Validation of reference genes for quantitative real-time PCR studies in the dentate gyrus after experimental febrile seizures
© Swijsen et al.; licensee BioMed Central Ltd. 2012
Received: 9 July 2012
Accepted: 24 September 2012
Published: 13 December 2012
Quantitative real-time PCR (qPCR) is a commonly used technique to quantify gene expression levels. Validated normalization is essential to obtain reliable qPCR data. In that context, normalizing to multiple reference genes has become the most popular method. However, expression of reference genes may vary per tissue type, developmental stage and in response to experimental treatment. It is therefore imperative to determine stable reference genes for a specific sample set and experimental model. The present study was designed to validate potential reference genes in hippocampal tissue from rats that had experienced early-life febrile seizures (FS). To this end, we applied an established model in which FS were evoked by exposing 10-day old rat pups to heated air. One week later, we determined the expression stability of seven frequently used reference genes in the hippocampal dentate gyrus.
Gene expression stability of 18S rRNA, ActB, GusB, Arbp, Tbp, CycA and Rpl13A was tested using geNorm and Normfinder software. The ranking order of reference genes proposed by geNorm was not identical to that suggested by Normfinder. However, both algorithms indicated CycA, Rpl13A and Tbp as the most stable genes, whereas 18S rRNA and ActB were found to be the least stably expressed genes.
Our data demonstrate that the geometric averaging of at least CycA, Rpl13A and Tbp allows reliable interpretation of gene expression data in this experimental set-up. The results also show that ActB and 18S rRNA are not suited as reference genes in this model.
KeywordsReference gene Quantitative real-time PCR Febrile seizures Dentate gyrus
Febrile seizures (FS) are convulsions associated with fever and occur in 4% of children between the age of 3 months and 5 years[1, 2]. Retrospective studies demonstrate that adult patients with hippocampal sclerosis-associated temporal lobe epilepsy (TLE) have a 40% incidence of FS, suggesting a causal relationship. Also, experimental FS have a long-lasting effect on hippocampal excitability, resulting in enhanced seizure susceptibility[3–5]. At a cellular level, an altered seizure threshold may come from a change in the expression of proteins that are known to control neuronal excitability (for review see). Hence, quantification of the post-FS expression of genes that encode receptors, ion channels, etc. might help elucidating FS-induced epileptogenesis.
Nowadays, quantitative real-time PCR (qPCR) is a commonly used tool to quantify gene expression. An advantage of this highly specific and sensitive technique is that it allows analysis on small amounts of starting material[7, 8]. However, measured gene expression levels may be confounded by several variables during the multistep procedure of isolating and processing RNA e.g. the amount and quality of starting material, enzymatic efficiency and variability between tissues or cells in overall transcriptional activity[9–11]. Internal reference genes are most frequently used to normalize methodology-induced variations in qPCR studies[9, 12]. Until recently, ‘housekeeping genes’ (HKGs) such as glyceraldehyde-3-phosphate dehydrogenase (GAPDH), 18S subunit ribosomal RNA (18S rRNA) or beta-actin (ActB) were commonly used as reference genes, also in neurobiological studies. HKGs are continually read and encode for products that are necessary for the metabolism and existence of a cell. They are supposed to be invariably expressed under different experimental conditions. However, the expression of these classical reference genes may vary per tissue type and developmental stage, and may even vary in response to experimental treatment[13–17]. Hence, validation of suitable reference genes for a specific sample set and experimental model is imperative to obtain consistent gene expression data. In addition, it has been shown that the accuracy of qPCR data further improves when at least three reference genes are used for normalization.
Although recent studies have validated reference genes for rat brain tissue in different experimental conditions[18–21], to our knowledge there is thus far no report of validated reference genes in hippocampal tissue from rats that have been exposed to experimental FS. Therefore, we used an established model where FS are evoked by exposing 10-day old rat pups to heated air. One week later, we evaluated the expression stability of seven frequently used reference genes in the hippocampal dentate gyrus (DG). To this end, we used two different mathematical algorithms (geNorm and Normfinder VBA applets for Microsoft Excel) for normalization.
Selected reference genes for analysis of expression stability
Primer sequence (5’ → 3’)aor SABiosciences qPCR assay IDb
Amplicon length (bp)
Cytoskeletal structural protein
F: TGT CAC CAA CTG GGA CGA TA
R: GGG GTG TTG AAG GTC TCA AA
Serine-threonine phosphatase inhibitor
F: TAT CTG CAC TGC CAA GAC TGA GTG
R: CTT CTT GCT GGT CTT GCC ATT CC
F: ACG GAC CAG AGC GAA AGC AT
R: TGT CAA TCC TGT CCG TGT CC
Structural component of 60S ribosomal subunit
F: GGA TCC CTC CAC CCT ATG ACA
R: CTG GTA CTT CCA CCC GAC CTC
General transcription factor
F: TGG GAT TGT ACC ACA GCT CCA
R: CTC ATG ATG ACT GCA GCA AAC C
Exoglycosidase in lysosomes
Catalysis of protein synthesis
Cycle threshold values of candidate reference genes
Validating candidate reference genes
Ranking of reference genes based on the expression stability evaluated by geNorm and Normfinder
CycA – Rpl13A
Influence of different normalization approaches on the expression profile of a gene of interest
Validated normalization is crucial to obtain reproducible qPCR data of genes of interest. In this context, normalizing to internal reference genes has become the most popular method to control for experimental errors introduced by the multitude of steps in this analysis. Several studies point out that the expression of reference genes may vary under different experimental conditions[13–17]. This implies the necessity of validating these genes in each new experimental setup.
To our knowledge, this is the first study that describes the stability of 18S rRNA, ActB, GusB, Arbp, Tbp, CycA and Rpl13A in the DG of rats one week after FS. Both, geNorm and Normfinder were used to rank the analyzed reference genes by their expression stability. This rank order differed slightly between both methods, probably because both tools are based on different mathematical models. Other studies have also described similar ranking discrepancies between geNorm and Normfinder[18, 24]. Interestingly though, both programs agreed on the three most stably expressed genes, being CycA, Tbp and Rpl13A. These converging results stress the significance of including these genes in the normalization factor. In addition, both programs also agreed on ActB and 18S rRNA as the least stably expressed genes. Comparison of these data with those of recent studies revealed similarities and differences. For instance, Bonefeld et al. validated eight reference genes in rat hippocampal tissue and also identified CycA and Rpl13A as the most stably expressed genes and ActB and 18S rRNA as the least stable genes. Also Pernot et al. found that CycA and Tbp were stably expressed in hippocampus samples from a mouse model of TLE, obtained across different phases of the disease. However, in contrast to our study they also observed a stable ActB expression. This discrepancy emphasizes the importance of validating reference genes in each experimental model.
Accurate normalization requires inclusion of multiple reference genes. Geometric averaging of the most stable reference genes is a validated method to obtain a reliable normalization factor. Based on a cut-off value of 1.5, geNorm indicated that the normalization factor should be based on five reference genes. However, according to the geNorm manual, this cut-off value can be set differently. geNorm calculates the optimal number of reference genes by pairwise variation analysis. In that respect, the trend of changing V values after adding additional genes can be used to obtain an estimate of the number of genes that should be included in the normalization factor. Determination of the optimal number of reference genes is always a trade-off between accuracy and practical considerations, but a minimum of three most stable reference genes is generally recommended. As indicated in Figure 2B, a pairwise variation of 0.198 was observed after adding the third most stable gene. Inclusion of the fourth or fifth most stable gene influenced only slightly the pairwise variation. The high V6/7 is caused by the high average M value of 18S rRNA, indicating that this gene is highly variably expressed under the present experimental conditions. The Acc.SD calculated by Normfinder suggested the use of six reference genes, though the additive value of genes four to six is minimal. Considering the pairwise variation values, the Acc.SD, and practical issues such as the available amount of RNA, we conclude that the geometric mean of CycA, Rpl13A and Tbp should be used to obtain an accurate normalization factor in this experimental setup. If the RNA yield allows the inclusion of an extra reference gene, GusB and Arbp may be added to this panel. These data also show that 18S rRNA is unfit as reference gene in this model.
Inclusion of the geNorm/Normfinder selected reference genes in the normalization factor, revealed an increased Cnr1 expression in animals that experienced FS (FS+). This finding is in agreement with quantitative western blot data from Chen et al.. This upregulated Cnr1 disappeared when expression levels were normalized to ActB and 18S rRNA, underscoring the suggestion that these ‘classical’ reference genes are not suitable for our experimental setup. In line with this observation, several studies have reported that including 18S rRNA or ActB in the normalization factor altered mRNA expression levels compared to normalization to geNorm proposed genes[18, 20]. As a possible explanation for erroneous normalization when 18S rRNA is used as reference gene, it has been suggested that this may relate to an imbalance between messenger RNA and ribosomal RNA.
In conclusion, the present study describes the expression stability of seven candidate reference genes in the hippocampal DG of rats, one week after FS. Our results demonstrate that the geometric averaging of at least CycA, Rpl13A and Tbp allows a reliable interpretation of mRNA expression data in this experimental set-up. These data also show that ActB and 18S rRNA are unfit to serve as reference gene in this model.
Induction of febrile seizures and tissue sampling
Litters of 5–10 male Sprague–Dawley rat pups (Harlan, Horst, The Netherlands) were housed with a dam under temperature controlled conditions and 12 h dark–light cycle with water and food ad libitum. At postnatal day 10, FS were evoked by hyperthermia as described before[26–29]. Briefly, pups were injected subcutaneously with 0.2 ml 0.9% NaCl to prevent dehydration, placed in a perspex cylinder and exposed to a regulated stream of heated air. Rectal temperatures were monitored every 2.5 min. A core temperature >39.5°C (usually reached within 5 min) indicated the start of a 30 min hyperthermia phase in which the heated air stream was adjusted to maintain a core temperature of 41–42.5°C. Behavioral seizures occurring during treatment (FS+), were monitored by two observers. These seizures were stereotyped and previously shown to correlate with rhythmic epileptic discharges in the hippocampus. Some rats did not display seizure behavior during the hyperthermia phase (FS-). The hyperthermia phase was terminated by dipping the pup in room temperature water, until the pre-treatment body temperature was reached and then returned to the dam. Normothermia control rats underwent the same treatment, except that the stream of air was adjusted to maintain the body temperature that was measured at the start of the experiment (~35°C). Six to nine days after FS induction, rats were decapitated, brains were rapidly removed from the skull and placed in ice-cold oxygenated (95%O2/5%CO2) sucrose-based artificial cerebrospinal fluid (sucrose-aCSF) containing (in mM): 210 sucrose, 2.5 KCl, 26 NaHCO3, 1.25 NaH2PO4, 25 glucose, 1 CaCl2, and 7 MgSO4 (pH 7.4, ~340 mOsm). Next, 350-μm-thick coronal slices were cut in ice-cold oxygenated sucrose-aCSF using a vibratome (Microm/Thermo Fisher Scientific, Walldorf, Germany) and DG regions were microdissected from each acute brain slice. DG samples were then quickly frozen in liquid nitrogen and stored at −80°C until RNA isolation. All experiments were approved by the Hasselt University ethics committee for animals.
RNA isolation and cDNA synthesis
Total RNA was isolated from DG samples using the RNAqueous-Micro kit (Ambion, Lennik, Belgium), according to the manufacturer’s protocol. Trace amounts of genomic DNA were removed by DNase I provided with the kit. RNA purity and concentration were checked by optical density, using a NanoDrop ND-1000 spectrophotometer (Thermo Fisher Scientific, Waltham, USA). For cDNA synthesis, total RNA (220 ng) was first incubated for 10 min at 70°C in order to prevent secondary structures, and then reverse transcribed using the Reverse Transcription System (Promega, Leiden, The Netherlands) in a 20 μl reaction volume containing 5 mM MgCl2, 1× Reverse Transcription buffer, 1 mM dNTP mixture, 0.25 μg Oligo(dT)15 primers, 0.25 μg hexamer oligonucleotides, 20 U RNase inhibitor and 12.5 U AMV reverse transcriptase, that was first incubated for 60 min at 42°C, then for 5 min at 95°C and then at 4°C. All cDNA samples were stored at −20°C until qPCR analysis.
Quantitative real-time PCR
qPCR was performed in optical 96-well plates with an ABI PRISM 7500 Fast sequence detection system (Applied Biosystems, Carlsbad, California), and carried out in a 10 μl reaction volume containing 5 μl RT SYBR green qPCR master mix (SABiosciences/Qiagen, Venlo, The Netherlands), 0.4 μM forward and reverse primer (Table 1), and 11 ng cDNA dissolved in nuclease-free water. A no-template control containing nuclease-free water instead of cDNA was included to test for possible contamination of assay reagents. Samples were run in duplicate. PCR conditions comprised a 10 min preincubation at 95°C, followed by 40 cycles of 15 s at 95°C and 60 s at 60°C. Fluorescence was measured at 522 nm wavelength during each annealing step. Each PCR program was followed by a general dissociation curve protocol to check product specificity. PCR efficiency of the reference genes was determined by a standard curve of cDNA samples according to the MIQE guidelines.
RNA copy numbers were quantified using the comparative ΔΔCt method as follows. Raw Cq values were first transformed to quantities. These raw reference gene quantities that are expressed relative to the sample with the highest quantity, served as data input for geNorm or Normfinder. The geNorm algorithm provides a measure of gene expression stability (M value) and determines the optimal number of reference genes using pairwise variation (V) analysis. In contrast to geNorm, Normfinder estimates not only the overall expression variation of the candidate reference gene, but also the variation between sample subgroups. The output of Normfinder consists of a stability value based on both intra- and intergroup expression variation. The Accumulated Standard Deviation (Acc.SD), as indicator for the optimal number of reference genes, was determined using GenEx software. For each sample, the normalization factor based on n reference genes was calculated as the geometric average of the n raw reference gene quantities.
Data are presented as mean ± standard error of the mean (SEM). Statistical analysis was performed using Graphpad Prism5 software. Differences between means were tested using the Mann–Whitney test. A value of P < 0.05 was considered as statistically significant.
- 18S rRNA:
18S subunit ribosomal RNA
Acidic ribosomal phosphoprotein P0
Quantitative real-time PCR
Ribosomal protein L13A
TATA box binding protein
Temporal Lobe Epilepsy
We would like to thank Rosette Beenaerts for technical assistance. This research was financially supported by a grant from the transnational University Limburg (tUL) and the Interuniversity Attraction Poles Program (IUAP – Belgian State – Belgian Science Policy).
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