- Open Access
Reference genes identification for normalization of qPCR under multiple stresses in Hordeum brevisubulatum
© The Author(s) 2018
- Received: 25 October 2018
- Accepted: 10 December 2018
- Published: 18 December 2018
Real-time quantitative PCR has been widely used as the most reliable method to measure gene expression, due to its high accuracy and specificity. Wild barley (Hordeum brevisubulatum (Trin.) Link) is a wild relative species in Triticeae that has strong tolerance to abiotic stresses and extremely wide adaptation. However, suitable references gene have not been documented for standardization of gene expression in wild barley under abiotic stress.
Here we report the first systematic and comprehensive analysis of reference genes for quantitative real-time PCR standardization in wild barley. We selected 11 genes, including ACT (Actin), ADP (ADP-ribosylation factor 1), CYP2 (Cyclophilin 2), EF-1α (Elongation factor 1-alpha), GAPDH (Glyceraldehyde 3-phosphate dehydrogenase), HSP90 (Heat shock protein 90), TUBα (Alpha-tubulin), TUBβ6 (Beta-tubulin 6), UBI (Ubiquitin), 18SrRNA-1 (guanine1575-N7-methyltransferase) and 18SrRNA-3 (adenine1779-N6-dimethyltransferase) from a wild barley transcriptome database and analyzed their expression stabilities in shoots and roots of wild barley seedling under various stress conditions using comparative ΔCt, BestKeeper, Normfinder and geNorm software. The results demonstrated that ADP was the most suitable reference gene in salt stress while UBI showed peak stability under mannitol and ABA stress; EF-1α was the most appropriate reference gene for PEG, GA3, ethylene and heat stress; 18SrRNA-3 was the best choice for cold stress; and TUBα was the first stable gene across different tissues.
Our main contribution was to identify reference genes with suitable and stable expression in wild barley under various stress conditions and in different tissues to provide a useful resource for future studies. The results demonstrate the importance of transcriptome data as a useful resource for the screening of candidate reference genes and highlight the need for specific reference genes for specific conditions. Furthermore, these findings will provide valuable information for wild barley and relative species for future research.
- Hordeum brevisubulatum
- Reference gene
- Abiotic stress
- Quantitative real-time PCR
Wild barley (Hordeum brevisubulatum), which is a relative of cultivated barley (H. vulgare), is an important wild germplasm resource with ecological, feeding and ornamental value. The salient feature of H. brevisubulatum is its high tolerance to multiple abiotic stresses, including drought, salinity and alkalinity, allowing it to grow in saline-alkali grasslands in the North of China where it is used as a major forage for livestock [1, 2]. Wild barley has evolved molecular mechanisms of abiotic stress tolerance during long-time adaptation. To better understand its adaptable mechanisms, it is important to discover key abiotic stress genes and dissect their function; gene expression profiles are, therefore, the first step for gene functional analysis. Although there were several reports on ion balance and gene function of H. brevisubulatum , appropriate reference genes for multiple stresses have not been documented yet.
Quantitative real-time PCR (qRT-PCR) is a commonly used technique for investigating gene expression levels with high accuracy and sensitivity [4, 5]. Approaches for detection of the amounts of PCR products (amplicons) using qRT-PCR are classified into two categories: relative quantification based on housekeeping genes (HKGs) and absolute quantification achieved with DNA standards via calibration curves . One of the most straightforward and robust methods for accurately quantifying subtle changes is the relative quantification. However, gene expression can be affected by many confounding factors such as RNA extraction, reverse transcription and qRT-PCR efficiency [7, 8]. To avoid biased results and erroneous interpretations, a critical component of relative quantification analysis is the normalization of data by measuring in parallel the expression of HKGs that are commonly used as “reference genes” from the same specimen [9–12]. The expression of HKGs that are constitutively expressed to maintain cellular function is relatively steady in different tissues and organs of specimens under various biotic and abiotic circumstances . Next-generation sequencing (NGS) data mining and HKG identification in model species have shown that some internal controls exhibited both species- and tissue- specific expression patterns. Furthermore, their expression levels are also influenced by environmental factors (drought, salinity, temperature and hormones) as well as specific experimental conditions [6, 14–17].
In general, genes that play key roles in the maintenance of basic cellular functioning are typically selected as reference genes such as 18S ribosomal RNA (18SrRNA), beta-actin (β-actin), elongation factor-1 alpha (EF-1α), ubiquitin (UBI) and glyceraldehyde-3-phosphate dehydrogenase (GAPDH), which have been widely adopted for normalization [18, 19]. Nevertheless, rather than randomly selecting reference genes from various sources, the reference genes used in specific species require experimental validation. Moreover, single gene quantification qPCR assays are well known to frequently exhibit variability in gene expression under various experimental conditions . The Minimum Information for Publication of Quantitative Real-Time PCR Experiments (MIQE) guidelines developed for the proper selection and validation of stable candidate reference genes for qPCR experiments highly recommend average data from more than two reference genes [20–22]. Several statistical algorithms such as geNorm, NormFinder and BestKeeper, have been developed for the selection of reference genes for qRT-PCR analysis [17, 23, 24]. These tools can calculate the expression stability value (M) for different reference genes. Application of all these algorithms can contribute to the identification of the best stable reference genes for different experimental samples.
In this study, we investigated several reference genes based on H. vulgare and Pennisetum glaucum [25–29]. After extracting the corresponding HKGs from H. brevisubulatum transcriptome data and detecting their expression using qRT-PCR, we identified 11 candidate reference genes and measured the expression stability of these genes in different adult tissues or under various abiotic stress and hormone treatments then analyzed the qRT-PCR results using GeNorm , NormFinder , BestKeeper  and the comparative ΔCt method . The web-based comprehensive tool RefFinder was used to rank their expression stability . This research represents the first comprehensive systematic screening of reference genes for H. brevisubulatum based on experiments examining temporal and spatial expression in response to abiotic stress and hormone treatment. Furthermore, the results will improve the accuracy and reliability of the qRT-PCR technique and will provide a useful reference for gene expression studies in specific species in the Hordeum genus.
Validation of candidate reference genes from transcriptome data
Comprehensive details of 11 candidate reference genes used for normalization
Regression coefficient (R2)
Expression patterns of candidate reference genes
A high Ct value represents a low expression level ; of the 11 reference genes, EF-1α and UBI had the highest expression levels and ACT the lowest levels (Fig. 3). In NaCl, the expression of ACT in roots was higher than shoots while the expression of CYP2 and GAPDH in roots were lower than shoots (Fig. 3a). In PEG6000, the expression of ACT in roots was lower than shoots and the expression of 18SrRNA-1 in roots was higher than shoots (Fig. 3b). In ABA, the expression of ADP, GAPDH, HSP90 and TUBβ6 in roots was higher than shoots (Fig. 3d). In ethylene, the expression of ADP in roots was higher than shoots (Fig. 3f). In cold, the expression of ADP and 18SrRNA-1 in roots was higher than shoots (Fig. 3g). In heat, the expression of ACT, CYP2, TUBα, TUBβ6 and 18SrRNA-3 in roots was lower than shoots (Fig. 3h). However, there was no significant difference in the expression of the 11 genes in shoots and roots under mannitol and GA3 treatment (Fig. 3c, e). While there was no difference in the expression of these 11 genes in shoot and root tissue under normal conditions (Fig. 2) some of these genes were differentially induced in root and shoot tissue by stress (Fig. 3). Notably, EF-1α and UBI did not differ significantly in shoots and roots under eight stress and phytohormone treatments, revealing the importance and stability of these two reference genes in the selection of internal reference genes in H. brevisubulatum.
Stability analysis of candidate reference genes
Salt stress (NaCl treatment) and drought stress (PEG6000, mannitol treatment) both induce cell osmotic stress responses . According to comparative ΔCt, BestKeeper and Normfinder, ADP and UBI were the most stable genes in NaCl treatment while ACT, CYP2 and GAPDH were the least stable. EF-1α, UBI and ADP were the most stable genes in PEG treatment according to comparative ΔCt, Normfinder and geNorm while 18SrRNA-1, CYP2 and ACT were the most unstable. UBI and EF-1α were two of the three genes with the best stability in mannitol treatment according to comparative ΔCt, BestKeeper and Normfinder while TUBβ6, ACT and TUBα were the least stable (Fig. 4a–c; Additional file 2: Table S1).
Definitive reference genes under multiple treatments and tissues in H. brevisubulatum
Optimal single reference gene
Optimal reference gene combination
UBI 18SrRNA-1 18SrRNA-3
EF-1α 18SrRNA-1 ADP
TUBα UBI TUBβ6
Observation of comparative ΔCt, BestKeeper, Normfinder and geNorm indicated that the most stable candidate genes across ABA treatment were UBI, 18SrRNA-1 and 18SrRNA-3 while the least stable genes were TUBβ6, GAPDH and ACT. The optimal reference genes across GA3 treatment were EF-1α, 18SrRNA-3 and UBI according to comparative ΔCt, Normfinder and geNorm and the least stable reference genes were TUBα, TUBβ6 and ACT. In the ethylene treatment, the preferred genes were EF-1α, TUBα and UBI according to comparative ΔCt, BestKeeper and Normfinder while CYP2, 18SrRNA-3 and ACT were the least stable (Fig. 4d–f; Additional file 2: Table S1).
According to RefFinder, the order of reference gene stability under ABA treatment was: UBI > 18SrRNA-1 > 18SrRNA-3 > EF-1α > CYP2 > ADP > HSP90 > TUBα > TUBβ6 > GAPDH > ACT. The ranking of gene stability across GA3 treatment was: EF-1α > 18SrRNA-3 > UBI > HSP90 > 18SrRNA-1 > CYP2 > GAPDH > ADP > TUBα > TUBβ6 > ACT. Under ethylene treatment the ranking of reference gene stability was: EF-1α > TUBα > UBI > TUBβ6 > HSP90 > GAPDH > 18SrRNA-1 > ADP > CYP2 > 18SrRNA-3 > ACT (Fig. 5d–f). According to value of Vn/n + 1 < 0.15 indicates that the supplemental reference genes will not manifestly change the normalization, the geNorm data predicted that the pair-wise value of V3/4 was < 0.15 in the ABA treatment. In the GA3 and ethylene treatments the pair-wise values of V2/3 were < 0.15 (Fig. 6). Therefore, UBI, 18SrRNA-1 and 18SrRNA-3 were considered stable candidate genes across the tested ABA treatments while EF-1α and 18SrRNA-3 were determined to be suitable reference genes under GA3 treatment and EF-1α and TUBα were found to be the most suitable reference genes under ethylene treatment (Table 2).
Based on the gene stability data, which were calculated by comparative ΔCt, BestKeeper, Normfinder and geNorm, 18SrRNA-3, UBI and ADP were found to be the most stable genes in cold treatment according to comparative ΔCt, Normfinder and geNorm while TUBβ6, TUBα and ACT were the least steady across cold treatment. Under heat stress, EF-1α, 18SrRNA-1 and ADP showed the best stability according to comparative ΔCt, Normfinder and geNorm while HSP90, TUBα and ACT showed the least stability (Fig. 4g, h; Additional file 2: Table S1).
According to RefFinder, the order of reference gene stability under cold treatment was: 18SrRNA-3 > UBI > ADP > HSP90 > GAPDH > CYP2 > EF-1α > 18SrRNA-1 > TUBβ6 > TUBα > ACT. Gene stability under heat stress was ranked: EF-1α > 18SrRNA-1 > ADP > GAPDH > 18SrRNA-3 > CYP2 > TUBβ6 > UBI > HSP90 > TUBα > ACT (Fig. 5g, h). The geNorm analysis data predicted that the pair-wise values of V2/3 were < 0.15 in cold treatment and that the pair-wise values of V3/4 were below the cut-off value of 0.15 under heat stress (Fig. 6). This suggests that 18SrRNA-3 and UBI was the best combination of reference genes under cold treatment and EF-1α, 18SrRNA-1 and ADP were the most suitable reference genes for H. brevisubulatum under heat stress (Table 2).
Shoot and root tissue
The comparative ΔCt, BestKeeper and Normfinder results indicated that TUBα and UBI were two of the three most stably expressed genes in shoot and root tissue, while geNorm results indicated that the two most stable genes were TUBα and TUBβ6. The least stable genes between shoot and root tissue were GAPDH, HSP90 and CYP2 (Fig. 4i; Additional file 2: Table S1).
Based on RefFinder, the ranking order of reference gene stability between shoot and root tissue was: TUBα > UBI > TUBβ6 > EF-1α > ACT > 18SrRNA-3 > ADP > 18SrRNA-1 > GAPDH > HSP90 > CYP2 (Fig. 5i). The geNorm data analysis showed that the pair-wise value of V3/4 was < 0.15 (Fig. 6). Therefore, TUBα, UBI and TUBβ6 were considered the most appropriate reference genes between shoot and root tissue in H. brevisubulatum (Table 2). Notably, the study found that the expression of TUBα and TUBβ6 in roots was unstable and decreased over time under heat stress while the expression of TUBβ6 in roots increased over time under ABA treatment. However, the expression of UBI in eight treatments was stable in both shoots and roots. Therefore, UBI is more adaptable and stable than TUBα and TUBβ6 following abiotic stress.
The qRT-PCR approach has become a key method for gene expression profiling owing to its accuracy, sensitivity and efficiency . It is crucial to select reference genes that are stably expressed amongst treatment groups in qRT-PCR studies; a good reference gene should maintain invariable expression levels in different tissues, organs and developmental stages, as well as under various stress conditions . Therefore, to select appropriate reference genes under specific conditions must be statistically and experimentally helpful for biological technicians.
RNA quantity, primer amplification efficiency and specificity are important for qRT-PCR analysis . Here, the OD ratio (A260/A280) of all RNA samples was between 1.8 and 2.0 and the amplification efficiency of the 11 candidates ranged from 88 to 115% (all R2 > 0.990) (Table 1). Thus, the quality of the RNA and amplification was sufficient for qRT-PCR (Fig. 1b). Previous studies have reported that the expression level of reference genes is not always stable under all experimental conditions [27–30] and that mRNA expression levels varied among several housekeeping genes [40, 41]. Here these factors were confirmed in different tissues of H. brevisubulatum under various abiotic stresses and hormone treatments (Fig. 3).
Thus far, several reports have shown the importance of selecting proper reference genes for data normalization and have highlighted the identification of these genes vary depending on the model of study [6, 7, 26, 27, 42, 43]. Although reference genes have been identified in barley (H. vulgare) [26, 28, 29, 32], there are no reports about a systematic and comprehensive study on the selection and identification of reliable reference genes for H. brevisubulatum under various conditions. In the current study, we tested the expression stabilities of 11 candidate reference genes under eight stress and phytohormone conditions at different time points in shoot and root tissues (Additional file 2: Table S1). We have selected these 11 reference genes by referring to existing research reports: ADP, UBI, ACT, GAPDH and HSP90 were reported in barley ; 18SrRNA, TUBα and TUBβ6 were reported in Corchorus capsularis ; and EF-1α and CYP2 were reported in Pennisetum glaucum and Lycoris aurea [25, 44]. We also analyzed large-scale transcriptome data of H. brevisubulatum to help select these candidate reference genes. Using three different software programs (geNorm, Normfinder and BestKeeper) [17, 23, 24], the 11 candidate reference genes were found to exhibit differences in their stability under eight stress and phytohormone treatments in H. brevisubulatum (Fig. 3; Additional files 1 and 2: Fig. S1 and Table S1). Additionally, because of the different algorithms, the rankings generated by the three software programs and ∆Ct were not completely identical (Additional file 2: Table S1). For example, in the NaCl stress subset, ADP and UBI were ranked as the most stable by ∆Ct, Normfinder and BestKeeper while geNorm identified EF-1α and 18SrRNA-3 as the most stable. In the GA3 stress subset and cold stress subset, EF-1α and 18SrRNA-3, which were the most stable genes identified by ∆Ct, Normfinder and geNorm, were ranked at a medium position in BestKeeper (Additional file 2: Table S1). This apparent divergence is probably because of discrepancies in the four statistical algorithms to calculate stability; similar situations have occurred in other studies [27, 44, 51].
The geNorm program was used to determine the stability of a candidate gene by pairwise variations and the Normfinder and BestKeeper programs were used to prevent co-regulation and to further assess the analysis results obtained from the geNorm program. According to the geNorm algorithm, reference genes with an M value below 1.5 were considered to be stably expressed and the optimal number of reference genes was determined based on the pairwise variation between sequential ranked genes (Vn/Vn + 1) with the cut-off value of 0.15. When the Vn/n + 1 value was below 0.15, no additional genes were required for accurate normalization . According to this study, the V2/3 values were below 0.15 in NaCl, PEG6000, mannitol, GA3, ethylene and cold, suggesting that adding an extra gene for normalization was not necessary to obtain more accurate results. For ABA, heat and tissue treatments, the V2/3 values were 0.152, 0.165 and 0.166, indicating that additional reference genes may be required (Fig. 6). Previous reports showed that the variation of reference genes was relatively large [44–47]; here, the V3/4 value of the ABA, heat and tissue treatments was less than 0.15, indicating that the variation of these 11 reference genes was relatively small under various stress conditions in H. brevisubulatum (Fig. 6). Considered to be an integrative statistical program, RefFinder has been widely applied to evaluate the overall stability of reference gene expression and determine appropriate reference genes for diverse plant species [31, 48]. Based on the comprehensive RefFinder analysis, we have summarized and demonstrated the ordering of reference gene stability under various treatments and tissues (Fig. 5). Comprehensive analysis of the ordering performed by RefFinder and the numbers produced by geNorm was used to identify the most stable reference gene or combination of genes in each treatment and tissue (Table 2).
Wild barley is a wild germplasm resource with excellent resistance to abiotic stress such as salt tolerance [1, 50]. Therefore, it is necessary to strengthen the research on the expression and function of genes in H. brevisubulatum. This study is the first systematic and comprehensive description of suitable and stable reference genes for H. brevisubulatum in different tissues under various stress conditions and has provided a selection of reference genes that can be used to accurately examine gene expression in subsequent research in H. brevisubulatum. In summary, 11 reference gene candidates were selected based on our transcriptome sequence data and previous reports and their expression stability was assessed using four algorithms. The candidates were then ranked according to their stability to determine the most suitable reference gene and gene combination for each treatment (Table 2). Most of the previous reports have studied appropriate combinations of reference genes and the identification of single reference genes suitable for certain stress conditions is rarely reported . In fact, it is often difficult to standardize qRT-PCR data when using a combination of reference genes. To ensure the accuracy of the experiment and simplify the experimental operation, we also proposed a standardization method for single reference genes (Table 2). Furthermore, EF-1α and UBI can be applied to any of the stress treatments and tissues (Table 2) as their expression did not differ significantly in shoot and root tissue under eight stress and phytohormone treatments (Fig. 3; Additional file 1: Fig. S1), revealing the importance and stability of these two reference genes under multiple stress conditions in H. brevisubulatum.
In this study, our main contribution was to identify reference genes with suitable and stable expression in wild barley under various stress conditions and in different tissues to provide a useful resource for future studies. 11 candidate reference genes were screened from the wild barley transcriptome database, and their stability was evaluated and ranked based on four algorithms (Normfinder, BestKeeper, geNorm and the comparative ∆Ct method). We identified the most stable single reference genes for each treatment: ADP for NaCl treatment; EF-1α for PEG, GA3, ethylene and heat stress; UBI for mannitol and ABA stress; 18SrRNA-3 for cold stress; TUBα for different tissues. We have also proposed the most suitable reference gene combinations: ADP and UBI in NaCl stress; EF-1α and UBI in PEG and mannitol stress; UBI, 18SrRNA-1 and 18SrRNA-3 in ABA treatment; EF-1α and 18SrRNA-3 in GA3 treatment; EF-1α and TUBα in ethylene treatment; 18SrRNA-3 and UBI in cold stress; EF-1α, 18SrRNA-1 and ADP in heat stress; and TUBα, UBI and TUBβ6 in different tissues. Our results demonstrate the importance of transcriptome data as a useful resource for the screening of candidate reference genes and highlight the need for specific reference genes for specific conditions. Furthermore, the reference genes selected in the current study will be helpful for accurate normalization of qRT-PCR data and will facilitate future gene expression and functional verification studies in H. brevisubulatum.
Plant material and treatments
Seeds of H. brevisubulatum were collected from the saline grassland in the suburbs of Hohhot of Inner Mongolia Autonomous Region of China and obtained this material through salt tolerance screening. A large number of individual plants have been obtained through tissue culture, and reserved plenty of seeds for subsequent research.
The wild barley seeds were immersed in water for 2 d at 4 °C for vernalization, then placed in an incubator at 22–25 °C (night and day thresholds) under a 16 h/8 h photoperiod for 2–3 d to promote seed germination. When the seedlings were about 1.0 cm long, they were transferred to a 250 ml beaker containing Hoagland’s nutrient solution. The seedling roots were immersed in the nutrient solution and the young shoots floated on gauze on the surface. The seedlings were then cultured for approximately 2 w until the plants grew to the two-leaf and one-heart stage at which point various abiotic stress treatments: 350 mM NaCl, 350 mM mannitol, 10% PEG6000, 20 μM ABA, 100 μM GA3, 100 μM ethylene, cold (4 °C) and heat stress (42 °C) were performed.
Sample collection and RNA extraction
Shoot and root tissues of H. brevisubulatum for the various abiotic stress treatments (salt, mannitol, PEG6000, ABA, GA3, ethylene, cold and heat stresses) were collected and labelled at 0 h, 0.5 h, 1 h, 2 h, 3 h, 6 h and 12 h with four biological replicates taken for each. No 12 h samples were taken for the ethylene treatment. To ensure the integrity of the sample RNA, isolated samples were immediately frozen in liquid nitrogen and stored at − 80 °C before RNA extraction.
Total RNA was extracted using Trizol lysis (Takara, Dalian, China). First, frozen specimens were ground in liquid nitrogen to a fine powder with a pestle and a mortar. Next, the powder was completely dissolved in Trizol reagent blended by vortexing. Then, the mixture was centrifuged at 12,000×g at 4 °C for 5 min. Phenol–chloroform equal to one-fifth the total volume was added to the supernatant to purify the RNA and the samples were centrifuged at 12,000×g at 4 °C for 5 min. An equal volume of chloroform was added and aspirated to remove the phenol before a half volume of 8 M LiCl and a half volume of 75% alcohol was added to the supernatant to precipitate the RNA for at least 1 h. Finally, the RNA precipitate was washed twice with 75% ethanol and dissolved with RNA-free water before the RNA quality and concentration were measured. The integrity and purity of the RNA samples were determined by 1.5% agarose gels electrophoresis and the RNA concentration was assessed by a Thermo Scientific NanoDrop 2000c UV–Vis spectrophotometer (Thermo Fisher Scientific Inc., Waltham, MA, USA).
cDNAs were reverse transcribed from total RNA using a HiScript II Q Select RT SuperMix reagent Kit (Vazyme Biotech Co., Ltd, Nanjing, China) following the manufacturer’s protocol. This reverse transcription kit removes trace amounts of DNA from total RNA to ensure that qRT-PCR amplification is completely derived from cDNA. The reverse-transcribed cDNA templates were diluted 1:5 with nuclease-free water and stored at − 20 °C until qRT-PCR analysis with minimal thawing and refreezing.
Specific primer design
We examined the reference genes of barley (H. vulgare) in the internal control genes (ICG) database that is a wiki-based knowledgebase of internal control genes (or reference genes) for RT-qPCR normalization in a variety of species (http://icg.big.ac.cn/index.php/Main_Page) such as ADP, UBI, ACT, GAPDH and HSP90. Moreover, we also referred to previous research in L. aurea (EF-1α, CYP2)  and Corchorus capsularis (18SrRNA, TUBα, TUBβ6) . Then, the NCBI local blast software (blast-2.7.1+) was used to compare the sequences of reference genes of different species with existing wild barley transcriptome databases and the sequences of 11 candidate reference genes of wild barley were obtained. The protein prediction was performed using the open reading frame (ORF) finder (http://www.ncbi.nlm.nih.gov/gorf/). Multiple alignments of predicted amino acid sequences were created using DNAMAN .
Specific primers were designed using the Primer-BLAST tool in NCBI (available online: (http://www.ncbi.nlm.nih.gov/tools/primer-blast/) based on the sequences of the candidate reference genes. The parameters were as follows: product size was 70–200 bp; primer melting temperature (Tm) was 58–62 °C; database was nr; organism was H. brevisubulatum (taxid: 52155). To obtain the most suitable primers, primer 5 was used to check the primer mismatch, hairpin structure and dimer energy value before 2–3 pairs of primers were designed per gene and synthesized by Sangon Biotech Co., Ltd. (Shanghai, China).
Primer-specific detection and amplification efficiency
It was necessary to detect the specificity of the primer by gel electrophoresis and melting curve analysis. The efficiency reflects the adequacy of the qRT-PCR reaction, the pros and cons of the primers, and the quality of the template . The efficiencies (E) and correlation coefficients (R2) were calculated for each reference gene . The standard curve of each primer pair was established with serial dilutions of cDNA ((1/5)0, (1/5)1, (1/5)2, (1/5)3 and (1/5)4). The amplification efficiency (E) of qRT-PCR was determined according to the equation: E = 10 1/K, where K represents the slope of the standard curve.
Quantitative real-time PCR (qRT-PCR)
qRT-PCR was performed using TB Green™ Premix Ex Taq™ II (Takara, Dalian, China) on the StepOne Plus Real-Time PCR System (Applied Biosystems, Foster City, CA, USA). Twenty microliter-reactions were performed in MicroAmp Fast Optical 96-Well reaction plates with barcodes (Applied Biosystems, Foster City, CA, USA) with each reaction containing 2 μl cDNA, 10 μl 2 × qPCR Mix, 0.4 μl 50 × ROX Reference Dye, 0.8 μl each of the forward and reverse primers, and 6 μl of nuclease-free water. The PCR program involved a two-step process of initial denaturation at 95 °C for 30 s followed by 40 cycles of denaturation at 95 °C for 5 s and annealing at 60 °C for 30 s where the fluorescence signal was detected. Four technical replicates were included for each reaction. Melting curve data were gathered from 95 °C maintain 15 s down to 60 °C hold 1 min, then up to 95 °C keep 15 s (with increments of 0.3 °C), with fluorescence signals detected during this increase.
Excel-based programs were used to analyze gene expression stability, including geNorm, NormFinder and BestKeeper. RefFinder, which is a user-friendly web-based comprehensive tool developed for evaluating and screening reference genes from extensive experimental datasets (http://184.108.40.206/referencegene.php), was also used. It integrates the currently available major computational programs (geNorm, Normfinder, BestKeeper and the comparative ∆Ct method) to compare and rank the tested candidate reference genes. Based on the rankings from each program, it assigned an appropriate weight to an individual gene and calculated the geometric mean of their weights for the overall final ranking . Finally, the most suitable internal reference gene under each treatment condition was determined. All assays were repeated at least three times and the data represent the mean ± SD. Microsoft® Excel 2016 and SAS 9.2 statistical software were used for data analysis and Duncan’s Multiple Range Test, respectively.
Conceptualization, LZ and RL; Data curation, LZ; Formal analysis, LZ and QZ; Funding acquisition, LZ and RL; Investigation, LZ, YL; Methodology, LZ; Resources, RL, HZ, YJ; Supervision, RL; Writing—original draft, LZ; Writing—review & editing, LZ and RL. All authors read and approved the final manuscript.
We thank Emma Tacken, PhD, from Liwen Bianji, Edanz Group China (www.liwenbianji.cn/ac), for editing the English text of a draft of this manuscript.
The authors declare that they have no competing interests.
Availability of data and materials
The data generated or analyzed during this study are included in this published article and its supplementary information files.
Consent for publication
Ethics approval and consent to participate
This work was funded by the China Postdoctoral Science Foundation (Grant No. 2017M620 676), Beijing Postdoctoral Research Foundation (Agreement No. 2018-ZZ-065), Special Program for Innovation of Beijing Academy of Agriculture and Forestry Sciences (Grant No. KJCX20180201), Beijing Academy of Agriculture and Forestry Sciences Postdoctoral Research Fund, and the National Natural Science Foundation of China (Grant No. 3177100015).
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- Li RF, Zhang JW, Wu GY, Wang HZ, Chen YJ, Wei JH. HbCIPK2 a novel CBL-interacting protein kinase from halophyte Hordeum brevisubulatum, confers salt and osmotic stress tolerance. Plant Cell Environ. 2012;35:1582–600.View ArticleGoogle Scholar
- Wang CM, Xia ZR, Wu GQ, Yuan HJ, Wang XR, Li JH, Tian FP, Zhang Q, Zhu XQ, He JJ, Kumar T, Wang XL, Zhang JL. The coordinated regulation of Na+ and K+ in Hordeum brevisubulatum responding to time of salt stress. Plant Sci. 2016;252:358–66.View ArticleGoogle Scholar
- Lü SY, Jing YX, Shen SH, Zhao HY, Ma LQ, Zhou XJ, Ren Q, Li YF. Antiporter gene from Hordum brevisubulatum (Trin.) link and its overexpression in transgenic tobaccos. J Integr Plant Boil. 2005;47:343–9.View ArticleGoogle Scholar
- Bustin SA. Quantification of mRNA using real-time reverse transcription PCR (RTPCR): trends and problems. J Mol Endocrinol. 2002;29:23–39.View ArticleGoogle Scholar
- Bustin SA, Nolan T. Pitfalls of quantitative real-time reverse-transcription polymerase chain reaction. J Biomol Tech. 2004;15:155–66.PubMedPubMed CentralGoogle Scholar
- Huis R, Hawkins S, Neutelings G. Selection of reference genes for quantitative gene expression normalization in flax (Linum usitatissimum L.). BMC Plant Biol. 2010;10.Google Scholar
- Hao XY, Horvath DP, Chao WS, Yang YJ, Wang XC, Xiao B. Identification and evaluation of reliable reference genes for quantitative real-time PCR analysis in tea plant (Camellia sinensis (L.) O. Kuntze). Int J Mol Sci. 2014;15:22155–72.View ArticleGoogle Scholar
- Fleige S, Pfaffl MW. RNA integrity and the effect on the real-time qRT-PCR performance. Mol Asp Med. 2006;27:126–39.View ArticleGoogle Scholar
- Yang CX, Pan HP, Liu Y, Zhou XG. Stably expressed housekeeping genes across developmental stages in the two-spotted spider mite, tetranychus urticae. PLoS ONE. 2015;10.Google Scholar
- Bustin SA, Benes V, Nolan T, Pfaffl MW. Quantitative real-time RT-PCR—a perspective. J Mol Endocrinol. 2005;34:597–601.View ArticleGoogle Scholar
- Strube C, Buschbaum S, Wolken S, Schnieder T. Evaluation of reference genes for quantitative real-time PCR to investigate protein disulfide isomerase transcription pattern in the bovine lungworm Dictyocaulus viviparus. Gene. 2008;425:36–43.View ArticleGoogle Scholar
- Dheda K, Huggett JF, Chang JS, Kim LU, Bustin SA, Johnson MA, Rook GAW, Zumla A. The implications of using an inappropriate reference gene for real-time reverse transcription PCR data normalization. Anal Biochem. 2005;344:141–3.View ArticleGoogle Scholar
- Bao WL, Qu YL, Shan XY, Wan YL. Screening and validation of housekeeping genes of the root and cotyledon of Cunninghamia lanceolate under abiotic stresses by using quantitative real-time PCR. Int J Mol Sci. 2016;17:1198.View ArticleGoogle Scholar
- Guenin S, Mauriat M, Pelloux J, VanWuytswinkel O, Bellini C, Gutierrez L. Normalization of QRT-PCR data: the necessity of adopting a systematic, experimental conditions-specific, validation of references. J Exp Bot. 2009;60:487–93.View ArticleGoogle Scholar
- Pfaffl MW, Prgomet C, Schmitz S, Meyer HHD, Bruckmaier RM. LPS effects on the mRNA expression of inflammatory factors in the mammary gland: Quantitative transcriptomics in various cell types using real-time RT-PCR. Tissue Antigens. 2004;64:326–7.Google Scholar
- Podevin N, Krauss A, Henry I, Swennen R, Remy S. Selection and validation of reference genes for quantitative RT-PCR expression studies of the non-model crop musa. Mol Breed. 2012;30:1237–52.View ArticleGoogle Scholar
- Andersen CL, Jensen JL, Orntoft TF. Normalization of real-time quantitative reverse transcription-PCR data: a model-based variance estimation approach to identify genes suited for normalization, applied to bladder and colon cancer data sets. Cancer Res. 2004;64:5245–50.View ArticleGoogle Scholar
- Tang XL, Wang HY, Shao CY, Shao HB. Reference gene selection for qPCR normalization of kosteletzkya virginica under salt stress. BioMed Res Int 2015;2015.Google Scholar
- Lu YH, Yuan M, Gao XW, Kang TH, Zhan S, Wan H, Li JH. Identification and validation of reference genes for gene expression analysis using quantitative PCR in spodoptera litura (Lepidoptera: Noctuidae). PLoS ONE. 2013;8.Google Scholar
- Bustin SA, Beaulieu JF, Huggett J, Jaggi R, Kibenge FSB, Olsvik PA, et al. MIQE precis: practical implementation of minimum standard guidelines for fluorescence-based quantitative real-time PCR experiments. BMC Mol Biol. 2010;11:74.View ArticleGoogle Scholar
- Bustin SA, Benes V, Garson JA, Hellemans J, Huggett J, Kubista M, et al. The MIQE guidelines: minimum information for publication of quantitative real-time PCR experiments. Clin Chem. 2009;55:611–22.View ArticleGoogle Scholar
- Bustin SA, Benes V, Garson JA, Hellemans J, Huggett J, Kubista M. The need for transparency and good practices in the qPCR literature. Nat Methods. 2013;10:1063–7.View ArticleGoogle Scholar
- Vandesompele J, DePreter K, Pattyn F, Poppe B, VanRoy N, DePaepe A, et al. Accurate normalization of real-time quantitative RT-PCR data by geometric averaging of multiple internal control genes. Genome Biol. 2002;3:1–11.View ArticleGoogle Scholar
- Pfaffl MW, Tichopad A, Prgomet C, Neuvians TP. Determination of stable housekeeping genes, differentially regulated target genes and sample integrity: BestKeeper-excel-based tool using pair-wise correlations. Biotechnol Lett. 2004;26:509–15.View ArticleGoogle Scholar
- Shivhare R, Lata C. Selection of suitable reference genes for assessing gene expression in pearl millet under different abiotic stresses and their combinations. Sci Rep. 2016;6:23036.View ArticleGoogle Scholar
- Cai J, Li PF, Luo X, Chang TL, Li JX, Zhao YW, Xu Y. Selection of appropriate reference genes for the detection of rhythmic gene expression via quantitative real-time PCR in Tibetan hulless barley. PLoS ONE. 2018;13(1):e0190559.View ArticleGoogle Scholar
- Niu XP, Qi JM, Zhang GY, Xu JT, Tao AF, Fang PP, Su JG. Selection of reliable reference genes for quantitative real-time PCR gene expression analysis in Jute (Corchorus capsularis) under stress treatments. Front Plant Sci. 2015;6:848.View ArticleGoogle Scholar
- Ferdous J, Li Y, Reid N, Langridge P, Shi BJ, Tricker PJ. Identification of reference genes for quantitative expression analysis of MicroRNAs and mRNAs in barley under various stress conditions. PLoS ONE. 2015;10(3):e0118503.View ArticleGoogle Scholar
- Hua W, Zhu JH, Shang Y, Wang JM, Jia QJ, Yang JM. Identification of suitable reference genes for barley gene expression under abiotic stresses and hormonal treatments. Plant Mol Biol Rep. 2015;33:1002–12.View ArticleGoogle Scholar
- Silver N, Best S, Jiang J, Thein SL. Selection of housekeeping genes for gene expression studies in human reticulocytes using real-time PCR. BMC Mol Biol. 2006;7:33.View ArticleGoogle Scholar
- Xie F, Xiao P, Chen D, Xu L, Zhang B. miRDeepFinder: a miRNA analysis tool for deep sequencing of plant small RNAs. Plant Mol Biol. 2012;80:75–84.View ArticleGoogle Scholar
- Rapacz M, Stępień A, Skorupa K. Internal standards for quantitative RT-PCR studies of gene expression under drought treatment in barley (Hordeum vulgare L.): the effects of developmental stage and leaf age. Acta Physiol Plantarum. 2012;34(5):1723–33.View ArticleGoogle Scholar
- Woffelman C. DNAMAN for Windows, Version 5.2.10. Lynon Biosoft, Leiden University, Netherlands: Institute of Molecular Plant Sciences, 2004.Google Scholar
- Ruijter JM, Ramakers C, Hoogaars WMH, et al. Amplification efficiency: linking baseline and bias in the analysis of quantitative PCR data. Nucleic Acids Res. 2009;37(6):45.View ArticleGoogle Scholar
- Kubista M, Andrade JM, Bengtsson M, Forootan A, Jonák J, Lind K, Sindelka R, Sjöback R, Sjögreen B, Strömbom L, et al. The real-time polymerase chain reaction. Mol Asp Med. 2006;27:95–125.View ArticleGoogle Scholar
- Chinnusamy V, Schumaker K, Zhu JK. Molecular genetic perspectives on cross-talk and specificity in abiotic stress signalling in plants. J Exp Bot. 2004;55(395):225–36.View ArticleGoogle Scholar
- Jacobsen KS, Nielsen KO, Winther TN, Glebe D, Pociot F, Hogh B. Identification of valid reference genes for microRNA expression studies in a hepatitis B virus replicating liver cell line. BMC Res Notes. 2016;9:38.View ArticleGoogle Scholar
- Chapman JR, Waldenström J. With reference to reference genes: a systematic review of endogenous controls in gene expression studies. PLoS ONE. 2015;10:e0141853.View ArticleGoogle Scholar
- González-Aguilera KL, Saad CF, Chávez Montes RA, Alves-Ferreira M, Folter SD. Selection of reference genes for quantitative real-time RT-PCR studies in tomato fruit of the genotype MT-Rg1. Front Plant Sci. 2016;7:1386.View ArticleGoogle Scholar
- Manoli A, Sturaro A, Trevisan S, Quaggiotti S, Nonis A. Evaluation of candidate reference genes for qPCR in maize. J Plant Physiol. 2012;169:807–15.View ArticleGoogle Scholar
- Cheng Y, Bian WY, Pang X, Yu JH, Ahammed GJ, Zhou GZ, Wang RQ, Ruan MY, Li ZM, Ye QJ, Yao ZP, Yang YJ, Wan HJ. Genome-wide identification and evaluation of reference genes for quantitative RT-PCR analysis during tomato fruit development. Front Plant Sci. 2017;8:1440.View ArticleGoogle Scholar
- Nguyen DQ, Eamens AL, Grof CPL. Reference gene identification for reliable normalisation of quantitative RT-PCR data in Setaria viridis. Plant Methods. 2018;14(1):24.View ArticleGoogle Scholar
- Jaiswal PS, Kaur N, Randhawa G. Identification of reference genes for real-time PCR gene expression studies during seed development and under abiotic stresses in Cyamopsis tetragonoloba (L.) Taub. bioRxiv. 2018;313437.Google Scholar
- Ma R, Xu S, Zhao YC, Xia B, Wang R. Selection and validation of appropriate reference genes for quantitative real-time PCR analysis of gene expression in Lycoris aurea. Front Plant Sci. 2016;7:536.PubMedPubMed CentralGoogle Scholar
- Shi CH, Yang FS, Zhu X, Du EX, Yang YT, Wang SL, Wu QJ, Zhang YJ. Evaluation of housekeeping genes for quantitative real-time PCR analysis of Bradysia odoriphaga (Diptera: Sciaridae). Int J Mol Sci. 2016;17:1034.View ArticleGoogle Scholar
- Liang WX, Zou XX, Lejarazú RC, Wu LJ, Sun WH, Yuan XY, Wu SQ, Li PF, Ding H, Ni L, Huang W, Zou SQ. Selection and evaluation of reference genes for qRT-PCR analysis in Euscaphis konishii Hayata based on transcriptome data. Plant Methods. 2018;14:42.View ArticleGoogle Scholar
- Tang X, Zhang N, Si HJ, Urrea AC. Selection and validation of reference genes for RT-qPCR analysis in potato under abiotic stress. Plant Methods. 2017;13:85.View ArticleGoogle Scholar
- Hu YN, Fu HT, Qiao H, Sun SM, Zhang WY, Jin SB, Jiang SF, Gong YS, Xiong YW, Wu Y. Validation and evaluation of reference genes for quantitative real-time PCR in Macrobrachium Nipponense. Int J Mol Sci. 2018;19:2258.View ArticleGoogle Scholar
- Li WG, Zhang LH, Zhang YD, Wang GD, Song DY, Zhang YW. Selection and validation of appropriate reference genes for quantitative real-time PCR normalization in staminate and perfect flowers of andromonoecious Taihangia rupestris. Front Plant Sci. 2017;8:729.View ArticleGoogle Scholar
- Zhang C, Ge RC, Zhang JW, Chen YJ, Wang HZ, Wei JH, Li RF. Identification and expression analysis of a novel HbCIPK2-interacting ferredoxin from halophyte H. brevisubulatum. PLoS ONE. 2015;10(12):e0144132.View ArticleGoogle Scholar
- Amorim LLB, Ferreira-Neto JRC, Bezerra-Neto JP, Pandolfi V, Araújo FT, Matos MKS, Santos MG, Kido EA, Benko-Iseppon AM. Cowpea and abiotic stresses: identification of reference genes for transcriptional profiling by qPCR. Plant Methods. 2018;14:88.View ArticleGoogle Scholar