 Research
 Open Access
 Published:
Accommodating multiple potential normalizations in microbiome associations studies
BMC Bioinformatics volume 24, Article number: 22 (2023)
Abstract
Background
Microbial communities are known to be closely related to many diseases, such as obesity and HIV, and it is of interest to identify differentially abundant microbial species between two or more environments. Since the abundances or counts of microbial species usually have different scales and suffer from zeroinflation or overdispersion, normalization is a critical step before conducting differential abundance analysis. Several normalization approaches have been proposed, but it is difficult to optimize the characterization of the true relationship between taxa and interesting outcomes.
Results
To avoid the challenge of picking an optimal normalization and accommodate the advantages of several normalization strategies, we propose an omnibus approach. Our approach is based on a Cauchy combination test, which is flexible and powerful by aggregating individual p values. We also consider a truncated test statistic to prevent substantial power loss. We experiment with a basic linear regression model as well as recently proposed powerful association tests for microbiome data and compare the performance of the omnibus approach with individual normalization approaches. Experimental results show that, regardless of simulation settings, the new approach exhibits power that is close to the best normalization strategy, while controling the type I error well.
Conclusions
The proposed omnibus test releases researchers from choosing among various normalization methods and it is an aggregated method that provides the powerful result to the underlying optimal normalization, which requires tedious trial and error. While the power may not exceed the best normalization, it is always much better than using a poor choice of normalization.
Introduction and motivation
Microbial communities have been revealed to be closely related to many conditions, such as obesity [1,2,3], diabetes [4,5,6], and HIV [7,8,9]. With the development of highthroughput sequencing technologies enabling largescale microbiome studies, human microbiome profiling studies for health conditions and diseases are gaining more attention. A central objective of human microbiome profiling studies is to identify individual bacterial taxa related to host outcomes, exposures, or other variables of interest among the meta data. This provides an important understanding of the mechanisms underlying different outcomes as well as host responses to exposures and potential contribution to therapeutic interventions.
The most common approach for identifying individual taxa related to variables of interest is to test the association between the variable and the abundance of each taxon, one by one. Many differential abundance analysis approaches have been proposed based on the linear model [10, 11], phylogenetic tree [12, 13], and zeroinflated model [14,15,16]. Based on these tests, the p value for the association of each taxon is generated and statistical significance is determined after controlling for multiple testing. On the other hand, global association tests have also been proposed to accommodate general dependency patterns between overall microbiome composition and profiles of other types of genomic data, including kernelbased tests [17,18,19,20] and distancebased tests [21,22,23].
Unfortunately, intrinsic challenges of microbiome data often make it difficult to identify differentially abundant taxa. For example, a central challenge of microbiome profiling studies is the issue of differential library size (total counts per sample), which is difficult to control [24] and does not reflect actual differences in microbial communities. Undersampling in some individuals may also exacerbate zeroinflation and overdispersion, leading to substantial power loss [25].
Normalization, broadly defined, is a strategy for overcoming differences in library size [26]. Failure to harmonize library sizes can lead to a severe loss of power as the scale of assessed abundances is essentially different for each sample. Common approaches to normalization include scaling the observations to have a unit sum (such that the norm of the abundances for each sample is equal to 1—the original definition of normalization), and scaling by other measures of central tendency, among others (see [27]). Theoretically, as long as read depth is not systematically confounded with the variable of interest, analysis under any normalizations is valid. However, in addition to philosophical differences between different normalization approaches, different normalizations also implicitly specify the expected relationship between each taxon under consideration and the outcome. A normalization that results in a better characterization of the true relationship between taxa and outcomes will lead to better power. Yet, the best normalization (leading to the highest power) is difficult to ascertain, as this depends on the unknown true state of nature and may also be different depending on the taxon under consideration.
To address the challenge of picking a single, optimal normalization, we develop an omnibus approach wherein we consider analyzing the data under several different normalization strategies. We then aggregate the results from different normalization approaches while adjusting for the fact that different normalizations have been used, in order to prevent phacking. Our approach is based on a Cauchy Combination Test (CCT) [28] which allows aggregation of correlated p values (calculated under different normalizations). Simulations show that our approach often leads to power similar to, or exceeds, the best individual normalization strategy, while still protecting the false discovery rate.
Methods
We assume a study in which there are n samples on which p taxa are measured. Let the raw vector of abundances for the \(i^{th}\) sample be \(X_i\). For a given normalization \(\mathcal {T}(\cdot )\), we set \(\tilde{X}_i = \mathcal {T}(X_i)\) and \(\tilde{X} = \mathcal {T}(X) = [\mathcal {T}(X_1),\ldots , \mathcal {T}(X_n)]\). We further assume that there are J different normalizations that can be considered such that we have \(\mathcal {T}_1(\cdot ), \mathcal {T}_2(\cdot ), \ldots , \mathcal {T}_J(\cdot )\). We focus on the objective of identifying individual bacterial taxa as associated with the outcome of interest.
The fundamental challenge that we hope to address is that it is unclear which normalization to use. Different normalizations correspond to different interpretations and implications of different bacterial taxa. Consequently, we propose a strategy in which we consider multiple potential normalizations. In this section, we first describe different, commonly used normalization strategies before outlining the specific approach for implicating taxa across different normalization approaches. We further describe simulation settings for evaluating the power and type I error of our strategy.
Common normalization approaches
Normalization is an important step for reducing variability in the data due to differential library size. Some easily applicable normalization strategies include:

(i)
None \(\mathcal {T}(X_i) = X_i\).

(ii)
Rarefaction Each sample’s observed counts are subsampled such that the total count is the same for all samples.

(iii)
Total sum scaling (TSS) Observed counts are scaled by the sample’s library size (sum of counts).

(iv)
Cumulative sum scaling (CSS) Observed counts are scaled by the sum of counts up to a cutoff quantile^{Footnote 1}. (see details in [29]).

(v)
Center Log Ratio (CLR) transform Observed counts are divided by the geometric mean of the sample’s counts, then logtransformed.
Even though these normalization strategies work well under many settings, some concerns are discussed in the literature: artificial uncertainty in the subsampling step (rarefaction) [30], a bias in differential abundance estimates (TSS) [31], and uncertainty in the selection of quantile (CSS). Hence, it is difficult to find an optimal normalization approach and it depends on the unknown form of relationship between microbiome data and interesting outcomes.
Given the inherent challenge of selecting a single optimal normalization strategy, we propose to simply apply multiple normalization approaches. Specifically, for each choice of normalization, we apply a valid statistical test to get the p value for the association between each taxon and the variable of interest. In the next section, we describe how we combine the p values to get a single omnibus p value for each taxon.
Combining results across normalizations via the cauchy combination test
Assume that after applying each normalization, we apply a valid test to assess the association between each taxon and the variable of interest such that we have a \(J\times p\) matrix of individual p values \({\textbf {P}}\) with \(p_{j,k}\), the p value for the \(k^{th}\) taxon after applying the \(j^{th}\) normalization strategy to the dataset.
Given \({\textbf {P}}\), we apply the Cauchy combination test (CCT) [28] for each taxon to obtain the omnibus p value. It is wellknown that the Cauchy combination test is useful for dealing with sparse alternatives, highdimensional largescale datasets, and small p values, which are common situations in GWAS. In particular, the analytic p value approximation by the Cauchy distribution is very accurate under arbitrary dependency structures. Hence, in practice, the test only requires the individual p values as input, so this omnibus testing procedure is very fast. Specifically, for \(k = 1, \ldots , p\), we set
to be the final p value for the kth taxon and \(p_{k}\) incorporates each normalization strategy.
Though CCT is convenient and exact for any number of p values, it suffers the drawback of sensitivity to p values at or near 1. Specifically, the Cauchy combination p value, \(p_{k}\), converges to 1 as one of \(p_{j,k}\) approaches 1 \((j = 1, \ldots , J)\). This can happen for tests of discrete data or when the model to derive p values is misspecified. To address this, we propose to use a truncated Cauchy combination test proposed by [32]:
where \(\epsilon = 0.01\). This prevents the overshoot of \(p_{k}\) over the threshold \(1\epsilon\).
Simulation setup
To check the performance of the method, we first follow the simulation setup in [16] using data generated to mimic a real data set. Specifically, we simulate data from the Coronary Artery Risk Development in Young Adults Study (CARDIA) [33] which aimed to investigate microbial taxa related to cardiovascular disease risk factors. The broader parent study [34] was balanced in terms of race (black or white), education (more than high school or not), and age. Between 1987 and 2016, each subject had up to eight followup visits. A variety of cardiovascular diseaserelated parameters, as well as physical measurements and lifestyle factors, were gathered.
We follow the preprocessing of [16] and focus on microbiome count data aggregated at the genuslevel. The processed data contains data on 106 genera for 549 subjects. Our goal is to identify differentially abundant taxa between subjects with high blood pressure (HBP) and without HBP and examine how powerful the omnibus approach is over individual normalization strategies. Here, we treat blood pressure as a binary variable (HBP vs. nonHBP). We then consider two scenarios based on unadjustment/adjustment for covariates:

Setting 1 (type I error and power of individuallevel analysis on a single taxon): We select ‘Streptococcus’ taxon, which is differentially abundant with strong differences in the mean abundance by HBP status, and test the association between the selected taxon and HBP without adjustment for other covariates. To assess the type I error rate, we generate 600 samples from the empirical distribution functions (edf) of the normalized abundance in subjects without HBP. To assess the power of the test, we generate 300 samples each from the edf of HBP and nonHBP groups. We also examine cases where the two groups are mixed by \(\delta\)% with each other. We simulate 10,000 datasets and the significance level is set to be 0.01.

Setting 2 (type I error and power of individuallevel analysis on an OTU table): We create the starting dataset by rarefying the CARDIA dataset 10 times and averaging the resulting datasets. With this starting data, we fit each of the genera by the twopart quantile regression model (see Additional file 1: Figure S1):
$$\begin{aligned} \text {logit}\{P(D=1X)\}&= \gamma _{0}+\gamma _{1}\text {HBP}+\gamma _{2}\text {age}+\gamma _{3}\text {physical activity} \\&\ \ \ \ +\gamma _{4}\text {diet quality score}, \\ Q_{Y}(\tau X,Y>0)&= \beta _{0}(\tau )+\beta _{1}(\tau )\text {HBP}+\beta _{2}(\tau )\text {age}+\beta _{3}(\tau )\text {physical activity} \\&\ \ \ \ +\beta _{4}(\tau )\text {diet quality score}, \end{aligned}$$where \(D = I(Y>0)\) is a binary indicator of the presence of genus, and \(\gamma _{i}\)’s and \(\beta _{i}\)’s are estimated by the starting data and nonzero observations of the starting data using \(\tau = 0.01,\ldots ,0.99\), respectively. To assess the type I error rate, we generate n samples by resampling each of the real covariates with replacement independently and simulate D with the constraint \(\gamma _{1}=\beta _{1}(\tau )=0\). If \(D=0\), we assign 0 as the count. If \(D=1\), we simulate the count by the inverse CDF method: compute \(Y=\beta _{0}(u)+\beta _{2}(u)\text {age}+\beta _{3}(u)\text {physical activity}+\beta _{4}(u)\text {diet quality score}\), where \(u\sim U(0,1)\) and round it to the nearest integer. To assess the power of the test, we follow the same procedure without the constraint. We simulate 1000 datasets and the significance level is set to be 0.05.
For each test, normalization strategies (i)–(v) are considered and we compare the omnibus p value with the p values based on each normalization strategy. To obtain the p values, we apply the simple linear regression, a zeroinflated quantile approach (ZINQ) proposed by [16], a quantile regression using a rank score function and ignoring zero inflation (QRank) proposed by [35]. In addition, the mixing rate \((\delta )\) and sample size (n) are chosen so that the results can be compared well between normalization strategies.
We also consider the simulation setup in [36] to examine the performance of the omnibus method by a global microbiome association test. Specifically, we generate n/2 genotype data of haplotypes from African and European ancestry by randomly pairing 2 haplotypes, respectively, over a 1 MB chromosome according to coalescent theory using the cosi2 program [37]. We also generate n samples of microbiome OTU counts from the Dirichletmultinomial distribution. We first estimate the parameters of the Dirichletmultinomial distribution using a real upperrespiratorytract microbiome dataset [38]. This dataset is publicly available by an \(\texttt {R}\) package \(\texttt {GUniFrac}\). This consists of 856 OTUs.

Setting 3 (type I error and power of communitylevel analysis on an OTU table): To assess the type I error rate, we use the above setting without introducing any genetic effect on the microbiome. To assess the power of the test, we introduce the association between genetics and microbiome. For each individual \(i = 1, \ldots , n\), let \(g_{i}\) be the genotype at a chosen common SNP (with MAF \(\ge\) 0.05). Then we increase the counts of the \(\eta\)th–20th most common OTUs by a factor \(f_{i} = 1 + 1.7*g_{i}\).
For each test, we use a kernel RV coefficient (KRV) test to evaluate the overall association between genetic expression and microbiome composition. [39, 40]. We use the BrayCurtis kernel and choose normalization strategies (i)–(iv) since CLR transformation provides negative results and this does not allow the KRV test. We simulate 1000 datasets and the significance level is set to be 0.05.
Results
Type I error
Table 1, 2, and 3 show the empirical size of the tests under Setting 1, 2, and 3, respectively. We see that the omnibus approach in general controls the type I error rate well, compared to other normalization approaches.
Power
Table 4, 5, and 6 show the estimated power of the tests under Setting 1, 2, and 3, respectively. Figure 1 shows their visualization. Under Setting 1, we see that CLR normalization exhibits the best performance, while rarefaction shows the worst performance. Within this gap, the omnibus approach exhibits power that is almost as high as the performance when using CLR normalization. On the other hand, under Setting 2, when applying the linear regression, CSS normalization exhibits high power, while the rarefaction approach shows the worst performance. Surprisingly, the omnibus approach exhibits the best performance, even over the CSS approach. When using ZINQ, rarefaction approach still shows the worst performance, while ZINQ achieves high power without normalization. The omnibus approach shows the best performance, the same as the linear regression case. When applying QRank, CLR approach exhibits high power, but the omnibus approach achieves the best power. Under Setting 3, the omnibus approach exhibits high power, while raw data and TSS normalization show good performance as well.
As shown in Table 4, 5, and 6, the best normalization strategy depends on different differential abundance methods and situations, and it is difficult to choose the optimal normalization strategy. However, the omnibus method generally performs well without prior or true relationship knowledge between taxa and outcomes, so this would be more efficient and useful when applying differential abundance tests in microbiome studies.
Real data application
In this section, we illustrate the omnibus approach on the HIV dataset analyzed in [41]. The HIV dataset is obtained by a multicolor flow cytometrybased method that separates neutrophils from other leukocytes in order to get a more precise measurement of neutrophil frequencies in the Gastrointestinal (GI) during HIV infection. This allows the identification of neurophils in blood and fresh GI issues and the calculation of the frequency of neutrophils as a percentage of all live CD45\(+\) cells.
As a result, this dataset consists of colorectal biopsies from a total of 40 HIVinfected, antiretroviral therapy (ART) suppressed individuals and 35 HIVuninfected individuals with relevant participant demographic information, such as age, sex, sexual orientation, and race/ethnicity. The authors characterized the intestinal microbiome of colorectal biopsies using 16S rRNA sequencing and studied the association between the mucosal microbiome composition of colorectal biopsies and some relevant factors. For example, based on the fact that men who have sex with men (MSM) have an increased abundance of Prevotella, independent of HIV status, and this may result in the dysbiosis previously attributed to HIV infection, the authors observed the significant association between the overall microbial composition at the genus level and sexual orientation (MSM or nonMSM). They also showed that this association remained when adjusted for age, race, and HIV status.
We utilize this dataset to illustrate how the omnibus approach accommodates several normalization strategies. Specifically, we conduct association tests between the mucosal microbiome composition of colorectal biopsies and the sexual orientation. According to the results in [41], we test the association with the sexual orientation without adjustment for other covariates or with adjustment for age, race, and HIV status. Here, we fix the false discovery rate (FDR) at 20%.
Table 7 shows the number of differentially abundant taxa out of 108 taxa based on the sexual orientation at 20% FDR. We see that the best normalization approach is different for each case, but the omnibus approach in general identifies nearly as many significant taxa as the best normalization approach.
We also assess type I error control based on permuted HIV datasets to check the validity of the omnibus test. For each normalization strategy, covariates as well as the sexual orientation are jointly permuted over the whole samples to create a permuted OTU table. This removes the association between the mucosal microbioal abundance and the sexual orientation, and taxa with small p values are considered false positive signals. We evaluate type I error control by the proportion of taxa with p values less than 0.1. We repeat this procedure 50 times and the results are presented via boxplots (Figs. 2 and 3). Compared to other normalization strategies, we see that the omnibus approach consistently controls the type I error rate well.
Discussion
We propose the omnibus approach to accommodate multiple potential normalization strategies. Essentially, each choice of normalization inherently assumes a different model for the relationship between taxa and variables of interest, with the optimal choice being unknown (and potentially differing across taxa). By using the omnibus approach, we can avoid the problem of choosing the optimal normalization strategy and instead test across a range of different normalization approaches. Numerical experiments and the real data application demonstrate that the omnibus test not only avoids the possibility of choosing the worstperforming normalization method but also exhibits power nearly as high as the power of the best normalization strategy.
Other factors, such as sequencing methods, amplicon bias, and target gene copy number could impact the differential abundance analysis results. However, they generate bias in microbiome sequencing, making measured relative abundances systematically different from their underlying truth. In this case, biasresistant modeling or biasinsensitive analytical methods are needed. However, the impact of bias is usually not handled via normalization approaches, and thus goes beyond the scope of this paper. This paper mainly handles the differences caused by differential library sizes that affect all taxa more or less evenly. The focus of this paper is to study whether the omnibus approach helps bypass the normalization issue in microbiome differential abundance testing.
Certain transformations, in principle, can reduce the impact of compositional effects. However, without extrinsic information, there ultimately remains a particular denominator for normalization. Thus, our approach does not seek to overcome the issue, but rather we note that the statistical analysis is “valid” under any choice of normalization and compositionality is an issue of subsequent interpretation. That is, interpretation of significant findings is affected by the compositionality of the data and potentially by the normalization approaches considered, but fully assessing the impact of compositionality on the omnibus test lies outside the scope of the present work.
In this paper, we focus on the linear regression, ZINQ, QRank, and KRV. We acknowledge that a wide range of alternative methods for differential abundance analysis could also be used [42,43,44]; however, many of these methods are specialized in particular normalizations. For example, a metagenomeSeq method proposed by [43] internally implements CSS normalization and a DESeq2 method proposed by [45] implements relative log expression (RLE) normalization. More importantly, many of these approaches often fail to control the type I error [26, 46, 47] and are, therefore, statistically invalid. In contrast, the simple linear regression, ZINQ, QRank, and KRV have been shown to consistently protect the type I error and do not depend on the particular choice of normalization. We could also combine results across different association testing methods, as well as normalizations, but given their lack of statistical validity, aggregating invalid results just results in further false positives.
In addition, we consider four normalization strategies, including the rarefaction, TSS, CSS, and CLR transformations. Other normalization methods are also commonly used, such as an additive logratio transformation (ALR) or an isometric logratio transformation (ILR) [48]. However, ALR is computed with respect to the last element of variables, so it heavily depends on this element and its noise. Though ILR has good theoretical properties, it is difficult to interpret the result since transformed variables are intricate mixtures of the original variables. To fairly examine the performance of our approach, we choose four normalization methods that are simpler and more flexible to use.
Availability of data and materials
Data used in this article is available from the CARDIA Study Data Coordinating Center at the University of Alabama at Birmingham. The process for obtaining data through CARDIA is outlined at https://www.cardia.dopm.uab.edu/publications2/publicationsdocuments. The HIV dataset and R scripts used during the current study are available from the corresponding author upon reasonable request. The main function code for the omnibus approach with an example code is available at https://github.com/hoseungs/Omnibus_normalization.
Notes
https://www.metagenomics.wiki/tools/16s/norm/css
Abbreviations
 CCT::

Cauchy combination test
 TSS::

Total sum scaling
 CSS::

Cumulative sum scaling
 CLR::

Center log ratio transformation
 CARDIA::

The coronary artery risk development in young adults study dataset
 HBP::

High blood pressure
 EDF::

Empirical distribution functions
 ART::

Antiretroviral therapy
 MSM::

Men who have sex with men
 FDR::

False discovery rate
 RLE::

Relative log expressions
References
Turnbaugh PJ, Ley RE, Mahowald MA, Magrini V, Mardis ER, Gordon JI. An obesityassociated gut microbiome with increased capacity for energy harvest. Nature. 2006;444(7122):1027–31.
John GK, Mullin GE. The gut microbiome and obesity. Curr Oncol Rep. 2016;18(7):1–7.
Maruvada P, Leone V, Kaplan LM, Chang EB. The human microbiome and obesity: moving beyond associations. Cell Host Microbe. 2017;22(5):589–99.
Hartstra AV, Bouter KE, Bäckhed F, Nieuwdorp M. Insights into the role of the microbiome in obesity and type 2 diabetes. Diabetes Care. 2015;38(1):159–65.
Komaroff AL. The microbiome and risk for obesity and diabetes. JAMA. 2017;317(4):355–6.
Vallianou NG, Stratigou T, Tsagarakis S. Microbiome and diabetes: Where are we now? Diabetes Res Clin Pract. 2018;146:111–8.
Saxena D, Li Y, Yang L, Pei Z, Poles M, Abrams WR, Malamud D. Human microbiome and HIV/AIDS. Curr HIV/AIDS Rep. 2012;9(1):44–51.
Bandera A, De Benedetto I, Bozzi G, Gori A. Altered gut microbiome composition in HIV infection: causes, effects and potential intervention. Curr Opin HIV AIDS. 2018;13(1):73–80.
Desai SN, Landay AL. HIV and aging: role of the microbiome. Curr Opin HIV AIDS. 2018;13(1):22–7.
Mallick H, Rahnavard A, McIver LJ, Ma S, Zhang Y, Nguyen LH, Tickle TL, Weingart G, Ren B, Schwager EH, et al. Multivariable association discovery in populationscale metaomics studies. PLoS Comput Biol. 2021;17(11):1009442.
Zhou H, He K, Chen J, Zhang X. Linda: linear models for differential abundance analysis of microbiome compositional data. Genome Biol. 2022;23(1):1–23.
Kim KJ, Park J, Park SC, Won S. Phylogenetic treebased microbiome association test. Bioinformatics. 2020;36(4):1000–6.
Huang C, Callahan BJ, Wu MC, Holloway ST, Brochu H, Lu W, Peng X, Tzeng JY. Phylogenyguided microbiome otuspecific association test (post). 2021.
Hu T, Gallins P, Zhou YH. A zeroinflated betabinomial model for microbiome data analysis. Stat. 2018;7(1):185.
Ai D, Pan H, Li X, Gao Y, Liu G, Xia LC. Identifying gut microbiota associated with colorectal cancer using a zeroinflated lognormal model. Front Microbiol. 2019;10:826.
Ling W, Zhao N, Plantinga AM, Launer LJ, Fodor AA, Meyer KA, Wu MC. Powerful and robust nonparametric association testing for microbiome data via a zeroinflated quantile approach (zinq). Microbiome. 2021;9(1):1–19.
Zhao N, Chen J, Carroll IM, RingelKulka T, Epstein MP, Zhou H, Zhou JJ, Ringel Y, Li H, Wu MC. Testing in microbiomeprofiling studies with Mirkat, the microbiome regressionbased kernel association test. Am J Human Genet. 2015;96(5):797–807.
Zhan X, Tong X, Zhao N, Maity A, Wu MC, Chen J. A smallsample multivariate kernel machine test for microbiome association studies. Genet Epidemiol. 2017;41(3):210–20.
Zhan X, Xue L, Zheng H, Plantinga A, Wu MC, Schaid DJ, Zhao N, Chen J. A smallsample kernel association test for correlated data with application to microbiome association studies. Genet Epidemiol. 2018;42(8):772–82.
Koh H, Li Y, Zhan X, Chen J, Zhao N. A distancebased kernel association test based on the generalized linear mixed model for correlated microbiome studies. Front Genet. 2019;10:458.
Chen J, Bittinger K, Charlson ES, Hoffmann C, Lewis J, Wu GD, Collman RG, Bushman FD, Li H. Associating microbiome composition with environmental covariates using generalized unifrac distances. Bioinformatics. 2012;28(16):2106–13.
Zhang Y, Han SW, Cox LM, Li H. A multivariate distancebased analytic framework for microbial interdependence association test in longitudinal study. Genet Epidemiol. 2017;41(8):769–78.
Zhang J, Wei Z, Chen J. A distancebased approach for testing the mediation effect of the human microbiome. Bioinformatics. 2018;34(11):1875–83.
Pan AY. Statistical analysis of microbiome data: the challenge of sparsity. Curr Opin Endoc Metab Res. 2021;19:35–40.
Chen L, Reeve J, Zhang L, Huang S, Wang X, Chen J. Gmpr: a robust normalization method for zeroinflated count data with application to microbiome sequencing data. PeerJ. 2018;6:4600.
Weiss S, Xu ZZ, Peddada S, Amir A, Bittinger K, Gonzalez A, Lozupone C, Zaneveld JR, VázquezBaeza Y, Birmingham A, et al. Normalization and microbial differential abundance strategies depend upon data characteristics. Microbiome. 2017;5(1):1–18.
Lin H, Peddada SD. Analysis of microbial compositions: a review of normalization and differential abundance analysis. NPJ Biofilms Microbiomes. 2020;6(1):1–13.
Liu Y, Xie J. Cauchy combination test: a powerful test with analytic pvalue calculation under arbitrary dependency structures. J Am Stat Assoc. 2020;115(529):393–402.
Flynn S, Reen FJ, CaparrósMartín JA, Woods DF, Peplies J, Ranganathan SC, Stick SM, O’Gara F. Bile acid signal molecules associate temporally with respiratory inflammation and microbiome signatures in clinically stable cystic fibrosis patients. Microorganisms. 2020;8(11):1741.
McMurdie PJ, Holmes S. Waste not, want not: why rarefying microbiome data is inadmissible. PLoS Comput Biol. 2014;10(4):1003531.
Dillies MA, Rau A, Aubert J, HennequetAntier C, Jeanmougin M, Servant N, Keime C, Marot G, Castel D, Estelle J, et al. A comprehensive evaluation of normalization methods for illumina highthroughput rna sequencing data analysis. Brief Bioinform. 2013;14(6):671–83.
Fang Y, Tseng GC, Chang C. Heavytailed distribution for combining dependent \(p\) values with asymptotic robustness. arXiv:2103.12967 (2021).
Sun S, Lulla A, Sioda M, Winglee K, Wu MC, Jacobs DR Jr, Shikany JM, LloydJones DM, Launer LJ, Fodor AA, et al. Gut microbiota composition and blood pressure: the cardia study. Hypertension. 2019;73(5):998–1006.
Friedman GD, Cutter GR, Donahue RP, Hughes GH, Hulley SB, Jacobs DR Jr, Liu K, Savage PJ. Cardia: study design, recruitment, and some characteristics of the examined subjects. J Clin Epidemiol. 1988;41(11):1105–16.
Song X, Li G, Zhou Z, Wang X, IonitaLaza I, Wei Y. Qrank: a novel quantile regression tool for eqtl discovery. Bioinformatics. 2017;33(14):2123–30.
Liu H, Ling W, Hua X, Moon JY, WilliamsNguyen JS, Zhan X, Plantinga AM, Zhao N, Zhang A, Knight R, et al. Kernelbased genetic association analysis for microbiome phenotypes identifies host genetic drivers of betadiversity. bioRxiv (2021)
Shlyakhter I, Sabeti PC, Schaffner SF. Cosi2: an efficient simulator of exact and approximate coalescent with selection. Bioinformatics. 2014;30(23):3427–9.
Charlson ES, Chen J, CustersAllen R, Bittinger K, Li H, Sinha R, Hwang J, Bushman FD, Collman RG. Disordered microbial communities in the upper respiratory tract of cigarette smokers. PLoS ONE. 2010;5(12):15216.
Zhan X, Zhao N, Plantinga A, Thornton TA, Conneely KN, Epstein MP, Wu MC. Powerful genetic association analysis for common or rare variants with highdimensional structured traits. Genetics. 2017;206(4):1779–90.
Zhan X, Plantinga A, Zhao N, Wu MC. A fast smallsample kernel independence test for microbiome communitylevel association analysis. Biometrics. 2017;73(4):1453–63.
HensleyMcBain T, Wu MC, Manuzak JA, Cheu RK, Gustin A, Driscoll CB, Zevin AS, Miller CJ, Coronado E, Smith E, et al. Increased mucosal neutrophil survival is associated with altered microbiota in hiv infection. PLoS Pathog. 2019;15(4):1007672.
Segata N, Izard J, Waldron L, Gevers D, Miropolsky L, Garrett WS, Huttenhower C. Metagenomic biomarker discovery and explanation. Genome Biol. 2011;12(6):1–18.
Paulson JN, Stine OC, Bravo HC, Pop M. Differential abundance analysis for microbial markergene surveys. Nat Methods. 2013;10(12):1200–2.
Trapnell C, Cacchiarelli D, Grimsby J, Pokharel P, Li S, Morse M, Lennon NJ, Livak KJ, Mikkelsen TS, Rinn JL. The dynamics and regulators of cell fate decisions are revealed by pseudotemporal ordering of single cells. Nat Biotechnol. 2014;32(4):381–6.
Love MI, Huber W, Anders S. Moderated estimation of fold change and dispersion for rnaseq data with deseq2. Genome Biol. 2014;15(12):1–21.
Hawinkel S, Mattiello F, Bijnens L, Thas O. A broken promise: microbiome differential abundance methods do not control the false discovery rate. Brief Bioinform. 2019;20(1):210–21.
Ferreira JA, Fuentes S. Some comments on certain statistical aspects of the study of the microbiome. Brief Bioinform. 2020;21(4):1487–94.
Egozcue JJ, PawlowskyGlahn V, MateuFigueras G, BarceloVidal C. Isometric logratio transformations for compositional data analysis. Math Geol. 2003;35(3):279–300.
Acknowledgements
Not applicable.
Funding
This work is supported in part by the National Institutes of Health grants R01 GM129512, R01 HL155417.
Author information
Authors and Affiliations
Contributions
HS developed the method, designed the analysis, and wrote the manuscript. MCW conceived the study. WL, NZ and AP contributed to the conceptation, methodological developments, and presentation. CAB, NRK, and THM prepared the data and contributed to the data analysis. All authors reviewed the manuscript.
Corresponding author
Ethics declarations
Ethics approval and consent to participate
Not applicable.
Consent for publication
Not applicable.
Competing interests
The authors declare that they have no competing interests.
Additional information
Publisher’s Note
Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.
Supplementary Information
Additional file 1
Figure on histograms of some simulated abundances vs. true abundances.
Rights and permissions
Open Access This article is licensed under a Creative Commons Attribution 4.0 International License, which permits use, sharing, adaptation, distribution and reproduction in any medium or format, as long as you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons licence, and indicate if changes were made. The images or other third party material in this article are included in the article's Creative Commons licence, unless indicated otherwise in a credit line to the material. If material is not included in the article's Creative Commons licence and your intended use is not permitted by statutory regulation or exceeds the permitted use, you will need to obtain permission directly from the copyright holder. To view a copy of this licence, visit http://creativecommons.org/licenses/by/4.0/. The Creative Commons Public Domain Dedication waiver (http://creativecommons.org/publicdomain/zero/1.0/) applies to the data made available in this article, unless otherwise stated in a credit line to the data.
About this article
Cite this article
Song, H., Ling, W., Zhao, N. et al. Accommodating multiple potential normalizations in microbiome associations studies. BMC Bioinformatics 24, 22 (2023). https://doi.org/10.1186/s1285902305147w
Received:
Accepted:
Published:
DOI: https://doi.org/10.1186/s1285902305147w
Keywords
 Normalization
 Different library size
 Omnibus approach
 Cauchy combination test