- Research article
- Open Access
Reference gene alternatives to Gapdh in rodent and human heart failure gene expression studies
© Brattelid et al; licensee BioMed Central Ltd. 2010
- Received: 6 May 2009
- Accepted: 23 March 2010
- Published: 23 March 2010
Quantitative real-time RT-PCR (RT-qPCR) is a highly sensitive method for mRNA quantification, but requires invariant expression of the chosen reference gene(s). In pathological myocardium, there is limited information on suitable reference genes other than the commonly used Gapdh mRNA and 18S ribosomal RNA. Our aim was to evaluate and identify suitable reference genes in human failing myocardium, in rat and mouse post-myocardial infarction (post-MI) heart failure and across developmental stages in fetal and neonatal rat myocardium.
The abundance of Arbp, Rpl32, Rpl4, Tbp, Polr2a, Hprt1, Pgk1, Ppia and Gapdh mRNA and 18S ribosomal RNA in myocardial samples was quantified by RT-qPCR. The expression variability of these transcripts was evaluated by the geNorm and Normfinder algorithms and by a variance component analysis method. Biological variability was a greater contributor to sample variability than either repeated reverse transcription or PCR reactions.
The most stable reference genes were Rpl32, Gapdh and Polr2a in mouse post-infarction heart failure, Polr2a, Rpl32 and Tbp in rat post-infarction heart failure and Rpl32 and Pgk1 in human heart failure (ischemic disease and cardiomyopathy). The overall most stable reference genes across all three species was Rpl32 and Polr2a. In rat myocardium, all reference genes tested showed substantial variation with developmental stage, with Rpl4 as was most stable among the tested genes.
- Reference Gene
- Candidate Reference Gene
- Stable Reference Gene
- Variance Component Analysis
- Human Heart Failure
Quantification of mRNA abundance is a central tool in studying pathological and compensatory mechanisms in heart failure. Quantitative real-time RT-PCR (RT-qPCR) has rapidly replaced other methods, allowing quantification of many gene transcripts in limited tissue samples and more sensitive detection of weakly expressed transcripts . However, this level of sensitivity requires a careful choice of method for comparison of expression data between samples. The most common strategy is to normalize the expression of a specific gene to a single reference gene, assuming that the reference gene expression is invariant between the compared physiological states. Variation in the reference gene expression between samples would therefore reflect variations in sample preparation and experimental variability. Several studies have concluded that it is difficult to identify general reference genes which can be used in all experimental settings, and that validation of the chosen reference gene(s) is important for each experimental setting [2–5].
In the heart failure literature, glyceraldehyde 3-phosphate dehydrogenase (Gapdh) and 18S ribosomal RNA are the most frequently used reference genes in quantification of gene expression, see e.g. [6–8]. In rat neonatal cardiomyocytes, it was shown that Gapdh expression was invariant with different hypertrophic stimuli , but was decreased in electrically stimulated cells . In a recent rat post-myocardial infarction (post-MI) heart failure study, the interpretation of changes in gene expression was dependent on the choice of Gapdh or 18S as reference gene . Only one recent study has examined possible reference gene candidates in human myocardium by mining public microarray data .
The aim of our study was to identify alternative reference genes to Gapdh and 18S rRNA for use in mouse and rat post-myocardial infarction heart failure models and in human heart failure studies. Since fetal and neonatal rat cardiomyocytes are commonly used in cardiac hypertrophy and signal transduction experiments, we also evaluated a subset of candidate reference genes in neonatal and embryonic myocardium in comparison to adult myocardium. In addition we have investigated the sources of variation in gene expression quantification data in terms of RNA preparation methods, technical replicates and biological sample variability.
Total RNA sample quality
Quality evaluation of total RNA samples
OD 260 nm/280 nm
28S/18S area ratio
RNA integrity number (RIN)
Interspecies variation in reference gene expression
The candidate genes Arb, Rpl32, Rpl4, Tbp, Polr2a, Hprt1, Pgk1, Ppia for each species and 18S ribosomal RNA were quantified by RT-qPCR. Due to the dominance of 18S transcripts compared to the other reference genes of interest, the 18S data were used only as a control of the RT reaction in addition to the RNA quality control (dilution curve linearity). In mouse hearts, the post-MI/Sham ratio for 18S was significantly higher than one (ratio 1.47, 95% CI: [1.19-1.82]). In rat hearts the 18S post-MI/Sham ratio was also above one, but with borderline significance (ratio 1.58, [1.00-2.51]). In the human myocardium there was no significant difference (failing/non-failing ratio 1.19, [0.76-1.84]).
The most stable reference genes in mouse, rat and human myocardium
To test the robustness of our findings, we evaluated the stability of a subset of reference genes in a second independent set of rat total RNA from Sham and post-MI myocardium (dataset 2). The samples prepared for dataset 2 differed in sample storage (dataset 1, - 80C freezer; dataset 2, RNALater), RNA isolation (dataset 1, homogenizer and Trizol; dataset 2, bead mill and Trizol) and cDNA priming methods (dataset 1, random hexamer; dataset 2, oligo-dT). Comparison of the same genes for datasets 1 and 2 yielded a nearly identical stability rank order by the geNorm method (dataset 1: Rpl32 ≤ Tbp <Arbp <Rpl4 <Gapdh; dataset 2: Tbp <Rpl32 <Arbp <Rpl4 <Gapdh). Analysis by the Normfinder method yielded also near-identical rank orders (dataset 1: Rpl32 ≤ Tbp <Arb <Rpl4 <Gapdh versus dataset 2: Tbp ≤ Rpl32 <Rpl4 <Arbp <Gapdh).
Reference gene stability across developmental stages in rat myocardium
The impact of normalization to a single reference gene with low (Rpl4, Arbp and Rpl32) or high (Gapdh) variability was evaluated in fetal, neonatal and adult stages (Figure 3B). Normalization of the serotonin transporter 5-HTT (Slc6a4, SERT) mRNA to Rpl4 suggested that 5-HTT expression increased with developmental stage. In contrast, normalization of 5-HTT to Gapdh indicated only a transient increase in 5-HTT expression.
We have identified several reference genes as alternatives to Gapdh and 18S for use in gene expression quantification in heart failure studies. The most stable reference genes were Rpl32, Gapdh and Polr2a in mouse post-infarction heart failure, Polr2a, Rpl32 and Tbp in rat post-infarction heart failure and Rpl32 and Pgk1 in human heart failure (ischemic disease and cardiomyopathy). The overall most stable reference genes across all three species were Rpl32 and Polr2a. In rat myocardium, Rpl4 was the most stable reference gene across developmental stages.
It is generally accepted that the best normalization strategy would be to calculate the geometric mean of several reference genes . However, this is not always feasible with limited amounts of tissue. Several of the reference gene candidates identified in this study should be sufficiently stable for single-gene normalization of gene expression data when necessary. We show that Gapdh is not suitable as a reference gene in human failing myocardium. A recent study using human heart failure microarray data also reached a similar conclusion .
Gene expression studies using fetal and neonatal heart material often use single reference gene normalization methods. Single reference gene normalization across developmental stages may be difficult because of the wide variation in expression at different developmental stages . We show here a marked shift in the expression stability of several reference genes in the transition from neonatal to adult rat myocardium. This effect was particularly pronounced for Gapdh, which would highly influence the interpretation of results. We found that Rpl4 and Rpl32 were better reference gene candidates across developmental stages in rat myocardium.
To explore the significance of normalization to different reference genes we analyzed the expression of the serotonin 5-HT transporter (5-HTT) during fetal and neonatal development as well as in adult heart. We have previously demonstrated that the mRNA encoding the 5-HT4 serotonin receptor is significantly upregulated in heart failure [11, 15, 16] and late fetal and neonatal development (T. Brattelid, unpublished observations). Serotonin plays an important role in cardiac development , and the 5-HT transporter can indirectly modulate the 5-HT4 response by regulating the extracellular 5-HT level in cardiac muscle. Although the expression profile of 5-HTT in late fetal and neonatal heart seems to be independent of the reference gene used, the estimated 5-HTT expression in the adult heart differs significantly with the choice of reference gene (Figure 3B). Rpl32 and Gapdh represent the extreme in each direction in stability, whereas Rpl4 is the most stable reference gene when comparing fetal, neonatal and adult heart tissue.
In the datasets for mouse, rat dataset 1 and human reference genes, we originally included a test set of 4 commonly queried transcripts in the heart failure literature (Apt2a2, Pln, Slc8a1, Nppa) to test the impact of choice of reference genes on gene expression ratios (MI/Sham or Failing/Donor). In contrast to the fetal and neonatal rat data, the ratios and statistical significance in the adult datasets were not markedly affected by choosing between the single most stable gene, the three most stable genes, Rpl32 alone or Gapdh alone in each species (data not shown). This was due to the very small differences in the stability between the most stable reference genes in our datasets.
We found a surprising discrepancy in the variability score for Polr2a between rodent and human datasets by both the geNorm and Normfinder algorithms, being low in mouse and rat (Figure 2), but high in the human dataset. In contrast, the variance component analysis indicated that human Polr2a was quite stable, and the Polr2a expression levels were very similar in the donor and failing human myocardial samples (Figure 1C). We therefore examined whether this could be due to differences in the mathematical algorithms. geNorm uses pairwise comparisons of genes and assumes that the ratio between the expression values of two stable reference genes should be approximately equal in all experimental samples . A gene is regarded as less stable if the pattern of variation between samples differs from the pattern observed for the majority of candidate genes, assuming that the majority are in average stable. Normfinder uses analysis of variance on log-transformed expression values, and all genes and samples are used simultaneously to estimate expected expression values . A stable gene is expected to deviate only modestly from these estimates. A stability value is computed based on intra- and inter-group variations, where calculation of the latter assumes equal average expression of the genes in the groups. Thus, although in a different way from geNorm, Normfinder also assumes good "average" behavior of the test genes. In the human myocardial samples, the donor hearts tended to have higher relative quantities than failing hearts for most of the tested genes (Figure 1C). Polr2a expression was very similar in the donor and failing groups, thereby deviating from the majority. Therefore, both geNorm and Normfinder classify Polr2a as less stable. In contrast, the variance component model considers the small difference between groups as an advantage. In light of these considerations, we chose to include both human Polr2a and rat Gapdh as satisfactory reference genes. A recent report investigating gene expression variation during the estrus cycle in female rats also discussed the potential shortcomings of geNorm and Normfinder and used similar methods to the variance component model used in our study .
Excellent quality of total RNA is vital for obtaining reliable quantification results [20–23]. The RNA sample quality was comprehensively evaluated. Total RNA quality is traditionally estimated by the 260 nm/280 nm O.D. ratio, even though this method has several shortcomings . All samples included in the study were regarded as high quality using 260 nm/280 nm O.D. ratio values. In contrast to the high 28S/18S ratios (>2) usually obtained in cell lines, we found a low ratio (average 1.3) in myocardial tissue from all three species. Studies in human tissues have shown poor correlation between the 28S/18S ratio and RNA sample quality [20, 21, 23, 24]. The RNA integrity number (RIN) is the most recent qualitative indicator of total RNA sample quality [20, 21, 24, 25]. We found that the RIN values for rat and mouse myocardial total RNA (average 8.0) were consistent with values from solid tissues [20, 21]. However, the RIN values for the human myocardial samples were consistently lower and the variation in the RT-qPCR data much larger than for mouse and rat, in particular for the failing hearts. This may be due to variable states of severely failing human myocardial tissue or to differences in the human sample harvesting time compared to the rapid handling of rodent myocardial samples. Even though we obtained very similar results for reference gene stability with rat datasets 1 and 2, which had considerable differences in preparation and RT priming methods, we cannot exclude that the difference in results between the human and rodent datasets may be due to differences in RNA isolation, cDNA priming methods or choice of reverse transcriptase enzymes [22, 26].
In our comparison of the two independent datasets from rat Sham and post-MI myocardium, we found that the stability of the selected reference genes was independent of sample processing and cDNA priming method, thus strengthening our findings. We also found that the biological variation contributed the most to the overall quantification variability rather than technical steps such as reverse transcription and PCR amplification reactions. Thus, for myocardial samples, increasing the biological sample size rather than number of RT reaction technical replicates is a key factor for increasing the reliability of gene expression analysis.
In the set of tested reference genes, the most stable reference genes were Rpl32, Gapdh and Polr2a in mouse post-infarction heart failure, Polr2a, Rpl32 and Tbp in rat post-infarction heart failure and Rpl32 and Pgk1 in human heart failure (ischemic disease and cardiomyopathy). The overall most stable reference genes across all three species were Rpl32 and Polr2a. In rat myocardium, Rpl4 was the most stable reference gene across developmental stages. These reference genes should be regarded as good a priori candidates, but validation of expression stability in each particular experimental setting is recommended.
Selection of candidate reference genes
Candidate reference genes were selected based on previous use in Northern blots and competitive RT-PCR and RT-qPCR studies in the literature: acidic ribosomal phosphoprotein P0 (Arbp), ribosomal protein L32 (Rpl32), ribosomal protein L4 (Rpl4), TATA-box binding protein (Tbp), RNA polymerase II alpha subunit (Polr2a), hypoxanthine guanine phosphoribosyl transferase (Hprt1), phosphoglycerate kinase 1 (Pgk1) and cyclophilin A (peptidyl prolyl isomerase A, Ppia), glyceraldehyde-3-phosphate dehydrogenase (Gapdh) and 18S ribosomal RNA.
Tissue material and total RNA sample sets
The B6/J mouse total RNA sample set was generated in this study. Rat and human myocardial total RNA sample sets were used previously in other studies in Wistar rats (adult dataset 1, adult dataset 2 ), fetal and neonatal rat material (Brattelid et al, in preparation), and humans . Random samples that fulfilled basic "good quality" OD 260/280 ratios (approximately 2.0) were chosen from each sample set. The RNA quality of these samples was reanalyzed more extensively in this study, including RIN profiling (Table 1). Samples sizes for datasets were as follows: mouse (Sham n = 3, MI n = 3), rat dataset 1 (Sham n = 3, MI n = 3), rat dataset 2 (Sham n = 6, MI n = 6) and human (Donor n = 4, Failing n = 6).
Myocardial infarction (MI) in B6/J mice and Wistar rats was induced by ligating the left anterior descending coronary artery as described [27, 28]. Age-matched Sham animals underwent the same operative procedure, but without ligating the artery. Mouse hearts were harvested after 1 week, whereas rat hearts were harvested after 6 weeks. In the original studies, criteria indicative of congestive heart failure (significantly increased left ventricular end-diastolic pressure, increased lung weight and increased lung weight/body weight ratios) were used to include mice and rats in the MI groups [28, 29]. In post-MI hearts, the infarct area and border zone were removed and the remaining viable left ventricular wall and septum were harvested. In Sham and de novo (control) animals, the left ventricular wall and septum were harvested. Total RNA from a second set of rat left ventricles from 6-week post-MI rat hearts, age-matched Sham hearts and de novo animals , were used to test whether the combined differences in tissue storage, RNA isolation and cDNA priming methods would affect reference gene stability results (rat data set 2).
Fetal rat hearts were harvested from embryos removed under 2% isoflurane anesthesia at day 3 (n = 6) and day 1 (n = 5) before the expected term. Neonatal rat hearts were harvested at 1 (n = 10), 3 (n = 6) and 5 (n = 6) days after birth. Atria were removed and ventricles from each litter were pooled. All animals were subjected to approved protocols in accordance with the Norwegian National Committee for Animal Welfare, conforming to the European Convention for the protection of Vertebrate animals used for Experimental and other Scientific Purposes (Council of Europe no. 123, Strasbourg 1985). Human samples were taken from left ventricular trabeculae from non-failing donor and failing hearts. The failing hearts were from patients undergoing heart transplantation for end-stage heart failure, resulting from ischemic heart disease or dilated cardiomyopathy. Samples were obtained under ethical approval #S01025 (Oslo University Hospital Rikshospitalet, Oslo, Norway) conforming to the Declaration of Helsinki. Mouse hearts and rat hearts for dataset 1 and human samples were immediately frozen in liquid nitrogen. Adult rat hearts for dataset 2, fetal, and neonatal rat hearts were submerged and stored in RNAlater™ (Applied Biosystems/Ambion, Austin, TX, USA).
Mouse total RNA was isolated from left ventricular myocardium using a tissue homogenizer (Polytron, Kinemetica AG, Luzern, Switzerland) and SV total RNA columns as described by the manufacturer (Promega, Madison, WI, USA). Adult rat total RNA for dataset 1 was isolated from left ventricular myocardium  using a tissue homogenizer and the phenol/chloroform method as included in the Atlas™ Pure Total RNA Labeling kit (Clontech Laboratories Inc. Mountain View, CA, USA). Adult rat left ventricular total RNA for dataset 2, fetal and neonatal RNA samples, were obtained by washing the RNAlater-conserved tissue in sterile 0.9% NaCl, followed by homogenization in 1.5 ml Trizol by mill grinding (MM301, Retsch GmbH, Haan, Germany) with ceramic beads at 30 Hz, and isolatation of total RNA by the Trizol method . Total RNA from human hearts was isolated by pulverization in liquid N2, homogenization with a tissue homogenizer and RNeasy columns (Qiagen Hilden, Germany) .: Mouse and rat dataset 1 total RNA samples were treated with DNase provided in the the RNA isolation kits, and human total RNA samples were treated with DNase I from Invitrogen (Carlsbad, CA, USA) as described by the manufacturers.
Pooled standard samples used to generate relative dilution curves for each species were prepared by mixing equal amounts of total RNA from 3 Sham and 3 MI hearts (mouse, rat), or 3 non-failing and 3 failing hearts (human), and used throughout the study.
RNA quality control
RNA concentrations were measured (1.5 μl) in an ND-1000 spectrophotometer (NanoDrop Technologies, Wilmington, DE, USA). Samples were quality checked using RNA 6000 Nano LabChips in a 2100 Bioanalyzer (Agilent Technologies, Santa Clara, CA, USA). The RNA integrity numbers (RIN)  were calculated by the instrument software. 18S serial dilution curves were run for each sample, and the linearity of the curves was used to verify the absence of inhibitory substances.
Mouse, rat (dataset 1), and human total RNA sample sets were reverse transcribed using random primers and TaqMan Reverse Transcription Reagents (P/N N808-0234, Applied Biosystems, Foster City, CA, USA). Each RNA sample was reverse transcribed independently on three separate days. All species-specific gene expression assays were run on the same cDNA generated in each independent RT reaction, thus allowing direct comparison of the relative abundance of all the reference genes within each species. The second set of de novo, Sham and post-MI adult rat myocardium total RNA as well as fetal and neonatal rat total RNA (5 μg) were oligo-dT-primed and transcribed with 400 U Superscript III (Invitrogen) in a 40 μl volume.
RT-qPCR assay information
Primer location on Refseq
AB ID Mm00725448_s1
F: CAC CAG TCA GAC CGA TAT GTG AAA A
R: TGT TGT CAA TGC CTC TGG GTT T
P: CCG CCA GTT TCG CTT AA
F: GGT GGT TGA AGA TAA GGT TGA AGG T
R: CTT TGA GTT TCT TGA GCA GCT GAA
P: CAG CCT CCT TGG TCT TC
AB ID Mm00446973_m1
F: CTT TGA GGA AAC GGT GGA TGT C
R: TCC CTT CAT CGG GTC ACT CT
P: ATG TGC TGC TGC TTC C
AB ID Mm00446968_m1
AB ID Mm99999915_g1
AB ID Mm00435617_m1
F: GCA CTG CCA AGA CTG AAT GG
R: TGC CTT CTT TCA CCT TCC CAA A
P: CTG GAT GGC AAG CAT G
AB ID Mm00437634_m1
AB ID Mm00452263_m1
AB ID Mm00441524_m1
F: GTA CAG TGC GGT GTC CAA CA
R: CTC ATC TTC TAC CGG CAT CTT CTC
P: AAG AAC CTG CTA GAC CAC C
AB ID Rn00821065_g1
AB ID Rn00820748_g1
AB ID Rn00821091_g1
F: CCT CTG AGA GCT CTG GGA TTG TA
R: GCC AAG ATT CAC GGT GGA TAC A
P: CCA CAG CTC CAA AAT A
F: CGT ATC CGC ATC ATG AAC AGT GA
R: TCA TCC ATC TTA TCC ACC ACC TCT T
P: CCT CCT CCT GCA TCT TG
AB ID Rn01527838_g1
F: GTC ATC TGC ATC CCT ACC TAT ATC ATT
R: GTG GGT GTT TCA GGA GTG ATA CTT T
P: AAT AAT CCG CTC CTT AAG TGT CCC CGG AGT
AB ID Rn99999916_s1
AB ID Rn00568762_m1
AB ID Rn01434045_m1
AB ID Rn00570527_m1
AB ID Rn00561661_m1
AB ID Hs99999902_m1
F: CAC CAG TCA GAC CGA TAT GTC AAA A
R: TGT TGT CAA TGC CTC TGG GTT T
P: CCG CCA GTT ACG CTT AA
F: CAG CAC TGG TCA TGT CTA AAG GT
R: AGC CTT CAA CTT TAT CTT CAA CTA CCA AA
P: CAT CGT ATT GAG GAA GTT C
AB ID Hs00427620_m1
AB ID Hs00172187_m1
AB ID Hs00355752_m1
AB ID Hs99999905_m1
AB ID Hs99999906_m1
AB ID Hs99999904_m1
AB ID Hs00544877_m1
AB ID Hs00160179_m1
AB ID Hs00253432_m1
AB ID Hs00383230_g1
Eukaryotic 18S endogenous control, part number 4319413E
The mean assay coefficient of variation (CV, given in %) per species was calculated by first calculating the CV of all data points for a given assay in a species, and then calculating the mean CV value for all assays within that species.
Reference gene expression variability was evaluated by geNorm  and Normfinder  analysis methods. Ratios were analyzed on the log scale to obtain approximately normally distributed observations (without outliers) and roughly equal variance across genes. Tests were two-sided, and p < 0.05 considered significant.
Mixed linear models were used to accommodate the nested experimental design and to estimate variance components and expression ratios with associated confidence intervals. Variance components included in the model were the RT reactions and the samples (nested within treatments), and with the triplicate PCR values with each run as the basic observation. We also used the sum of the variance components for the samples and the triplicates as an additional tool when evaluating gene expression stability. These types of models take into account the study design, but are limited as a general tool for evaluation of reference gene stability, because they are sensitive to large variations in total RNA quantity between samples.
We gratefully acknowledge Alexandra Finsen for Sham and post-MI mouse hearts, Odd Geiran and Halfdan Aass at Oslo University Hospital Rikshospitalet, Oslo, Norway for the human heart tissue samples, and the Department of Medical Genetics, Oslo University Hospital Ullevål, for use of the ABI 7700 instrument. We also thank Cathrine Husberg, Kåre Olav Stensløkken, and William E. Louch for critical reading of the manuscript.
Supported by The Research Council of Norway, The Norwegian Council on Cardiovascular Diseases, Anders Jahre's Foundation for the Promotion of Science, The Novo Nordisk Foundation, The Family Blix foundation, a University of Oslo EMBIO senior fellowship (KBA) and a Southeastern Norway Regional Health Authority senior fellowship (KBA).
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