Molecular Biology Reports

, Volume 46, Issue 6, pp 6371–6379 | Cite as

Promoter activity of earthworm metallothionein in mouse embryonic fibroblasts

  • Victoria Drechsel
  • Birgit Fiechtner
  • Martina HöcknerEmail author
Open Access
Original Article


The regulation of metallothionein (MT) gene expression as important part of the detoxification machinery is only scarcely known in invertebrates. In vertebrates, MT gene activation is mediated by the metal-transcription factor 1 (MTF-1) binding to metal response elements (MREs). In invertebrates, the mechanisms of MT gene activation seems to be more diverse. In some invertebrate species, MTF-1 orthologues as well as their ability to activate MT genes via MREs have been uncovered. Although earthworm MTs have been well studied, a MTF-1 orthologue has not yet been described and MT gene activation mechanisms are largely unknown. Analyses of the earthworm wMT2 promoter by reporter gene assays have been performed. We could show that the wMT2 promoter was active in mouse embryonic fibroblasts (NIH/3T3) as well as in mouse MTF-1−/−cells (DKO7). The presence of mouse MTF-1 (mMTF1) led to a significant increase in reporter gene activity. We observed that cadmium as well as zinc had an effect on promoter activity. In the presence of zinc, promoter activity doubled in NIH cells, however, we did not observe a significant effect in the DKO7 cell line. Cadmium decreased promoter activity in DKO7 cells, but this effect could be reversed by providing mMTF1 in a co-transfection experiment. We suggest that MT gene expression in the earthworm is not entirely dependent on a MRE binding protein. Interestingly, the shortest promoter fragment including MRE1 showed the highest promoter activity under control conditions.


Metallothionein Gene regulation Earthworm MTF-1 Reporter gene assay 


Metallothioneins (MTs) are a group of small, cysteine-rich proteins with metal binding capacity [1] that respond to a wide range of stimuli. Several types of stress induce transcription, among others free radicals [2], or transition metals like cadmium (Cd) [3], zinc (Zn) [4], and copper (Cu) [5]. The protein family of MTs shares the characteristic cysteine motifs and occur throughout the animal kingdom [6, 7].

In vertebrates, MT gene expression is mediated by the metal-transcription factor 1 (MTF-1) [8], which is a zinc-finger protein in the His2Cys2 family and responsible for basal and metal-dependent transcriptional activation [9]. Hereby, MTF-1 mediates response to transition metals, oxidative stress, and hypoxia [10, 11, 12]. Upon stress, MTF-1 translocates from the cytoplasm into the nucleus [13] binding to metal response elements (MREs) in the promoter region of MT genes [14, 15]. Free Zn is required to activate MTF-1 allowing its DNA binding [16, 17, 18]. Besides six highly conserved zinc fingers [12], MTF-1 consists of three activation domains, a nuclear localization, and an export signal [8]. These mechanisms are evolutionary conserved in human, mouse, fruit fly, fish, or rodents. Although human and mouse MTF-1 are very similar in amino acid sequence and domain structure [19], human MTF-1 showed an intrinsically stronger heavy metal inducibility compared to mouse MTF-1 [20]. Previous studies proposed the acidic activation domain of the human MTF-1 as mediator of metal induction [8]. The MTF-1 of capybara, the largest living rodent, shares a higher sequence similarity to human MTF-1, but the same low metal-responsiveness compared to mouse MTF-1 [21]. Phosphorylation of MTF-1 is supposed to be essential for transactivation of MT [22]—Saydam et al. declared a model, where phosphorylation of MTF-1 is necessary only for the regulation of the nuclear export, whereas transcriptional activation of MTF-1 is mediated by dephosphorylation of specific sites [23].

The knowledge of MT gene regulation in invertebrates on the other hand is scarce. Recently, however, MTF-1 orthologues have been identified in some invertebrate species. Qiu et al. identified a MTF in the Pacific oyster Crassostrea gigas (cgMTF) for the first time in bivalvia [24]. The cgMTF contains four putative zinc finger-like regions and a phylogenetic analysis revealed a high similarity to vertebrate MTF-1. Binding of cgMTF to the MREs in cgMT genes was confirmed under Cd exposure [24]. The pacific abalone Haliotis discus hannai is the first gastropod where MTF-1 was found so far. The abalone MTF-1 shows high similarity within the DNA binding region of vertebrate MTF-1 with its six zinc-finger regions, a short acidic domain, and an auxiliary nuclear localization signal, but no nuclear export signal was observed [25]. Unlike the mammalian MTF-1, the abalone MTF-1 gene includes, among others, a MRE binding site. Therefore, a possible modulation of MTF-1 itself by heavy metals was suggested [25]. After two MT isoforms were identified in the freshwater pearl mussel Hyriopsis schlegelii [26], Wang et al. identified just recently a MTF-like transcription factor [27]. The amino acid sequence of HsMTF-like is relatively short compared to other species; it possesses six putative zinc finger regions, but no transcription activation domain. They further showed, that the expression of HsMT1 and HsMT2 was upregulated upon heavy metal exposure by HsMTF-like binding to MREs [27]. On the other hand, the CiMT-1 promoter of Ciona intestinalis is metal-responsive, contains amongst other putative transcription factor binding sites, four MREs [28], but there is no evidence for the expression of a MTF. The wMT2 promoter of Lumbricus rubellus—wMT2 is involved in Cd detoxification [29], contains three MREs [30], but a MTF-1 orthologue has not been discovered in the earthworm so far. In Helix pomatia, three MT isoforms were identified with different roles in metal homeostasis, namely CdMT, CuMT, and Cd/CuMT [3]—the CdMT contains four MREs and also no MTF-1 has been described [31]. A cAMP-responsive element binding protein (CREB) was suggested to contribute to the transcriptional regulation of the wMT2 gene in L. rubellus [32]. In Caenorhabditis elegans, the leucine zipper transcription factor ATF-7 was identified as regulator of MT [33], but also GATA binding factors are required for Cd-inducible activation [34]. As reviewed previously, other regulatory sequences, besides MREs, are present in the promoter regions of MTs like antioxidant-response elements (AREs), glucocorticoid-response elements (GREs), or cAMP-response elements (CRE) [7]. Therefore, not only MTF-1 but a variety of regulators are involved in MT activation like NF1 [35], and USF-1 [36].

Earthworms are one of the most valuable bioindicators for environmental health [37, 38] and it is known, that they are able to tolerate Cd exposure by inducing MT expression [30, 39], however, the underlying regulatory pathways of MT-based detoxification mechanisms are still unknown. Hence, we accomplished reporter gene assays to characterize the earthworm wMT2 promoter region under control and Cd-exposed conditions in mouse embryonic fibroblasts.

Materials and methods

Cell culture

MTF-1 knockout cells were used to characterize the promoter regions of the wMT2 gene. The mouse DKO7 cell line with a functional knockout of the MTF-1 gene (MTF-1−/−) [9] was a generous gift from Prof. Walter Schaffner (University of Zurich, Switzerland). The cells were cultured in Dulbecco´s Modified Eagle Medium (DMEM) without pyruvate (Life Technologies, USA), supplemented with 8% fetal bovine serum (FBS) (Life Technologies, USA), 1% Penicillin/Streptomycin (Life Technologies, USA), and 1% l-glutamine (Life Technologies, USA). As control cells expressing a functional MTF-1 (MTF-1+/+), the embryonic fibroblast NIH/3T3 cell line was used (LGC Standards, USA) and cultured in DMEM containing pyruvate (Life Technologies, USA), supplemented with 10% calf serum (CS) (Sigma-Aldrich, USA), and 1% Penicillin/Streptomycin (Life Technologies, USA). Both cell lines were maintained in a 37  °C, 5% CO2 incubator and split once a week.

Generation of promoter constructs

The reporter gene consisted of the Renilla luciferase coding sequence driven by four Lumbricus rubellus wMT2 promoter fragments that differed in length (Fig. 1). The wMT2 promoter contains three MRE binding sites [40]. Four forward primers (insert1_Forward: 5′-GGAGAAGAAAAGGGAGGAAA-3′, insert2_Forward: 5′-TGCGTGGCGTTAAAATCT-3′; insert3_Forward: 5′-CGTCACATTTCGCTCTACACA-3′; insert4_Forward: 5′-TCGCTCTACACACGAAGT-3′) and one reverse primer (5′-CAAGTTCAACAGCAGCTT-3′) were designed to PCR amplify the promoter fragments. According to the transcription start site, insert lengths were as follow: insert 1: − 1016 to − 41; insert 2: − 293 to − 41; insert 3: − 218 to − 41; insert 4: − 209 to − 41 (Fig. 1; sequence details in Figure S1). The PCR product was purified with QIAquick PCR Purification Kit (Qiagen, Germany), and cloned into the pGEM-T-Vector System (Promega, USA). After double-digest with HindIII/XmaI (Thermo Fisher Scientific, USA), the fragments were ligated with T4 DNA ligase (Thermo Fisher Scientific, USA) into the pRLnull vector, directly upstream of the Renilla luciferase reporter gene (Promega, USA). The promoter constructs of the reporter gene plasmids have been sent to Microsynth (Switzerland) for sequencing. The plasmids were purified using the EndoFree Plasmid Maxi Kit (Qiagen, Germany). For co-transfection experiments, mouse MTF-1 expression plasmid (pcDNA3_mMTF1) was used, which was generously provided by Carl Séguin (Centre Hospitalier Universitaire de Québec, Canada).
Fig. 1

Schematic overview of insert 1–4. MRE = Metal-response element 1–3, CRE = CREB-binding site, TATA = TATA-Box

Transfection and reporter gene assay

1.5 × 105 cells were seeded into six-well culture plates (Sarstedt, Germany) in a total volume of 2 ml medium. The next day, cells were transfected using Lipofectamine 2000 Reagent (Invitrogen by Thermo Fisher Scientific, USA) diluted in Opti-MEM Medium (Thermo Fisher Scientific, USA) according to manufacturer´s instructions. As internal control, the firefly luciferase reporter (pGL3) was used. A 1:10 ratio of the control- to experimental vector was applied in a total of 3 µg DNA per well. In co-transfection experiments, 0.4 µg accounted for the mouseMTF1 expression plasmid (mMTF1). For the treatments, cells were incubated with serum-free DMEM supplemented with 1% Penicillin/Streptomycin containing 1  µM, 10  µM, or 50  µM cadmium chloride (CdCl2) (Sigma-Adrich, USA) for one or 12 h. After exposure for 1 h, cells were left for 5 h to recover in 2  ml DMEM containing FBS/CS and 1% Penicillin/Streptomycin. For Zn exposures we added 100 µM zinc chloride (ZnCl2) (Sigma-Aldrich, USA) to the recovery media. After passive cell lysis according to the manufacturer´s instructions (Promega, USA), Renilla and firefly luciferase activities were measured for each sample in a 96-well plate (PerkinElmer, USA) on an EnSpire plate reader (Perkin Elmer, USA), using the Dual-Luciferase® Reporter Assay System (Promega, USA). Expression levels were determined as the ratio of Renilla to firefly luciferase activity.

Chromatin immunoprecipitation assay

To verify if phosphorylated CREB/ATF-1 is bound to the specific wMT2 promotor region, the Chromatin Immunoprecipitation SimpleChiP® Plus Kit (New England Biolabs, Great Britain) was used according to manufacturer´s instructions. Since L. rubellus is not commercially available, we used L. terrestris for CHIP experiments. Between the two species, the wMT2 amino acid sequence shows 97% homology and 163 bp of the promoter region shows homology in 96% of nucleotides. In short, L. terrestris were kept in control or Cd-spiked soil (50 mg/kg CdCl2) for 2 weeks. Coelomocytes were then harvested by stimulation with a 9 V battery to expel coelomic fluid through the dorsal pores. To prevent cell aggregation, 50 mM Guaiacol glyceryl ether (Sigma Aldrich, St. Louis, ME, USA) was added to 1x PBS. The cells were fixed with formaldehyde to preserve the protein-DNA interaction. Chromatin was harvested and digested with Micrococcal Nuclease, before it was subjected to immunoprecipitation using the pCREB (Ser133) antibody (Cell-Signaling Technology, Danvers, MA, USA). Any DNA sequence in the coelomocytes of both control- and Cd-exposed earthworms, that was associated with the antibody, built the so-called cross-linked chromatin complex, which was then enriched and identified by quantitative Real-time PCR (Forward primer: 5′-GCACACGGCGAGTCACAGT-3′; Reverse primer: 5′-TTGGTCTGCACGCGTTTTT-3′). The relative enrichment was calculated by normalization to IgG.

Statistical analysis

All data were analyzed using non-parametric tests in Graph Pad Prism 6. A P value below 0.05 was considered statistically significant. Outliers were calculated with Dixon´s Q-Test and Rout-Test. The data set consists of at least 4 biological replicates (detailed number of biological replicates are presented in Table S1) and results are shown as mean values ± SEM.


First, we examined the promoter activity of all inserts under control conditions. After 1 h we observed significantly different activity levels between almost all inserts in both cell lines (Fig. 2). This difference, however, disappeared after 12 h in insert 1–3, whereas the activity of insert 4 increased significantly in both cell lines (Fig. 2). The shortest promoter fragment therefore revealed the highest activity in controls.
Fig. 2

Comparison of the promoter activity of all inserts under control conditions in DKO7 (MTF-1−/−) and NIH/3T3 (MTF1+/+) cells. Samples for measuring promoter activity were taken 1 and 12 h post transfection. Luciferase activity is shown as Renilla to Firefly ratio. A Mann–Whitney Rank Sum test was used for statistical analysis (Graph Pad Prism 6). Error bars represent mean values ± SEM. Letters indicate significant differences (p ≤ 0.05)

Since we wanted to determine promoter inducibility, we tested the activity of all inserts using Cd exposure experiments. In a preliminary experiment, the pRLnull vector without specific MT promoter insert revealed a basic luciferase activity, which decreased in both cell lines upon Cd exposure, however, a significant reduction was only observed in NIH/3T3 cells (Figure S2). Insert 1 revealed significantly decreased activity in DKO7 cells after Cd exposure, which was not the case in NIH/3T3 cells (Fig. 3). Reduced promoter activity in Cd-exposed DKO7 cells could be reversed when mMTF1 was co-transfected. Overexpression of mMTF1 in NIH/3T3 cells also led to an increase of luciferase activity (Fig. 3).
Fig. 3

Promoter activity of insert 1 after exposure to control conditions (C), 10 µM (Cd10), or 50 µM (Cd50) CdCl2 for 1 h and co-transfection with mMTF1 in DKO7 (MTF-1−/−) and NIH/3T3 (MTF-1+/+) cells. Luciferase activity is shown as Renilla to Firefly ratio. A Mann–Whitney´s Rank Sum Test was used for statistical analysis (Graph Pad Prism 6). Error bars represent mean values ± SEM. Stars indicate significant differences (*p ≤ 0.05, ** p < 0.01, ** p < 0.001, ***p < 0.0001), the hashtags indicate significant differences to the respective control (p ≤ 0.05)

The addition of 100 µM Zn to the recovery medium did not cause a significant increase in promoter activity in DKO7 cells. However, the addition of Zn when mMTF1 was over-expressed in NIH/3T3 cells led to an increased insert 1 promoter activity (Fig. 4).
Fig. 4

Promoter activity of insert 1 alone or co-transfected with mMTF1 in DKO7 (MTF-1−/−) and NIH/3T3 (MTF1+/+) cells after exposure to control conditions (C), or 10 µM (Cd10) CdCl2 for 1 h and an addition of 100 µM (Zn) ZnCl2 to the recovery medium. Luciferase activity is shown as Renilla to Firefly ratio. A Mann–Whitney´s Rank Sum Test was used for statistical analysis (Graph Pad Prism 6). Error bars represent mean values ± SEM. Stars indicate significant differences (p ≤ 0.05)

Subsequently, we reduced the Cd exposure concentration to 1 µM (Cd1) CdCl2. In insert 1 we were still able to observe a significant decrease of promoter activity in DKO7 cells after Cd exposure. In NIH/3T3 cells, insert 1 and 2 showed a significant increase in luciferase activity upon exposure to 1 µM CdCl2, whereas the activity of insert 3 and 4 did not change (Fig. 5). In the presence of mMTF1 a significant increase in promoter activity occurs in insert 1, 2, and 3 in DKO7 cells (Fig. 5). Over-expression of mMTF1 in NIH/3T3 cells led to a significantly increased luciferase activity in insert 1 and 3. In the presence of mMTF1 in DKO7 cells, Cd exposure caused a significant increase in insert 3 and 4. However, in mMTF1 over-expressing NIH/3T3 cells, Cd did not lead to a further increase of insert 1 and 4 promoter activity. Interestingly, an activity increase caused by over-expressed mMTF1 in insert 1 and 3 was abolished in insert 2.
Fig. 5

Induction ratio of the four inserts alone or co-transfected with mMTF1 in DKO7 (MTF-1−/−) and NIH/3T3 (MTF-1+/+) cells after exposure to control conditions or 1 µM (Cd1) CdCl2 for 12 h. The induction ratio is shown as log2-fold induction compared to control. A Mann–Whitney´s Rank Sum Test was used for statistical analysis (Graph Pad Prism 6). Error bars represent mean values ± SEM. Letters indicate significant differences among each other, whereas letters in bold indicate significant differences to the respective insert control (p ≤ 0.05)

Table 1, as explained in detail in the following, provides an overview of results we presented in Fig. 6. We observed that in DKO7 cells an effect of mMTF1 in the presence of Cd is obvious in all promoter fragments. Interestingly, insert 3 shows the same behavior in all treatments in DKO7 and NIH/3T3 cells. In contrast to that, insert 2 behaves the exact opposite in all treatments when we compare DKO7 and NIH/3T3 cells. Insert 3 lacks 75 bp including MRE2 in comparison to insert 2. Insert 4 in NIH/3T3 cells is not responsive to Cd, MTF-1, or a combination of both. However, we already demonstrated that insert 4 showed the highest promoter activity under control conditions.
Table 1

Schematic overview of treatment effects on promoter fragments compared in DKO7 (MTF-1−/−) and NIH/3T3 cells (MTF-1+/+)


Cd effect wo/intrinsic mMTF1

Cd effect in the presence of mMTF1

mMTF1 effect

mMTF1 effect in the presence of Cd









Cd vs C

mMTF1 + Cd vs mMTF1

mMTF1 vs C

mMTF1 + Cd vs Cd

Insert 1



Insert 2





Insert 3



Insert 4







Significant differences are shown as arrows indicating an up-or down regulation

X stands for no significant difference

For details of statistical analyses, refer to Fig. 5

Fig. 6

Effect of promoter length on treatments in DKO7 (MTF-1−/−) and NIH/3T3 (MTF-1+/+) cells after exposure to control conditions (C), or 1 µM (Cd1) CdCl2 for 12 h. The log2-fold induction ratio is shown compared to control. A Kruskal–Wallis and Dunn´s multiple comparison Test was used for statistical analysis (Graph Pad Prism 6). Error bars represent mean values ± SEM. Letters indicate significant differences (p ≤ 0.05). The star indicates a significant difference (p ≤ 0.05) of insert 1 between cell lines exposed to 1 µM (Cd1) CdCl2. A Mann–Whitney Rank Sum Test was used (Graph Pad Prism 6)

We compared all inserts regarding treatment effects in both cell lines using fold induction rates shown in Fig. 6. As expected, we observed a strong difference between DKO7 and NIH/3T3 cells regarding Cd exposure. Insert 1 showed a significant difference between the cell lines in contrast to insert 2–4 (Fig. 6a, b). The induction level of insert 2 and 4 differed only significantly in DKO7 cells when mMTF1 was present under control conditions (Fig. 6c, d). The promoter fragments were not different from each other in the presence of mMTF1 in Cd-exposed cells in both cell lines (Fig. 6e, f).

A putative transcription factor binding site along the wMT2 gene promoter is the CRE binding site. The association between the pCREB/pATF-1 protein and CRE was observed in control- and Cd-exposed earthworms. However, no significant difference was found (Fig. 7).
Fig. 7

Relative enrichment of pCREB/pATF-1 normalized to IgG. A Mann–Whitney´s Rank Sum Test was used for statistical analysis (Graph Pad Prism 6). Error bars represent mean values ± SEM. Letters indicate significant differences (p ≤ 0.05)


Analyses of the earthworm wMT2 promoter revealed that the intrinsic transcription factor machinery of mouse embryonic fibroblasts is able to activate the reporter gene. We observed promoter activity even in DKO7 cells that do not express a functioning MTF-1 protein. Specifically insert 4, the shortest promoter construct, containing one MRE binding site, showed a high activity under control conditions in the presence and absence of mMTF1. This activity difference under control conditions between the inserts became obvious after 12 h revealing a consecutive activation of insert 4 over time. Since the reporter gene was expressed in DKO7 cells, we conclude that the promoter activity is not dependent on mMTF1. Furthermore, we suggest that the additional distal promoter regions in insert 1–3 cause a repression of the consecutive activation, which makes sense, considering that MT genes have to be expressed rapidly under stressful conditions and show very low expression levels in controls [39, 41]. The activation of genes in response to stress can be manifold—either way, cells aim at changing their transcriptional landscape within minutes in response to stress [42]. Moreover, in NIH/3T3 cells insert 4 did not respond to Cd, an over-expression of mMTF1 or a combination of both. It is therefore highly probable that this promoter region, including MRE1, is involved in basal transcription of the wMT2 gene.

We used Cd as a known inducer of MT gene expression [29], [30] to check for the induction behavior of the wMT2 promoter. The reporter gene lacking a wMT2 promoter insert showed luciferase activity. Cd decreased this activity suggesting that Cd interferes with the transcriptional or translational machinery of the cells rather than being a wMT2 promoter-driven specific effect. The inhibition of DNA, RNA, and protein biosynthesis by high Cd concentrations was shown in mammalian cells [43]. The Hyriopsis schlegelii HsMT2 promoter in human hepatoblastoma HepG2 cells exposed to 1.5 µM CdCl2 for 12 h also showed an inhibition of the luciferase reporter gene [27]. Zhou et al. revealed that in the yeast Saccharomyces cerevisiae the activity of the RNA Polymerase I is constrained after exposure to 50 µM Cd [44]. A Cd-based decrease of luciferase activity using insert 1 as a promoter also occurred in DKO7 cells in contrast to NIH/3T3 cells. The provision of mMTF1 in DKO7 cells reversed this effect revealing significantly increased promoter activity, which confirms that Cd detoxification depends on the presence of mMTF1.

The activation of mouse MTs in DKO7 cells was shown to be dependent on MTF-1 and Zn [10]. The insert 1 driven reporter gene confirmed that Zn was able to significantly increase also the earthworm MT promoter activity in mMTF1 over-expressing NIH/3T3 cells. We conclude that Cd-induced wMT2 promoter activity in NIH/3T3 cells can be activated in the same manner as vertebrate MTs. We know from previous studies that MT promoters usually contain more than one MRE, which can differ slightly in their core sequence and function. The MT gene promoter of tilapia (Oreochromis aureus) contains for example six functional MREs with six different nucleotide sequences. The so-called MREg shares the nucleotide sequence with MRE2 from the wMT2 promoter, and is, besides others, responsible for MT promoter activity in response to Cd [45]. In the MT2 promoter of Hyriopsis schlegelii two MREs were identified: a proximal MREa and a distal MREb, which confers metal inducibility [27]. Sims et al. determined metal-specific consensus sequences in Drosophila. They proposed that the core sequence of the Cu responsive MRE is TGCAC(A/G)GC, while the core of the Cd-responsive MRE is TGCAC(C/T)GC [46]. Whether the MRE core sequences relate to a metal-specific function still needs clarification. Herein, we could not determine a Cd-responsive MRE sequence.

Besides MTF-1, several other cis or trans factors are of particular importance for MT gene expression [47, 48]. Putative transcription factor binding sites were found in proximity to MRE2, for instance CREB/ATF, USF2, GATA, and C/EPB [40]. We suggest that MRE2 is the most important MRE in response to Cd in the earthworm. The cAMP response element-binding (CREB) protein is one of the transcription factors that are activated upon various types of stress in control of gene expression [42, 49]. A previous finding that the CRE binding site might be responsible for the activation of MT gene activation in earthworms [32, 40] was tested herein using a CHIP assay. We found that the CRE binding site was occupied under both control and Cd-exposed conditions not confirming a Cd-specific effect. It is known, that the upstream stimulatory factors USF1 and − 2 are involved in Cd-induced MT-I gene expression in mice [50]. USF-2 binding sites share the core sequence with CRE/ATF-1. Also, a cooperation of MTF-1 and USF-1 for MT-I gene expression was found in response to Zn [36]. USF could therefore be a Cd-specific regulator of earthworm MT2 gene expression, which has not been tested in the present study.


The earthworm wMT2 promoter can be activated in mouse embryonic fibroblasts even in the absence of MTF-1. We were, however, able to show that the presence of mMTF1 as well as Zn and Cd had a significant effect on reporter gene activity. Interestingly, the shortest promoter fragment showed the highest luciferase activity under control conditions. We suggest that the proximal MT promoter region is responsible for basal gene activity. Moreover, we propose that the MT promoter is repressed under control conditions, which allows a fast response in case of cellular stress probably by releasing negative regulators from the distal promoter region. Further studies will be needed to identify the earthworm MRE binding protein and further transcription factors that are able to activate the MT promoter, specifically in the absence of MTF-1.



Open access funding provided by University of Innsbruck and Medical University of Innsbruck.


This study was funded by the University of Innsbruck, ID 235916.

Compliance with ethical standards

Conflict of interest

The authors declare that they have no conflict of interest.

Supplementary material

11033_2019_5082_MOESM1_ESM.pdf (776 kb)
Supplementary material 1 (PDF 14 kb)


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Authors and Affiliations

  1. 1.Institute of Zoology, Center for Molecular Biosciences InnsbruckUniversity of InnsbruckInnsbruckAustria

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