many cases subsequently could not be substantiated in validation studies [1, 2]. Prominent examples are the findings in [3, 4]. This development has resulted in large scepticism from both clinicians and regulatory agencies, which will make the application of valid biomarkers into the arsenal of clinical diagnostics even more of a challenge [5, 6]. Further, it is now generally accepted that single biomarkers are unlikely to result in major advancements as the complexity of disease cannot be captured by a single marker; instead, a panel of such biomarkers must be employed [7, 8]. However, it is equally evident that such a panel must consist of clearly defined and validated biomarkers in order to provide a well defined signature. This raises the issue of the definition of a valid biomarker. As this is obviously of central importance, we have revisited this issue, not only employing theoretical considerations, but also by using a tractable yet realistic case study. The theoretical considerations in this area apply to the following main challenges:

1
Is the change (frequency or abundance) of a certain molecule observed in a proteomics study of disease, the result of the disease, or does it merely reflect an artefact due to technical variability in the preanalytical steps or in the analysis, biological variability, or bias introduced in the study (e.g. due to lifestyle, age, and gender)?

2
How should we estimate the number of samples required for the definition of likely valid biomarkers?

3
Which algorithms can be employed to combine biomarkers into a multimarker classifier, and how can the validity of a multimarker classifier be assessed? Is validation in an independent test set necessary?
In an effort to investigate these issues and propose answers to these questions, we have employed different analysis and statistical strategies towards biomarker definition and validation using a set of data obtained from real samples. While technical differences do exist between proteomics and peptidomics, these approaches investigate a highly similar chemical entity, and the problems and challenges associated with the identification of potential proteomic and peptidomics biomarkers (features significantly associated with the studied physiological or pathophysiological condition) are essentially identical. Therefore, we feel it is appropriate not to distinguish between peptidomics and proteomics throughout this manuscript. Several platforms for proteomics or peptidomics are currently being used in biomarker discovery studies (reviewed in e.g. [9].
We have chosen data from CEMS as one representative example, due to the following reasons: a) CEMS is being used in clinical trials and data from CEMS are applied in clinical decisionmaking, b) sufficient datasets of CEMS were available to us, and c) the analytical performance characteristics of the CEMS platform are well documented [10, 11]
In order to permit a rigorous and realistic assessment of the methodology, the study must (i) represent a real proteomic dataset that is acquired using the same technologies and experimental design as for a biomarker study; (ii) be a classification problem with "typical" complexity, but simple enough to be tractable by standard methods; and (iii) permit the deployment of commonly used statistical analysis strategies in order to benchmark them against an unequivocal outcome. Based on these considerations we choose as an example the definition of proteomic differences between apparently healthy adult males and females. This avoids any bias due to a nonverifiable physiological condition in the subjects, since gender can be assessed with close to 100% confidence [12]. This design avoids an important problem in biomarker discovery pipelines: the so called verification bias. This bias occurs if subjects are not equally likely to have the diagnosis verified by a goldstandard test and if selection for further evaluation is dependent on the diagnostic test result. Of course, in general the clinical situation will not allow for such a sharp definition as in the malefemale case, but standard methods exist for accounting for the verification bias if the clinical readout cannot be assigned with 100% confidence [13–15]. We also used a cohort of subjects with diabetes type II either with normal kidney function (controls, CD) or diabetic nephropathy (cases, DN) to demonstrate the applicability of the methods to a case where the clinical readout may not be verified with 100% confidence. The difference in the malefemale study turned out to be more subtle than in the CD versus DN case, as the differences between the proteomic profiles between males and females are less pronounced than in the CDDN case.
As body fluid to be analysed we have chosen urine. The urinary proteome/peptidome is of high stability, reducing preanalytical variability [16]. CEMS was chosen as technology as it allows for the routine analysis of a large number of samples, and has been thoroughly validated as a platform technology for proteomic biomarker studies [17]. As result of the current study we demonstrate the importance of a strict and correct use of statistics, especially adjustment for multiple testing. We further describe algorithms that enable prediction of the number of samples required for the definition of biomarkers with high confidence. The results presented here also show that different machine learning algorithms perform similarly (and very well) in establishing discriminatory multimarker models. However, it is equally evident that these only lead to meaningful results if the number of data points employed is sufficient to learn the difference between the groups, and that the performance of such models can only be assessed on an independent test set. Although our results have been obtained with a particular proteomic technology, CEMS, the principal conceptual considerations, and hence also the conclusions, are independent of the technology used. Therefore, the results reported here should also be applicable to other datasets generated using alternative standard proteomics technologies such as LCMS or MALDI. Unfortunately, to the best of our knowledge, there is currently no similar dataset publicly available for MALDI or for LCMS. Hence, we cannot report on the application of the proposed methods for either platform.
Results and Discussion
Biomarker selection
The design of the study is depicted in Figure 1. To detect possible biomarkers, we employed samples from 67 males and 67 females, aged 2140, as the training set. All relevant data on all samples used in the study are available in the Additional file 1 and Additional file 2. We accepted only peptides that were present in at least 30% of the male or female samples, as a feature with a smaller frequency in both groups may hardly be seen as significantly associated with gender in this study. This threshold resulted in a total of 1216 peptides for further consideration. The appropriateness of a statistical test is primarily determined by the data distribution. Usually, after lowlevel data processing the resulting data exhibit a mixture distribution characterized by a proportion of observations in a pointmass at zero representing the samples where a peptide is not detected, and a continuous component (see Figure 2). The origin of the pointmass at zero may either be biological, as the protein is really absent in these samples, or technical, as the protein is present but its signal is below the limit of detection (LOD) [18]. The only known fact about the point mass at zero is that those values are between zero and the LOD. In statistical terminology, the proteomics data are left censored. Therefore, usage of standard statistical methods which focus on one part of this mixture at a time can fail to detect differences between classes. The data employed here contains 1169 consonant differences (the group with the higher proportion of zeros has the smaller mean in the continuous component), 38 dissonant differences (the group with the higher proportion of zeros has a larger mean in the continuous component) and 9 without pointmass component. The higher number of consonant markers reflects the fact that markers showing a higher mean are better detectable than those with a mean near to the LOD. A difference in means between the two groups may have its origin in a difference in the proportion of zeros, a difference in the mean of the continuous component, or both. The standard parametric ttest may be inappropriate for such data as the underlying assumptions of the test are strongly violated. Nonparametric tests like the Wilcoxon rank sum test (WT) may be more appropriate [19], but may still fail to distinguish the contributions of the two mixture components to the male and female profiles [20]. This suggests the usage of hypothesis tests specifically developed for pointmass mixture data, like the twopart ttest, twopart WT and empirical likelihood ratio test, which tests the null hypothesis of no difference in the pointmass proportions and no difference in the means of the continuous components [20]. As expected, owing to differences in statistical power, the number of biomarkers declared statistically significant strongly varies with the type of test adopted (Table 1). When subsequently validating in the holdout set, the majority of the initially defined potential biomarkers could not be confirmed. This result is likely due to the inherent multiplicity of the problem, strongly supporting the requirement for adjustment for multiple testing [21–23]. These results are even more pronounced when a smaller cohort is employed, resulting in ≤ 10% of the potential biomarkers being confirmed in the test set (data not shown). To control the false discovery rate (FDR) as correction to multiple testing, the BenjaminiHochberg (BH) procedure was used [24]. In Table 1 we report the number of potential markers with adjusted pvalues less than 0.05. After adjustment for multiple testing, the WT reports the largest number of significant markers (Table 1). Moreover, 78% of the 112 markers declared significant by the twopart WT are also significant when using the standard WT, indicating that using just standard WT, which is part of standard statistical software (e.g., SAS or SPSS), should enable definition of reliable biomarkers. The fact that many of the values in the profiles are tied to zero only makes the WT conservative and the pvalues more trustable [25]; as in a pilot study, a false negative is less harmful than a false positive. To test the stability of the significant markers chosen by the different tests, we investigated which of the differentially expressed markers established will still be a valid marker when tested alone on an independent test set (2 × 67 samples). As seen from Table 1 the standard WT has the most markers holding up in the independent test set. Furthermore, the concordance between the biomarkers found in the training set and in the test set is only slightly lower than that for the twopart WT. The results given above argue in favour of using the standard WT for any similar proteomics data. Previous reports have already stressed that nonparametric statistical tests such as the WT may be more appropriate for proteomics data. However, the use of the standard ttest is still frequently used and reported in the literature [26–28]. We subsequently investigated the number of potential biomarkers that can be defined when employing only a subset of the original samples. Statistically, if a real difference exists, it may always be detected when the sample size is adequate. Hence, studies on small cohorts may overlook important markers. With appropriate sample size all the differentially expressed markers should be detected. Of course, not every difference found with larger sample sizes will be of clinical relevance, hence the need for the incorporation of biological background information. Interestingly, even a subset of the markers found using moderate sample size may still be enough for building a good classifier. As expected, the number of significant markers increases with increasing sample size (see Figure 3). Our simulations, where populations of sizes up to 2 × 480 were generated using resampling with replacement from the 2 × 67 samples, showed that this behaviour stops at sample sizes around 2 × 400 where a plateau is reached (Figure 3 on top left). The concordance of these potential biomarkers in the test set also increases with the sample size. With sample sizes less than 13, no differentially expressed markers are detected at all.
Resampling as means to define "better biomarkers"
Variable selection may be seen as the first part in finding a good classifier and must be performed based on training data only. Usually, variable selection is performed only once using all the available training data. This may, however, introduce a substantial bias in declaring a biomarker differentially expressed. This fact is due to the biological variability in the compared populations (here male and female). Crossvalidation and Monte Carlo crossvalidation (random splitting into learning and test sets) may be adopted to protect the analysis against such a bias. However, as the number of biomarkers may be quite high, these procedures are computationally challenging. Holding out 30% randomly from the 134 male and female training samples and examining the distribution of these biomarkers in the 134 independent test samples, we can detect a clear advantage of the biomarkers that were found with higher frequency in the resamples. From Table 2 we see, provided enough resamplings are done (i.e., N ≥30), that if a biomarker is found significant in more than 75% of the independent resamples then the chance that it could be confirmed in the test set was between 70 and 100%. However, this procedure also results in a further reduction of the available biomarkers, and appears to be only useful when a rather large number of potential biomarkers should be reduced. In depth analysis of the data indicated that for building classifiers (see also below), a reduction via resampling of the number of biomarkers may not be necessary (data not shown). However, the implementation of such resampling is clearly advantageous for e.g. describing any association with (patho) physiology, as this procedure allows for identifying those biomarkers that show the highest likelihood of actually being associated with the investigated (patho)physiology.
Estimation of the sample sizes
An important question in the design of clinical proteomics studies is the selection of an appropriate sample size [29]. The number of units to be included in the study should typically address two issues. First, the differential sample size N_{diff} should allow the identification of putative biomarkers that are differentially expressed between two conditions (e.g. disease versus control). Second, the discriminative sample size N_{disc} of the training data should allow the learning of a confident rule for classifying blinded items.
Estimation of the differential sample size
Here the question is: what is the minimum sample size required to attain a desired statistical power for detecting a meaningful difference between samples? This can be answered by estimation of the differential sample size N_{diff}. This sample size depends on the false positive rate α, typically set at 0.05, the statistical power 1β (e.g. 0.9) and the standardized effect size (e.g. Cohen's δ ) for quantifying how the classes differ. Indeed, the effect size and its variation turn out to be the most important factors influencing N_{diff} estimation. Both, effect size and its variation, are traditionally estimated from previously reported experimental data. Unfortunately, in proteomics typically no previous data are available and anticipation of the expected as in [30, 31] may hardly be justified. We therefore investigated a resamplingbased approach by directly sampling from the pilot data at hand. To simulate a typical proteomics study, we randomly choose 7 samples of each gender from the total training set of 67 males and 67 females. From the 2 × 7 data, we used the bootstrap [32] to generate 2000 sample sets of different larger sizes (2 × 10 to 2 × 120) without any assumption about the underlying distribution of the sampled population. To take into account the multivariate aspect of the problem, we ask for the sample size required for declaring all the markers significant while controlling the FDR at 0.05 using the BH procedure. This is equivalent to conducting the single tests at a more stringent "average type one error" α_{ave}. Using the result [24]
where (1  β)_{ave} is the average power for a single marker (set e.g. to 0.9), q is the expected value of the false discovery rate, i.e. q = E(FDR), and π_{0} is the proportion of markers that are differentially non expressed (true null). To estimate π_{0} we use the method described in [33] and fit the observed distribution of the Wilcoxon pvalues to the following two component model
with f_{0}(p) being the density of the null features (that is the differentially non expressed markers) is given by the uniform distribution U(0, 1), whereas f_{ A }(p) is the alternative density for the differentially expressed markers. Hence we may write
This resulted in a estimate π_{0} = 0.5652831 which plugged into Equation 1 leads to α_{ave} = 0.00223.
To estimate N_{diff} we set the value of α_{ave} = 0.00223 to control the FDR at 0.05 and examined for biomarkers that can be declared significantly differentially distributed. WT was applied to each data set generated. Let $\mathcal{N}$ be the number of times the null hypothesis is rejected. Discarding 5% of $\mathcal{N}$ (the false positives) is essentially a power estimate. By examining the graphs as in Figure 4 the sample size required for any predefined power can be deduced. Obviously, the more precise the information about the effect size δ, the better the trial can be designed. If the sample size is "sufficiently large", then the central limit theorem guarantees that δ will be approximately normally distributed. The bootstrap provides a powerful tool to estimate the required differential sample size by directly sampling from the available data and has been shown to give an unbiased estimate of power [34]. However, the key issue here is that the available data be reliable and representative. In the absence of a reliable data set, bootstrapping is not appropriate [35].
In the above considerations, we opted for simplicity for the standard definition of the sample size as the minimum number of samples necessary to achieve a specified power. Alternatively, the "confidence probability formulation" [36] may also be used as it relies on the permutation of pilot study data of small sample sizes.
Estimation of the discriminative sample size
To estimate the effect of training sample size on a classifiers performance we employed learning curves [37]. We used the inverse powerlaw model
where E(Y_{train}) is the expected value of a performance metric, e.g. the misclassification error rate MER (MER = 1ACC, with ACC being the overall model accuracy) or the area above the curve AAC (AAC = 1AUC), given training sample size N_{train}. Γ is the minimum classification error that can be expected as N_{train} → ∞, the so called Bayes error which provides the lowest achievable error rate for a given pattern classification problem (Γ =Γ(∞)), γ is referred to as the learning rate, and β the scale. Using SVM classification, the learning curves for AAC and MER are given in Figure 5. SVM was chosen since this approach has been found to give the best or the near best performance for many microarray data sets [38]. For the actual male and female data, the fit resulted in the equations: $\text{AAC}=0.03+1.39\times {N}_{\text{train}}^{0.716}$ and $\text{MER}=0.02+1.052\times {N}_{\text{train}}^{0.597}$. From these equations the required sample size can easily be deduced. E.g. for reaching AAC or MER of 10%, N_{disc} = 65 and N_{disc} = 75, respectively. Hence, MER seems to overestimate the sample size N_{disc}, as this quantity holds only for a given threshold whereas the AAC gives a global measure for all thresholds. It is important to note that different classifiers will result in different estimates for the AAC and MER and hence another estimate of N_{disc} will be obtained.
In practice it is impossible to reach Γ and only upper bound estimates to it can be reached. The aim is to find the discriminative sample size N_{disc}, that guarantees that Γ (N_{disc}) of the classifier is within some threshold (e.g ϵ = 5%) from the optimal Bayes classifier obtained for infinite N_{disc} [39] (that is, Γ(∞)  Γ(N_{disc}) ≤ ϵ). N_{disc} may then be obtained by resolving the equation Γ(∞)  Γ(N_{disc}) = ϵ. Interestingly, here again the effect size δ turns out to be the parameter that determines N_{disc}. In the classification context, the effect size measures the distance between the classes. If the pilot study shows a small effect size then it is unlikely that a good discriminator will be easily obtained. The required N_{disc} that maximizes the Γ(N_{disc}) implicitly depends on the false positive rate α [39, 40]. Consequently, using those markers that control the FDR should generally produce a good classifier [39, 40]. For the 67 male and 67 female profiles, controlling the FDR at 0.05 we are able to define 78 significant peptide markers requiring an N_{diff} < 67. With their calculated effect sizes we found that N_{disc} = 48 is required to obtain a classifier with 10% performance short of the optimal Bayes classifier. The analytical method described in [39, 40] relies on strong distributional assumptions and seems to be less conservative than the learning curve estimation of N_{disc}.
Classification
Once a classification rule has been built, its performance must be evaluated. Frequently, complete leaveoneout cross validation (or similar approaches that all are a reflection of the classifier onto the training set) is employed for error estimation. We have investigated if such an approach is indeed appropriate. An SVMbased classifier was built, based on randomly selected 2 × 7, 2 × 20, 2 × 33 datasets, and the entire 2 × 67 cases and controls. As shown in Figure 6 assessment of the performance based on the complete leaveoneout cross validation (LOOCV) resulted in apparently excellent performance, with the classifier based on 7 cases and controls only appearing to be 100% correct. However, when the classifiers are then tested in the blinded dataset, the results of the classifiers that were built only on a small set of samples could not be verified. As expected, best performance was observed for the classifier based on all available data, where the results from the cross validation and the assessment in the independent dataset are quite similar. These data indicate that results based on the training set only remain questionable, evaluation in an independent set is indeed essential and the ultimate test any procedure must pass. This conclusion supports the findings of [41, 42] where the LOOCV error estimate was found to be biased for small samples sizes. For large sample sizes the LOOCV error estimates may be seen as reliable. Therefore we employed the independent test set consisting of 67 male and 67 female samples for evaluation of the performance of all classifiers. The classification results are reported in Table 3. The results suggest that the performance of many machine learning algorithms is quite similar and outperforms a simple tree model. Table 3 also suggests that the use of a generalized linear model (GLM) may not be suitable for similar data. GLM, and the tree model seem to be the more sensitive to the variability and the censored structure of the data.
Applications to the CDDN case study
To further test the applicability of the reported methods we investigated the difference between CD and DN patients using a data set of 120 CD and 120 DN subjects randomly split into 2 60 training and 2 × 60 test datasets (data available as Additional file 3 and Additional file 4). The differences in this dataset are much more pronounced than the malefemale case (Additional file 5). Using the 2 × 60 training data and 10 different random splits we found that on average 447 peptides may be declared differentially expressed using the adjusted WT. 65% of those markers could be validated in the test data (Additional file 6). The fact that using a pilot study of larger size results in more markers being declared significant clearly applies here too, as readily seen from the figure in the Additional file 7. The learning curve of this dataset also shows clearly the inverse power law behaviour (Figure in Additional file 8) and suggests that for the CDDN case fewer subjects than in the malefemale comparison may be required to obtain a classification of comparable performance.
Conclusions
In this report we have examined what requirements have to be met in order to identify significant proteomic biomarkers and establish classifiers that have a high probability of being valid and can be generalized. To avoid misinterpretation: we did not aim at actually identifying biomarkers that we claim to be genderassociated. The aim of this study was purely to analyse and delineate approaches which ensure a robust study design. In addition, we realize that a study aiming at the identification of biomarkers for classifiers is associated with further challenges, like the above mentioned verification bias. However, some of the main challenges in biomarker discovery may best be investigated using a well defined experimental system, as the one chosen here. In regard to the first major challenge: how to improve the detection of biomarkers clearly associated to disease, we show that the WT test seems to be best suited for this challenge. However, it also is evident that statistical analysis must be adjusted for multiple testing [43], and we demonstrate the deleterious effects of the avoidance of multiple testing. This effect is even more pronounced when only a small number of samples is being used for the analysis. The unadjusted pvalues obtained from a small sample set are essentially meaningless, and are not at all connected with the probability of a certain molecule to be a true biomarker in the test set. In fact, the commonly made silent assumption that among the apparently significant biomarkers (based on unadjusted testing), true significant biomarkers can be found with higher probability than in the apparently nonsignificant group, could not be verified (data not shown). In our dataset the actual significant features were evenly distributed in these two artificial groups (unadjusted pvalues below and above 0.05), which are only generated due to inappropriate statistics, hence they should be considered to be artefacts. This again underlines the notion that unadjusted pvalues should not be reported in the absence of other evidence. The lack of statistical power, as well as the unadjusted pvalues that erroneously are often considered significant, are mostly a consequence of an incorrect estimation of the true distribution. Due to the relatively high variability observed (in the datasets employed here mostly due to biological variability), the true mean cannot be correctly assessed based on a small set of samples. The incorrect distribution suggests significant differences, which in fact are not true. Only upon investigation of a sufficiently large number of samples can the true mean in the cases and controls be determined. This is also evident from the example shown in Figure 7. We also show that confidence in the identified biomarkers can be further improved by resampling of the data, thereby generating a larger number of experiments. Biomarkers that appear significant in each of these experiments, are likely also significant in an independent test set, hence can be generalized. While such a strategy clearly comes at a cost: the number of biomarkers identified is significantly lower, this strategy may nevertheless represent a preferred option to define likely valid biomarkers, due to the high level of confidence that can be reached. Based on a representative proteomic data set, we also presented methods for answering the second important question: how to estimate the required sample size, both for class comparison (differential sample size) and subject classification (discriminative sample size). Our data demonstrate that estimation of the differential sample size required for achieving significance in detecting a certain number of specific biomarkers is possible based on resampling from a relatively small dataset. While we have successfully employed only 7 cases and controls, it seems advisable to slightly increase this number to 12 [44]. A similar strategy may be adopted for estimating the discriminative sample size required for achieving a predefined confidence of a given classifier. Based on the data subsequently obtained, we used the approach of fitting learning curves. This approach may result in an overestimation of the required discriminative sample size. This is in fact beneficial, as it will generally avoid the initiation of an underpowered study. Our data also indicate that testing of biomarkers (e.g. by assessing the pvalue) or biomarker models (e.g. by cross validation) in the training set will likely result in an overestimation of their quality. As a consequence, it appears that the quality of biomarkers or combinations thereof can only be addressed with confidence in an independent test set. Even when analysing a significant number of samples, statistics appears to overestimate the value of the potential biomarkers. Statistics is based on the assumption of an even distribution of the features across the training and test sets, that the findings can be generalized, and on the association with (in our example) gender only. This is apparently not even the case when using the data from 134 cases and controls. The expected result, that 95% of the significant biomarkers should stay significant in the test set, could not be observed. This may indicate that additional variables influence the outcome, and result in an overestimation of the statistical value. Especially when sample sizes are small, even statistically valid results must be interpreted with caution. In such situations, findings should be viewed as tentative and exploratory rather than conclusive. Our results further reveal that different machine learning algorithms perform similarly well, and seem to outperform linear classifiers. However, we could also clearly demonstrate that the assessment of the performance of such a classifier can only be performed on an independent test set, the results obtained from the training set (even when performing leaveoneout cross validation) may be misleading. Based on the data presented here, it appears advisable to begin a study aiming at identification of biomarkers or classifiers by performing an analysis of 12 cases and controls, estimate sample size required for certain performance (e.g. accuracy of classification, level of confidence for biomarkers) based on resampling, and then perform the actual study with a sufficiently large set of samples. Potential biomarkers must pass WT, adjusted for multiple testing, preferably consistently when employing a set of > 30 resamples that each contain e.g. 70% of the available data. Classifiers are best established employing any of the available machine learning algorithms. The validity of both, biomarkers and classifiers, is generally overestimated in the training set, hence can only be addressed with confidence in an independent test set. The methods proposed here are independent on which clinical readout is considered. This fact has been shown by applying them to a dataset composed from diabetes type II either with normal kidney function or diabetic nephropathy. This last case study shows that the malefemale case is reasonably representative of situations where the search for biomarkers and the classification tasks are rather involved.
Methods
Patients, Procedures and Demographics
Second morning urine samples were collected from apparently healthy volunteers in the course of the medical examination prior to employment at the Hannover Medical School. Consent was given by all participants. Samples were collected in 10 ml Sarstedt urine monovettes and frozen immediately after collection without the addition of any preservatives. All samples were collected anonymously, only age and gender were recorded. All samples were collected in Germany, and under German law this study does not require IRB approval.
Sample preparation and CEMS analysis
Urine samples were stored at 20°C for up to 3 years until analysis. For proteomic analysis, a 0.7 mL aliquot of urine was thawed immediately before use and diluted with 0.7 ml of 2 M urea, 10 mM NH4OH containing 0.02% SDS. To remove higher molecular mass proteins, samples were filtered using Centrisart ultracentrifugation filter devices (20 kDa molecular weight cutoff; Sartorius, Goettingen, Germany) at 3,000 rcf until 1.1 ml of filtrate was obtained. This filtrate was applied onto a PD10 desalting column (Amersham Bioscience, Uppsala, Sweden) equilibrated in 0.01% NH4OH in HPLCgrade H2O (Roth, Germany) to remove urea, electrolytes, and salts. Finally, all samples were lyophilized, stored at 4°C, and suspended in HPLCgrade H2O shortly before CEMS analysis, as described in [45]. CEMS analysis was performed as described [45, 46] using a P/ACE MDQ capillary electrophoresis system (Beckman Coulter, Fullerton, USA) online coupled to a MicroTOF MS (Bruker Daltonic, Bremen, Germany). Data acquisition and MS acquisition methods were automatically controlled by the CE via contactcloserelays. The ESI spectra were accumulated every 3 s, over a range of m/z 350 to 3000 Th. Accumulation time has been chosen to be 3 s, since at peak width of ca. 15 sec at half peak height, essentially no resolution is lost when accumulating signal for 3 s. Faster sampling would result in any additional gain, but in loss in sensitivity, and also increase in the size of the data file. Accuracy, precision, selectivity, sensitivity, reproducibility, and stability are described in detail elsewhere [10, 17, 45]. In short, the detection limit is in the range of 1 fmol, depending on the ionization properties of the individual peptide. This corresponds to 100  1000 fmol/ml in a crude urine sample (before processing).
Data processing
Mass spectral ion peaks representing identical molecules at different charge states were deconvoluted into single masses using MosaiquesVisu software [47]. Migration time and ion signal intensity (amplitude) were normalized based on 29 collagen fragments that serve as internal standards [17]. These internal polypeptide standards are the result of normal biological processes and have proven to be unaffected by any disease state studied to date (greater than 10,000 samples analysed to date) [48]. The resulting peak list characterizes each peptide by its molecular mass [Da], normalized migration time [min], and normalized signal intensity. All detected peptides were deposited, matched, and annotated in a Microsoft SQL database, allowing further analysis and comparison of multiple samples (patient groups). To establish the identity of peptides observed in different samples, a linear function was employed that allowed, depending on the mass of the polypeptide, a 50 ppm absolute mass deviation for peptides of 800 Da that increased linearly to 100 ppm absolute mass deviation for peptides with a maximum mass of 20 kDa. These values have been found appropriate in several recent studies [11, 49, 50], as a compromise between avoiding erroneous assignment of the same identity to two different peptides, and assigning two different identities to the same peptide in different analyses, due to mass deviation, especially at low abundance. A similar linear function was used when comparing CE migration times, allowing a 4% absolute deviation. CEMS data of all individual samples can be accessed in Additional files 1, 2.
Statistical methods, definition of biomarkers and sample classification
All the statistical analyses were implemented with internal scripts, using the R core software [51] as well as the contributed cranpackages ada, Kernlab, RandomForest, rpart, WilcoxCv, multtest, and ROCR available at http://cran.us.rproject.org.
Authors' information
Joost P Schanstra, Antonia Vlahou and Harald Mischak are all members of EUROKUP
Abbreviations
 1) AUC:

area under the ROC curve
 2) AAC:

area above the ROC curve
 3) BH:

BenjaminiHochberg
 4) CEMS:

capillary electrophoresis coupled mass spectrometry
 5) CD:

diabetes type II with normal kidney function
 6) DN:

diabetic nephropathy
 7) ESI:

electrospray ionization
 8) FDR:

false discovery rate
 9) GLM:

generalized linear model
 10) LCMS:

liquid chromatography coupled mass spectrometry
 11) LOD:

limit of detection
 12) LOOCV:

leaveoneout cross validation
 13) MALDI:

matrix assisted laser desorption ionization
 14) MER:

misclassification error rate
 15) N_{diff}:

differential sample size
 16) N_{disc}:

discriminative sample size
 17) ROC:

receiver operating characteristic
 18) SQL:

structured query language
 19) SVM:

support vector machine
 20) WT:

Wilcoxon rank sum test.
References
 1.
Rifai N, Gillette MA, Carr SA: Protein biomarker discovery and validation: the long and uncertain path to clinical utility. Nat Biotechnol 2006, 24(8):971–83. [Rifai1, Nader Gillette, Michael A Carr, Steven A Research Support, N.I.H., Extramural Research Support, NonU.S. Gov't Review United States Nature biotechnology Nat Biotechnol. 2006 Aug;24(8):97183.] 10.1038/nbt1235
 2.
Listgarten J, Emili A: Practical proteomic biomarker discovery: taking a step back to leap forward. Drug Discov Today 2005, 10(23–24):1697–702. 10.1016/S13596446(05)036457
 3.
Petricoin EF, Ardekani AM, Hitt BA, Levine PJ, Fusaro VA, Steinberg SM, Mills GB, Simone C, Fishman DA, Kohn EC, Liotta LA: Use of proteomic patterns in serum to identify ovarian cancer. Lancet 2002, 359(9306):572–7. 10.1016/S01406736(02)077462
 4.
McLerran D, Grizzle WE, Feng Z, Thompson IM, Bigbee WL, Cazares LH, Chan DW, Dahlgren J, Diaz J, Kagan J, Lin DW, Malik G, Oelschlager D, Partin A, Randolph TW, Sokoll L, Srivastava S, Thornquist M, Troyer D, Wright GL, Zhang Z, Zhu L, Semmes OJ: SELDITOF MS whole serum proteomic profiling with IMAC surface does not reliably detect prostate cancer. Clin Chem 2008, 54: 53–60. 10.1373/clinchem.2007.091496
 5.
Diamandis EP: Point: Proteomic patterns in biological fluids: do they represent the future of cancer diagnostics? Clin Chem 2003, 49(8):1272–5. 10.1373/49.8.1272
 6.
Ransohoff DF: Bias as a threat to the validity of cancer molecularmarker research. Nat Rev Cancer 2005, 5(2):142–9. 10.1038/nrc1550
 7.
Mischak H, Apweiler R, Banks RE, Conaway M, Coon J, Dominiczak A, Ehrich JHH, Fliser D, Girolami M, Hermjakob H, Hochstrasser D, Jankowski J, Julian BA, Kolch W, Massy ZA, Neusuess C, Novak J, Peter K, Rossing K, Schanstra J, Semmes OJ, Theodorescu D, Thongboonkerd V, Weissinger EM, Van Eyk JE, Yamamoto T: Clinical proteomics: A need to define the field and to begin to set adequate standards. PROTEOMICS  Clinical Applications 2007, 1(2):148–156. [http://dx.doi.org/10.1002/prca.200600771] 10.1002/prca.200600771
 8.
Decramer S, Gonzalez de Peredo A, Breuil B, Mischak H, Monsarrat B, Bascands JL, Schanstra JP: Urine in clinical proteomics. Mol Cell Proteomics 2008, 7(10):1850–62. 10.1074/mcp.R800001MCP200
 9.
Fliser D, Novak J, Thongboonkerd V, Argiles A, Jankowski V, Girolami MA, Jankowski J, Mischak H: Advances in Urinary Proteome Analysis and Biomarker Discovery. J Am Soc Nephrol 2007, 18(4):1057–1071. [http://jasn.asnjournals.org/cgi/content/abstract/18/4/1057] 10.1681/ASN.2006090956
 10.
Haubitz M, Good DM, Woywodt A, Haller H, Rupprecht H, Theodorescu D, Dakna M, Coon JJ, Mischak H: Identification and validation of urinary biomarkers for differential diagnosis and evaluation of therapeutic intervention in antineutrophil cytoplasmic antibodyassociated vasculitis. Mol Cell Proteomics 2009, 8(10):2296–307. 10.1074/mcp.M800529MCP200
 11.
Good DM, Zürbig P, Argilés n, Bauer HW, Behrens G, Coon JJ, Dakna M, Decramer S, Delles C, Dominiczak AF, Ehrich JHH, Eitner F, Fliser D, Frommberger M, Ganser A, Girolami MA, Golovko I, Gwinner W, Haubitz M, HergetRosenthal S, Jankowski J, Jahn H, Jerums G, Julian BA, Kellmann M, Kliem V, Kolch W, Krolewski AS, Luppi M, Massy Z, Melter M, Neusüss C, Novak J, Peter K, Rossing K, Rupprecht H, Schanstra JP, Schiffer E, Stolzenburg JU, Tarnow L, Theodorescu D, Thongboonkerd V, Vanholder R, Weissinger EM, Mischak H, SchmittKopplin P: Naturally Occurring Human Urinary Peptides for Use in Diagnosis of Chronic Kidney Disease. Molecular and Cellular Proteomics 2010, 9(11):2424–2437. [http://www.mcponline.org/content/9/11/2424.abstract] 10.1074/mcp.M110.001917
 12.
Mischak H, Allmaier G, Apweiler R, Attwood T, Baumann M, Benigni A, Bennett SE, Bischo R, BongcamRudloff E, Capasso G, Coon JJ, DHaese P, Dominiczak AF, Dakna M, Dihazi H, Ehrich JH, FernandezLlama P, Fliser D, Frokiaer J, Garin J, Girolami M, Hancock WS, Haubitz M, Hochstrasser D, Holman RR, Ioannidis JPA, Jankowski J, Julian BA, Klein JB, Kolch W, Luider T, Massy Z, Mattes WB, Molina F, Monsarrat B, Novak J, Peter K, Rossing P, SanchezCarbayo M, Schanstra JP, Semmes OJ, Spasovski G, Theodorescu D, Thongboonkerd V, Vanholder R, Veenstra TD, Weissinger E, Yamamoto T, Vlahou A: Recommendations for Biomarker Identification and Qualification in Clinical Proteomics. Science Translational Medicine 2010, 2(46):46ps42. [http://stm.sciencemag.org/content/2/46/46ps42.abstract] 10.1126/scitranslmed.3001249
 13.
Alonzo TA, Kittelson JM: A novel design for estimating relative accuracy of screening tests when complete disease verification is not feasible. Biometrics 2006, 62(2):605–12. [Alonzo, Todd A Kittelson, John M R01 GM54438/GM/NIGMS NIH HHS/United States Comparative Study Research Support, N.I.H., Extramural Research Support, NonU.S. Gov't United States Biometrics Biometrics. 2006 Jun;62(2):605–12.] [Alonzo, Todd A Kittelson, John M R01 GM54438/GM/NIGMS NIH HHS/United States Comparative Study Research Support, N.I.H., Extramural Research Support, NonU.S. Gov't United States Biometrics Biometrics. 2006 Jun;62(2):60512.] 10.1111/j.15410420.2005.00445.x
 14.
Buzoianu M, Kadane JB: Adjusting for verification bias in diagnostic test evaluation: a Bayesian approach. Stat Med 2008, 27: 2453–2473. 10.1002/sim.3099
 15.
Page JH, Rotnitzky A: Estimation of the diseasespecific diagnostic marker distribution under verification bias. Computational Statistics and Data Analysis 2009, 53(3):707–717. [http://www.sciencedirect.com/science/article/B6V8V4SX9FTT1/2/a708b210a358c83a359bd1c2ca7bef7f] 10.1016/j.csda.2008.06.021
 16.
Mischak H, Coon JJ, Novak J, Weissinger EM, Schanstra JP, Dominiczak AF: Capillary electrophoresismass spectrometry as a powerful tool in biomarker discovery and clinical diagnosis: an update of recent developments. Mass Spectrom Rev 2009, 28(5):703–24. 10.1002/mas.20205
 17.
JantosSiwy J, Schiffer E, Brand K, Schumann G, Rossing K, Delles C, Mischak H, Metzger J: Quantitative urinary proteome analysis for biomarker evaluation in chronic kidney disease. J Proteome Res 2009, 8: 268–81. 10.1021/pr800401m
 18.
Wang P, Tang H, Zhang H, Whiteaker J, Paulovich AG, Mcintosh M: Normalization regarding nonrandom missing values in highthroughput mass spectrometry data. Pac Symp Biocomput 2006, 315–326. full_text
 19.
Helsel R: Nondetects and data analysis: statistics for censored environmental data. New York: WileyInterscience; 2005.
 20.
Taylor S, Pollard K: Hypothesis tests for pointmass mixture data with application to 'omics data with many zero values. Stat Appl Genet Mol Biol 2009, 8: Article 8.
 21.
Broadhurst D, Kell D: Statistical strategies for avoiding false discoveries in metabolomics and related experiments. Metabolomics 2006, 2(4):171–196. [http://dx.doi.org/10.1007/s11306–006–0037z] 10.1007/s113060060037z
 22.
Dakna M, He Z, Yu WC, Mischak H, Kolch W: Technical, bioinformatical and statistical aspects of liquid chromatographymass spectrometry (LCMS) and capillary electrophoresismass spectrometry (CEMS) based clinical proteomics: a critical assessment. J Chromatogr B Analyt Technol Biomed Life Sci 2009, 877: 1250–1258. 10.1016/j.jchromb.2008.10.048
 23.
Oberg AL, Vitek O: Statistical Design of Quantitative Mass SpectrometryBased Proteomic Experiments. Journal of Proteome Research 2009, 8(5):2144–2156. 10.1021/pr8010099
 24.
Benjamini Y, Hochberg Y: Controlling the False Discovery Rate: A Practical and Powerful Approach to Multiple Testing. Journal of the Royal Statistical Society. Series B (Methodological) 1995, 57: 289–300. [http://vorlon.case.edu/~sray/mlrg/controlling_fdr_benjamini95.pdf]
 25.
Hemelrijk J: Note on Wilcoxon's TwoSample Test when Ties are Present. Annals of Mathematical Statistics 1952, 23: 133–135. 10.1214/aoms/1177729491
 26.
Soares AJ, Santos M, Trugilho M, NevesFerreira A, Perales J, Domont G: Differential proteomics of the plasma of individuals with sepsis caused by Acinetobacter baumannii. Journal of Proteomics 2009, 73(2):267–278. [http://www.sciencedirect.com/science/article/B8JDC4X9NVD1–1/2/e97759e56b52f471a9361b9d05d3072b] 10.1016/j.jprot.2009.09.010
 27.
Matsubara J, Ono M, Honda K, Negishi A, Ueno H, Okusaka T, Furuse J, Furuta K, Sugiyama E, Saito Y, Kaniwa N, Sawada J, Shoji A, Sakuma T, Chiba T, Saijo N, Hirohashi S, Yamada T: Survival Prediction for Pancreatic Cancer Patients Receiving Gemcitabine Treatment. Molecular and Cellular Proteomics 2010, 9(4):695–704. [http://www.mcponline.org/content/9/4/695.abstract] 10.1074/mcp.M900234MCP200
 28.
Ma Y, Peng J, Huang L, Liu W, Zhang P, Qin H: Searching for serum tumor markers for colorectal cancer using a 2D DIGE approach. Electrophoresis 2009, 30(15):2591–2599. 10.1002/elps.200900082
 29.
Altman DMD, TN B, MJ G: Statistics with Confidence: Confidence intervals and statistical guidelines. 2nd edition. London: BMJ Books; 2000.
 30.
Cairns DA, Barrett JH, Billingham LJ, Stanley AJ, Xinarianos G, Field JK, Johnson PJ, Selby PJ, Banks RE: Sample size determination in clinical proteomic profiling experiments using mass spectrometry for class comparison. Proteomics 2009, 9: 74–86. 10.1002/pmic.200800417
 31.
Jackson D, Herath A, Swinton J, Bramwell D, Chopra R, Hughes A, Cheeseman K, Tonge R: Considerations for powering a clinical proteomics study: Normal variability in the human plasma proteome. PROTEOMICS  CLINICAL APPLICATIONS 2009, 3(3):394–407. 10.1002/prca.200800066
 32.
Efron B, Tibshirani R: An Introduction to the Bootstrap. Boca Raton: Chapman & Hall/CRC; 1993.
 33.
Strimmer K: A unified approach to false discovery rate estimation. BMC Bioinformatics 2008, 9: 303. 10.1186/147121059303
 34.
Lesaffre E, Scheys I, Frohlich J, Bluhmki E: Calculation of power and sample size with bounded outcome scores. Stat Med 1993, 12: 1063–1078.
 35.
Walters SJ: Sample size and power estimation for studies with health related quality of life outcomes: a comparison of four methods using the SF36. Health Qual Life Outcomes 2004, 2: 26. 10.1186/14777525226
 36.
Lin WJ, Hsueh HM, Chen JJ: Power and sample size estimation in microarray studies. BMC Bioinformatics 2010, 11: 48. 10.1186/147121051148
 37.
Mukherjee S, Tamayo P, Rogers S, Rifkin R, Engle A, Campbell C, Golub TR, Mesirov JP: Estimating dataset size requirements for classifying DNA microarray data. J Comput Biol 2003, 10(2):119–42. 10.1089/106652703321825928
 38.
Kenneth RH, Caimiao W: Learning Curves in Classification With Microarray Data. Seminars in oncology 2010, 37: 65–68. 10.1053/j.seminoncol.2009.12.002
 39.
Dobbin KK, Zhao Y, Simon RM: How large a training set is needed to develop a classifier for microarray data? Clin Cancer Res 2008, 14: 108–14. 10.1158/10780432.CCR070443
 40.
Dobbin KK, Simon RM: Sample size planning for developing classifiers using highdimensional DNA microarray data. Biostatistics 2007, 8: 101–117. 10.1093/biostatistics/kxj036
 41.
BragaNeto UM, Dougherty ER: Is crossvalidation valid for smallsample microarray classification? Bioinformatics 2004, 20(3):374–80. 10.1093/bioinformatics/btg419
 42.
Molinaro AM, Simon R, Pfeiffer RM: Prediction error estimation: a comparison of resampling methods. Bioinformatics 2005, 21(15):3301–7. 10.1093/bioinformatics/bti499
 43.
Dudoit S, van der Laan M: Multiple Testing Procedures with Applications to Genomics. New York: Springer; 2008.
 44.
Hogg R, Tannis E: Probability and Statistical Inference. 8th edition. Prentice Hall: Pearson; 2010.
 45.
Theodorescu D, Wittke S, Ross MM, Walden M, Conaway M, Just I, Mischak H, Frierson HF: Discovery and validation of new protein biomarkers for urothelial cancer: a prospective analysis. Lancet Oncol 2006, 7(3):230–40. 10.1016/S14702045(06)705848
 46.
Wittke S, Mischak H, Walden M, Kolch W, Radler T, Wiedemann K: Discovery of biomarkers in human urine and cerebrospinal fluid by capillary electrophoresis coupled to mass spectrometry: towards new diagnostic and therapeutic approaches. Electrophoresis 2005, 26(7–8):1476–87. 10.1002/elps.200410140
 47.
Neuhoff N, Kaiser T, Wittke S, Krebs R, Pitt A, Burchard A, Sundmacher A, Schlegelberger B, Kolch W, Mischak H: Mass spectrometry for the detection of differentially expressed proteins: a comparison of surfaceenhanced laser desorption/ionization and capillary electrophoresis/mass spectrometry. Rapid Commun Mass Spectrom 2004, 18(2):149–56. 10.1002/rcm.1294
 48.
Coon JJ, Zurbig P, Dakna M, Dominiczak AF, Decramer S, Fliser D, Frommberger M, Golovko I, Good DM, HergetRosenthal S, Jankowski J, Julian BA, Kellmann M, Kolch W, Massy Z, Novak J, Rossing K, Schanstra JP, Schiffer E, Theodorescu D, Vanholder R, Weissinger EM, Mischak H, SchmittKopplin P: CEMS analysis of the human urinary proteome for biomarker discovery and disease diagnostics. Proteomics Clin Appl 2008, 2: 964. 10.1002/prca.200800024
 49.
Alkhalaf A, Zürbig P, Bakker SJL, Bilo HJG, Cerna M, Fischer C, Fuchs S, Janssen B, Medek K, Mischak H, Roob JM, Rossing K, Rossing P, Rychlík I, Sourij H, Tiran B, WinklhoferRoob BM, Navis GJ, for the PREDICTIONS Group: Multicentric Validation of Proteomic Biomarkers in Urine Specific for Diabetic Nephropathy. PLoS ONE 2010, 5(10):e13421. [http://dx.doi.org/10.1371%2Fjournal.pone.0013421] 10.1371/journal.pone.0013421
 50.
Maahs DM, Siwy J, Argilés n, Cerna M, Delles C, Dominiczak AF, Gayrard N, Iphöfer A, Jänsch L, Jerums G, Medek K, Mischak H, Navis GJ, Roob JM, Rossing K, Rossing P, Rychlík I, Schiffer E, Schmieder RE, Wascher TC, WinklhoferRoob BM, Zimmerli LU, Zürbig P, SnellBergeon JK: Urinary Collagen Fragments Are Significantly Altered in Diabetes: A Link to Pathophysiology. PLoS ONE 2010, 5(9):e13051. [http://dx.doi.org/10.1371%2Fjournal.pone.0013051] 10.1371/journal.pone.0013051
 51.
R Development Core Team: R: A Language and Environment for Statistical Computing.R Foundation for Statistical Computing, Vienna, Austria; 2010. [http://www.Rproject.org] [ISBN 3900051070]
Acknowledgements
This work was funded in part by grants from the European Union through InGenious HyperCare (LSHMC72006037093) and Geninca (HEALTHF22008202230) to HM and the EuroKUP COST Action (BM0702) and AV from the FP7 DECanBio (201333) and by the European Community's 7th Framework Programme, grant agreement HEALTHF22009241544 (SysKID). JPS acknowledges financial support from the Agence Nationale pour la Rechérche (ANR07PHYSIO00401), and support by Inserm, the "Direction Régional Clinique" (CHU de Toulouse, France) under the Interface program. WK is supported by the Science Foundation Ireland under Grant No. 06/CE/B1129.
Author information
Affiliations
Corresponding author
Additional information
Authors' contributions
All authors participated in the design of the study. MD and HM performed the statistical analysis. HM performed the CEMS analysis and initial data evaluation. AK, KH, SC, MD, and MG developed the high dimensional models. JPS and MH were involved in the recruitment of study participants. All authors were involved in drafting the manuscript, have read and approved the final manuscript.
Electronic supplementary material
Training set data file for the malefemale study
Additional file 1: . The pivot table CEMSmalefemaletrain.xls contains the amplitudes of each peptide in the 67 males (labelled as M...) and 67 females (labelled as F...) used for defining the biomarkers and training the classifiers for different N_{train}. The pivot tables also contain a worksheet named "Peptides assignment" that shows the mass (Mass, in Da) and migration time (CETime, in min) of peptides assigned to a certain Pep:ID, which is subsequently utilized as the unique identifier in the database. (XLS 1 MB)
Test set data file for the malefemale study
Additional file 2: . The table CEMSmalefemaletest.xls contains the amplitudes in the 67 males and 67 females used for testing the concordance of the biomarkers and estimating the errors of different classifiers. The pivot tables also contain a worksheet named "Peptides assignment" that shows the mass (Mass, in Da) and migration time (CETime, in min) of peptides assigned to a certain Pep:ID, which is subsequently utilized as the unique identifier in the database. (XLS 1 MB)
Training set data file for the CDDN study
Additional file 3: . The pivot table CEMSDNCNtrain.xls contains the amplitudes of each peptide in the 60 DN (labelled as DN...) and 60 CD (labelled as CN...) used for defining the biomarkers and training the classifiers for different N_{train}. (XLS 1 MB)
Test set data file for the CDDN study
Additional file 4: . The table CEMSDNCNtest.xls contains the amplitudes in the 60 DN and 60 CD used for testing the concordance of the biomarkers and estimating the errors of different classifiers. (XLS 1 MB)
Typical effect size of a differentially expressed marker in CD versus DN case
Additional file 5: . The distribution of two peptides, ID:67632 (upper panel) and ID:48751 (lower panel), was investigated in the complete training set (2 × 60) and 1000 resampled distributions. Typical effect size δ = (μ_{CD}  μ_{DN})/σ (with μ_{CD} and μ_{DN} being the mean logarithmic intensity for a given peptide in the CD and DN populations, and σ the pooled standard deviation) is shown. Effect sizes as extreme as 4 and +8 are observed.(PDF 9 KB)
Concordance in the biomarkers using CDDN data set
Additional file 6: . The concordance of the markers defined using 60CD and 60DN subjects as training set in an independent test set of 60CD and 60DN is reported using 10 random splits of the total (2 × 120) data. On average, 447 markers are reported as being significant and 65% of them may be validated on average in the test data. (PDF 27 KB)
Number of significant markers depends on sample size
Additional file 7: . From the 2 × 60 training data, data sets of sizes N_{diff} ranging from 7 to 60 were built via resampling. At each sample size the number of significant biomarkers (defined as having a pvalue after BH adjustments < 0.05) is shown on the vertical axis. The procedure was repeated 10 times to generate the BoxWhisker plots. In all 10 experiments, no biomarkers could be declared significantly differentially expressed below a sample size of 7. (EPS 30 KB)
Learning curve estimation of
Additional file 8: N_{ disc }. Cohorts with sample sizes ranging from 2 × 7  2 × 58 (given on the xaxis) were arbitrarily generated out of the entire 2 × 60 CDDN training dataset. 20 repetitions were performed for each size cohort. An SVMbased classifier was built for each dataset and its performance was tested in the independent test set. In the left hand panel the area above the curve AAC (AAC = 1AUC) for each classifier is shown. The misclassification error rate MER is shown on the right. The red curves represent the mean AAC and mean MER. The inverse power law behaviour is obvious. (EPS 32 KB)
Authors’ original submitted files for images
Below are the links to the authors’ original submitted files for images.
Rights and permissions
About this article
Cite this article
Dakna, M., Harris, K., Kalousis, A. et al. Addressing the Challenge of Defining Valid Proteomic Biomarkers and Classifiers. BMC Bioinformatics 11, 594 (2010). https://doi.org/10.1186/1471210511594
Received:
Accepted:
Published:
Keywords
 Continuous Component
 Hannover Medical School
 Verification Bias
 Empirical Likelihood Ratio
 Training Sample Size