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Makorin 1 controls embryonic patterning by alleviating Bruno1-mediated repression of oskar translation

  • Annabelle Dold ,

    Contributed equally to this work with: Annabelle Dold, Hong Han, Niankun Liu

    Roles Investigation, Writing – original draft

    Affiliation RNA Epigenetics, Institute of Molecular Biology, Mainz, Germany

  • Hong Han ,

    Contributed equally to this work with: Annabelle Dold, Hong Han, Niankun Liu

    Roles Investigation, Writing – original draft

    Affiliation Department of Biology, McGill University, Montréal, Québec, Canada

  • Niankun Liu ,

    Contributed equally to this work with: Annabelle Dold, Hong Han, Niankun Liu

    Roles Investigation, Writing – original draft

    Affiliation Department of Biology, McGill University, Montréal, Québec, Canada

  • Andrea Hildebrandt,

    Roles Methodology

    Affiliations Chromatin Biology and Proteomics, Institute of Molecular Biology, Mainz, Germany, Genomic Views of Splicing Regulation, Institute of Molecular Biology, Mainz, Germany

  • Mirko Brüggemann,

    Roles Formal analysis

    Affiliation Buchmann Institute for Molecular Life Sciences, Goethe University Frankfurt, Frankfurt, Germany

  • Cornelia Rücklé,

    Roles Formal analysis

    Affiliations Genomic Views of Splicing Regulation, Institute of Molecular Biology, Mainz, Germany, Buchmann Institute for Molecular Life Sciences, Goethe University Frankfurt, Frankfurt, Germany

  • Heike Hänel,

    Roles Methodology

    Affiliation Genomic Views of Splicing Regulation, Institute of Molecular Biology, Mainz, Germany

  • Anke Busch,

    Roles Formal analysis

    Affiliation Bioinformatics Core Facility, Institute of Molecular Biology, Mainz, Germany

  • Petra Beli,

    Roles Supervision

    Affiliation Chromatin Biology and Proteomics, Institute of Molecular Biology, Mainz, Germany

  • Kathi Zarnack,

    Roles Supervision

    Affiliation Buchmann Institute for Molecular Life Sciences, Goethe University Frankfurt, Frankfurt, Germany

  • Julian König,

    Roles Supervision

    Affiliation Genomic Views of Splicing Regulation, Institute of Molecular Biology, Mainz, Germany

  • Jean-Yves Roignant ,

    Roles Conceptualization, Supervision, Writing – review & editing (JYR); (PL)

    Affiliations RNA Epigenetics, Institute of Molecular Biology, Mainz, Germany, Center for Integrative Genomics, Génopode Building, Faculty of Biology and Medicine, University of Lausanne, Lausanne, Switzerland

  • Paul Lasko

    Roles Conceptualization, Supervision, Writing – review & editing (JYR); (PL)

    Affiliations Department of Biology, McGill University, Montréal, Québec, Canada, Department of Human Genetics, Radboud University Medical Center, Nijmegen, Netherlands

Makorin 1 controls embryonic patterning by alleviating Bruno1-mediated repression of oskar translation

  • Annabelle Dold, 
  • Hong Han, 
  • Niankun Liu, 
  • Andrea Hildebrandt, 
  • Mirko Brüggemann, 
  • Cornelia Rücklé, 
  • Heike Hänel, 
  • Anke Busch, 
  • Petra Beli, 
  • Kathi Zarnack


Makorins are evolutionary conserved proteins that contain C3H-type zinc finger modules and a RING E3 ubiquitin ligase domain. In Drosophila, maternal Makorin 1 (Mkrn1) has been linked to embryonic patterning but the mechanism remained unsolved. Here, we show that Mkrn1 is essential for axis specification and pole plasm assembly by translational activation of oskar (osk). We demonstrate that Mkrn1 interacts with poly(A) binding protein (pAbp) and binds specifically to osk 3’ UTR in a region adjacent to A-rich sequences. Using Drosophila S2R+ cultured cells we show that this binding site overlaps with a Bruno1 (Bru1) responsive element (BREs) that regulates osk translation. We observe increased association of the translational repressor Bru1 with osk mRNA upon depletion of Mkrn1, indicating that both proteins compete for osk binding. Consistently, reducing Bru1 dosage partially rescues viability and Osk protein level in ovaries from Mkrn1 females. We conclude that Mkrn1 controls embryonic patterning and germ cell formation by specifically activating osk translation, most likely by competing with Bru1 to bind to osk 3’ UTR.

Author summary

To ensure accurate development of the Drosophila embryo, proteins and mRNAs are positioned at specific sites within the embryo. Many of these factors are produced and localized during the development of the egg in the mother. One protein essential for this process that has been heavily studied is Oskar (Osk), which is positioned at the posterior pole. During the localization of osk mRNA, its translation is repressed by the RNA-binding protein Bruno1 (Bru1), ensuring that Osk protein is not present outside of the posterior where it is harmful. At the posterior pole, osk mRNA is activated through mechanisms that are not yet understood. In this work, we show that the conserved protein Makorin 1 (Mkrn1) is a novel factor involved in the translational activation of osk. Mkrn1 binds specifically to osk mRNA, overlapping with a binding site of Bru1, thus alleviating the association of Bru1 with osk. Moreover, Mkrn1 is stabilized by poly(A) binding protein (pAbp), a translational activator that binds osk mRNA in close proximity to one Mkrn1 binding site. Our work thus helps to answer a long-standing question in the field, providing insight about the function of Mkrn1 and more generally into embryonic patterning in animals.


In the Drosophila embryo, the maternally deposited pole plasm is a site of specialized translation of mRNAs required for germ cell specification and posterior patterning [1]. Numerous mRNAs accumulate in the pole plasm during oogenesis and early embryogenesis through several different localization mechanisms [2,3]. Among these mRNAs is oskar (osk), which localizes during oogenesis to the posterior along a polarized microtubule network [4] and via a trapping mechanism [5]. Several lines of evidence indicate that osk is the primary determinant that specifies germ cells and posterior patterning. Ectopic expression of osk at the anterior can induce a second set of pole cells and a bicaudal embryonic segmentation pattern with mirror-image posterior segments [6,7]. Mutations such as Bicaudal-D (Bic-D), ik2, and others that produce a duplicated anterior focus of osk mRNA also produce bicaudal embryos [810]. Conversely, embryos from females carrying hypomorphic loss-of-function mutations of osk lack posterior segmentation and pole cells [11]. Mutations in a number of other genes can produce a similar phenotype, and these are collectively known as posterior-group genes [12]. Some of these genes (for example cappuccino, chickadee, spire and staufen (stau)) are required for posterior localization of osk. A failure to deploy osk produces the posterior-group phenotype in these mutants [13,14]. Other posterior-group genes (for example vasa (vas), tudor, nanos (nos), and aubergine (aub)), produce mRNAs and/or proteins that also accumulate in pole plasm and operate downstream of osk [1517].

osk translation is under elaborate temporal and spatial regulation, ensuring that Osk protein becomes abundant only in the posterior pole plasm and not before stage 9 of oogenesis [18,19]. A key repressor of osk translation prior to that stage and outside the pole plasm is Bruno1 (Bru1), which interacts with binding sites called Bru1 response elements (BREs) in the osk 3’ UTR. Mutations affecting the BREs result in premature and excessive Osk expression [1820]. Two mechanisms have been proposed for Bru1-mediated repression of osk translation. In the first, Bru1 recruits Cup, which inhibits assembly of an active cap-binding complex by competitively inhibiting eIF4G for binding to eIF4E [21]. The second mechanism involves oligomerization of osk mRNA into large ribonucleoprotein particles (RNPs) that are inaccessible to the translational machinery [2224]. These mechanisms may be connected, in that physically concentrating osk mRNA molecules in RNPs can enable regulation in trans through inter-molecular interactions. For instance, Bru1 bound to the 3’ end of one osk mRNA molecule could recruit Cup to eIF4E bound to the 5’ cap structure of another osk mRNA molecule, thus repressing its translation [25,26]. Importantly, osk translation and osk mRNA localization are tightly coupled. In nonsense osk alleles or when 3’ UTR elements required for translational activation are mutated, osk mRNA localizes transiently to the pole plasm but its accumulation is not maintained [9,27,28].

While several proteins have been implicated in activating osk translation in the pole plasm [14,29,30], a comprehensive picture of how this is achieved has not yet emerged. For instance, it has been proposed that activation of osk translation involves inhibition of Bru1 [24]. Related to this, a BRE-containing region in the distal part of the osk 3’ UTR (BRE-C) functions in repression as well as in activation [25]. Nevertheless, the mechanism underlying the dual function of this element has not yet been solved.

Large-scale in situ hybridization screens have identified many other mRNAs that localize to the pole plasm [3,31], and some of the corresponding genes could potentially be involved in osk regulation. To search for new posterior-group genes, we previously expressed shRNAs targeting 51 different mRNAs that accumulate in the pole plasm to determine if doing so produced defects in posterior patterning or pole cell formation. We observed that a substantial proportion of embryos produced by Makorin 1 (Mkrn1) knockdown females showed a posterior-group phenotype [32]. Makorin proteins are conserved in plants, fungi, and animals, and contain a RING-domain as well as one or more C3H-type zinc fingers (ZnF) [33]. The role of Makorin proteins is somewhat enigmatic despite their widespread evolutionary conservation. Mammalian MKRN1 has been identified as an E3 ubiquitin ligase that promotes degradation of target proteins [3436], but proteomic analysis does not support an association with proteasome components [37,38]. Furthermore MKRN1’s shorter isoform stimulates translation in rat forebrain neurons but the mechanism is currently unknown [39].

Here, we analyzed the function of Mkrn1 during oogenesis and early embryogenesis. We generated several alleles that alter different domains of the Mkrn1 coding sequence. Using these mutants, we found that Mkrn1 is required for accumulation of Osk protein at the posterior pole of the oocyte. We also show that Mkrn1 is not required for osk mRNA localization, but essential for its translation. Furthermore, we present evidence that Mkrn1 directly binds to the osk 3’ UTR via its N-terminal zinc finger domain. Using Drosophila S2R+ cells we further found that binding of Mkrn1 to osk partially overlaps with the BRE-C domain, adjacent to an A-rich region that recruits pAbp to the osk 3’ UTR [40]. Moreover, the association between Mkrn1 and osk mRNA is stabilized by the physical association with pAbp. Strikingly, depletion of Mkrn1 results in an increased level of Bru1 binding to osk 3’ UTR and reduction of bru1 gene dosage partially rescues Mkrn1 mutant phenotypes. Based on these data we propose that Mkrn1 competes with Bru1 for osk mRNA binding, thus positively regulating osk translation and explaining the specific role of BRE-C in translational activation.


The Drosophila genome includes four Makorin-related genes

In many organisms, up to four distinct genes encoding members of the Makorin family exist, but only one such gene, Mkrn1, has been annotated in Drosophila. To investigate whether flies are unusual in this regard, we searched for sequences similar to human MKRN1. This analysis uncovered four Drosophila genes, Mkrn1, CG5334, CG5347, and CG12477, with substantial similarity to MKRN1 (S1A Fig). All four predicted polypeptides from these genes contain a region of approximately 130 amino acids that is highly conserved and contains a RING-domain as well as C3H-type zinc fingers (ZnF). The proteins are otherwise more divergent from one another, with the exception that all but CG12477 contain a ZnF domain near the amino-terminus.

To analyze the differences in their functionalities, we first determined the expression profile of all four Makorin genes during development. Mkrn1 mRNA is expressed at detectable levels at all developmental stages (Fig 1A) and clearly peaks in early (0–2.5 h) embryos and ovaries. In contrast, expression of the other three Makorin genes is undetectable during early development but peaks in pupae and adult males (S1B Fig). From these results, we conclude that Mkrn1 is the gene of the family most predominantly expressed in ovaries and early embryos and suggest that the three other genes could be specifically expressed in testes.

Fig 1. Mkrn1 alteration affects ovarian development.

(A) Relative Mkrn1 mRNA levels (normalized to RpL15 mRNA) at various stages of development, measured by quantitative RT-PCR. Error bars depict Stdev, n = 3. (B) Schematic diagram of the proteins encoded by the Mkrn1 alleles used to analyze its function in vivo. Mkrn1N is a null allele and produces no protein. (C-F) Bright-field micrographs of entire ovaries from wild-type and Mkrn1 mutant flies. Note the reduced size of Mkrn1S and Mkrn1N ovaries. Scale bars, 500 μm. (G-J) Individual egg chambers stained with the DNA marker DAPI. Fewer stage 10 and older egg chambers are present in Mkrn1S and no late stage egg chambers are present in Mkrn1N ovaries. Abscission defects resulting from inappropriate follicle cell migration are frequently observed in Mkrn1N ovaries (J, arrow). Scale bars, 20 μm. (K-N) Individual egg chambers stained with α-Lamin to highlight nuclear membranes. Scale bars, 20 μm. (M) The oocyte nucleus (marked with an arrow in K, L, and M) remains at the posterior of Mkrn1S oocytes. (N) Some Mkrn1N egg chambers have 16 germline cells whose nuclei are all of similar size, suggesting a defect in oocyte differentiation. Note also irregularities in the follicle cell monolayer in the Mkrn1N egg chamber. (O-Q) Dark-field photographs of eggs and embryos produced by wild-type and Mkrn1 mutants Scale bars, 100 μm. (P) Most embryos produced by Mkrn1W females have a posterior-group phenotype. (Q) Eggs produced by Mkrn1S females lack dorsal appendages and do not support embryonic development. (R, S) Immunostaining with α-Ftz (red) and α-Vas (green) reveals segmentation defects and the absence of pole cells in Mkrn1W embryos Scale bars, 50 μm. (T, U) Surface images of embryos immunostained with α-Ftz (red) to better illustrate segmentation defects in Mkrn1W embryos. Scale bars, 50 μm.

Mkrn1 mutants reveal essential roles in oogenesis and embryogenesis

To elucidate the role of Mkrn1, we used CRISPR/Cas9 to produce three different mutant alleles: Mkrn1N, a complete deletion of the coding sequence, Mkrn1S, a frameshift mutation that is predicted to produce a C-terminally truncated protein of 124 amino acids, including only ZnF1 among conserved domains, and Mkrn1W, a small in-frame deletion that disrupts only the ZnF1 domain (Fig 1B). In the strong Mkrn1 mutants (Mkrn1S and Mkrn1N), most egg chambers cease development at or before stage 10 (Fig 1C–1J). The nuclei of Mkrn1S oocytes that progress as far as stage 9 or later remain at the posterior, failing to migrate to the antero-dorsal corner (Fig 1M). The very few eggs laid by Mkrn1S females have no dorsal appendages and do not develop (Fig 1Q). Mkrn1N egg chambers do not progress as far as stage 9 and showed variable defects in early oogenesis including failure of oocyte differentiation (Fig 1N) and inappropriate follicle cell migration (Fig 1J and 1N). On the other hand, ovaries of females homozygous for Mkrn1W have a similar morphology to wild-type (Fig 1C and 1D). Mkrn1W mutant ovaries completed oogenesis and produced fertilizable eggs in similar numbers as wild-type controls (Fig 1G, 1H, 1K and 1L, Table 1). To examine the role of Mkrn1 in embryonic patterning, we compared cuticle preparations of wild-type and Mkrn1W embryos (Fig 1O and 1P). We found that most Mkrn1W embryos lack posterior segments, a phenotype similar to osk mutants and to what we previously observed at lower frequency from females expressing shRNA targeting Mkrn1 [32]. To investigate this more closely, we stained wild-type and Mkrn1W embryos for Fushi tarazu (Ftz) and Vas proteins. In wild-type blastoderm-stage embryos, Ftz is expressed in seven stripes along the anterior-posterior axis, while in posterior-group embryos the number of Ftz stripes is usually reduced to four (Fig 1R and 1T, [41]). At blastoderm stage in wild-type embryos, Vas-positive pole cells are clustered at the posterior pole [16] (Fig 1R). Consistent with a posterior-group phenotype, we observed four Ftz stripes in 65% of Mkrn1W embryos (30/46) (Fig 1S and 1U). Most of the remaining embryos had even fewer Ftz stripes with an additional broad domain of Ftz expression. In addition, 95% of Mkrn1W embryos (63/66) showed no pole cells by Vas staining (Fig 1S). The posterior patterning defects result in lethality for most (97%) Mkrn1W embryos. However, the small number of Mkrn1W embryos that hatch into viable larvae (40/1222, 3.3%, Table 1) can complete development to adulthood.

Table 1. Expression of tagged Mkrn1 from transgenes rescues oogenesis and viability to embryos produced by Mkrn1 mutant females.

Mkrn1 accumulates in the pole plasm during oogenesis

To examine the distribution of Mkrn1 in the germline, we expressed transgenic Venus- and FLAG-tagged Mkrn1 using a nos>GAL4 driver. Since Mkrn1 females could be rescued to fertility by germline specific expression of these transgenes (Table 1), we concluded that these tagged transgenes are functional, and thus inferred that their localization should reflect the endogenous one. When expressed in ovaries, Venus- or FLAG-tagged Mkrn1 (subsequently called Mkrn1) becomes detectable in a uniform distribution in germline cells from early oogenesis. We observed a mild accumulation of Mkrn1 in cytoplasmic particles resembling nuage at the outer surface of nurse cell nuclear membranes and in the early oocyte (Fig 2A, 2G and 2M). In later egg chambers, Mkrn1 remains abundant in nurse cells and is tightly localized in the pole plasm in the oocyte (Fig 2D, 2J and 2P). Next, we conducted double labeling experiments in wild-type ovaries to determine the degree of colocalization between Mkrn1 and known pole plasm components. In both, stage 8 and stage 10 oocytes, Mkrn1 co-localizes extensively with Stau (Fig 2A–2F), osk mRNA (Fig 2G–2L), Osk protein (S2A–S2F Fig), Vas (S2G–S2L Fig) and Aub (Fig 2M–2R). This close association between Mkrn1 and many important pole plasm components suggests that Mkrn1 is an integral component of pole plasm.

Fig 2. Mkrn1 accumulates in pole plasm.

(A-C) The three panels show the same egg chambers stained for (A) Venus-Mkrn1, (B) Stau, and a (C) merged image. Scale bars, 25 μm. Venus-Mkrn1 expression was driven by nos>Gal4. Colocalization of Venus-Mkrn1 and Stau can be observed in particles that have not yet accumulated at the posterior of the early stage 8 oocyte. (D-F) The three panels show the same stage 10 egg chamber stained for (D) Venus-Mkrn1, (E) Stau and (F) a merged image. Scale bars, 25 μm. There is extensive colocalization of Venus-Mkrn1 and Stau in the posterior pole plasm of the oocyte. (G-I) The three panels show the same egg chambers stained for (G) Venus-Mkrn1, (H) osk mRNA, and (I) a merged image. Scale bars, 25 μm. Colocalization of Venus-Mkrn1 and osk can be observed in an early stage 8 oocyte where osk has not yet fully localized at the posterior of the oocyte. (J-L) The three panels show the same stage 10 egg chamber stained for (J) Venus-Mkrn1, (K) osk mRNA and (L) a merged image. Scale bars, 25 μm. There is extensive colocalization of Venus-Mkrn1 and osk mRNA in the posterior pole plasm of the oocyte. (M-O) The three panels show the same egg chambers stained for (M) Venus-Mkrn1, (N) Aub, and a (O) merged image. Scale bars, 5 μm. Colocalization of Venus-Mkrn1 and Aub can be observed at the nuage surrounding the nurse cell nuclei (P-R). The three panels show the same egg chambers stained for (P) Venus-Mkrn1, (Q) Aub, and a (R) merged image. Scale bars, 20 μm. There is extensive colocalization of Venus-Mkrn1 and Aub in the posterior pole plasm of the oocyte.

To determine whether Mkrn1 depends on the pole plasm assembly pathway for its posterior localization, we expressed the tagged Mkrn1 transgenes in osk (osk54/Df) and vas (vasPH165/vas1) mutant backgrounds. We found that loss of osk abolished Mkrn1 localization (S3A Fig). In contrast, Mkrn1 localized normally to the posterior in vas mutant oocytes (S3B Fig), placing Mkrn1 between osk and Vas in the pole plasm assembly pathway.

To obtain insights into the link between Mkrn1 and pole cell determination, we collected embryos from females trans-heterozygous for a Mkrn1 allele and for either a vas or osk allele. Next, we compared the number of pole cells with single heterozygous controls. When heterozygous, Mkrn1W or Mkrn1S had little effect on pole cell number. However, either allele reduced the number of pole cells produced by vas1 heterozygotes, and further by osk54 heterozygotes (S4 Fig). These data support a genetic interaction between Mkrn1 and genes involved in embryonic patterning and pole cell specification.

Mkrn1 ensures correct deployment of specific mRNAs and proteins involved in embryonic patterning

To address whether Mkrn1 mutations may affect the distribution of proteins involved in embryonic patterning, we performed immunostaining experiments. We found a striking reduction in posterior accumulation of Osk in oocytes from all Mkrn1 alleles (Fig 3A–3D). For Stau, we observed weaker and more diffuse posterior localization in Mkrn1W, as compared to wild-type (Fig 3E and 3F) and no localized protein in Mkrn1S and Mkrn1N (Fig 3G and 3H). On the other hand, Grk localized normally to the antero-dorsal corner of Mkrn1W oocytes (Fig 3I and 3J). In Mkrn1S, Grk was observed at reduced levels associated at the posterior with the mislocalized oocyte nucleus (Fig 3K) and diffusely distributed at a very low level in Mkrn1N (Fig 3L). Posterior localization of Aub and Vas was lost in oocytes of all Mkrn1 mutant alleles (Fig 3M–3T). Finally, Orb localization was unaffected in Mkrn1W (Fig 3U and 3V), but was concentrated at the posterior in Mkrn1S (Fig 3W). Many Mkrn1N egg chambers included a single Orb-positive cell (Fig 3X), indicating that, in these cases, oocyte differentiation had taken place. Importantly, normal accumulation of all proteins could be restored by nos>GAL4 driven expression of a tagged Mkrn1 transgene (S5 Fig), confirming the specificity of the Mkrn1 phenotypes.

Fig 3. Mkrn1 mutations affect accumulation of proteins involved in axis patterning.

(A-D) Posterior accumulation of Osk is greatly reduced in stage 10 Mkrn1W and Mkrn1S oocytes as compared with wild-type. Osk is nearly undetectable in Mkrn1N egg chambers. Scale bars, 25 μm. (E-H) Posterior accumulation of Stau is greatly reduced in stage 10 Mkrn1W and Mkrn1S oocytes as compared with wild-type. Stau is nearly undetectable in Mkrn1N egg chambers. Scale bars, 25 μm. (I-L) Anterodorsal accumulation of Grk is normal in stage 10 Mkrn1W oocytes. Grk remains associated with the oocyte nucleus and is mislocalized to the posterior in stage 10 Mkrn1S oocytes. Grk is present at uniformly low levels or undetectable levels in all germ cells in Mkrn1N egg chambers. Scale bars, (I-K) 20 μm, (L) 25 μm. (M-P) Posterior accumulation of Aub is greatly reduced in stage 10 Mkrn1W and Mkrn1S oocytes as compared with wild-type. Aub is present at uniform levels in all germ cells in Mkrn1N egg chambers. Scale bars, 20 μm. (Q-T) Posterior accumulation of Vas is greatly reduced in stage 10 Mkrn1W and Mkrn1S oocytes as compared with wild-type. Vas is present at uniform levels in all germ cells in Mkrn1N egg chambers. Scale bars, 25 μm. (U-X) Accumulation of Orb is similar in wild-type and Mkrn1W oocytes, but Orb is more concentrated in the posterior of Mkrn1S oocytes. In early-stage Mkrn1N egg chambers there is usually a single Orb-positive cell, indicating that some steps toward oocyte differentiation are able to take place. Scale bars, (U-W) 20 μm, (X) 25 μm.

Mkrn1W oocytes transiently accumulate osk mRNA at the posterior pole but do not produce Osk protein

To investigate whether the primary effect of Mkrn1W on Osk deployment occurred at the level of RNA localization or translation, we examined more closely the effects of Mkrn1W on osk expression. Therefore, we performed in situ hybridization for osk mRNA and immunostaining for Osk protein on the same samples (Fig 4A). In stage 7 egg chambers, osk mRNA accumulation is robust in both wild-type and Mkrn1W oocytes. Faint expression of Osk protein is occasionally visible in wild-type stage 7 oocytes but never in similarly staged Mkrn1W oocytes. This difference becomes more pronounced in stages 9 and 10A. While 95% (41/43) of stage 9-10A Mkrn1W oocytes show posterior accumulation of osk mRNA, only 7% (3/43) of Mkrn1W oocytes show even a faint posterior signal for Osk protein. All (20/20) similarly-staged wild-type oocytes show strong posterior accumulation of both osk mRNA and Osk protein (Fig 4A). Subsequently, posterior accumulation of osk mRNA is lost in Mkrn1W oocytes. In 88% of stage 10B Mkrn1W oocytes (30/34), osk mRNA remains in a tight focus, but is no longer anchored at the posterior pole (Fig 4A). osk translation remains repressed with only 6% of stage 10B Mkrn1W oocytes (2/34) having detectable posterior Osk. In later Mkrn1W oocytes, neither osk mRNA nor Osk protein is detectable at the posterior. We conclude from these experiments that Mkrn1 is not directly required for the localization of osk mRNA at the posterior pole but is necessary for its translation. Consistent with previous observations in other conditions that abrogate Osk anchoring or translation [9,27,28,42], posterior accumulation of osk mRNA is not maintained in Mkrn1W oocytes because of their failure to accumulate localized Osk protein. To confirm these results, we compared Osk protein levels by western blot analysis and osk mRNA levels by quantitative PCR (qPCR). Consistent with our immunostaining experiments, we observed a pronounced reduction in Osk protein (Fig 4B), but only minor positive or negative effects on osk mRNA depending on the particular Mkrn1 allele (Fig 4C).

Fig 4. Translation of osk mRNA is impaired in Mkrn1W ovaries.

(A) Fluorescent in situ hybridization for osk mRNA (red) with co-immunostaining for Osk protein (green) in wild-type and Mkrn1W egg chambers. For each genotype and in each column the top and bottom images are of the same egg chamber. In wild-type oocytes posterior accumulation of osk mRNA and Osk protein is robust and stable from stage 9 onward. In Mkrn1W oocytes accumulation of osk mRNA resembles the wild-type pattern through stage 10A but is not maintained, while Osk protein is rarely detectable at the oocyte posterior at any stage. Scale bars, 25 μm. (B) Western blot analysis from ovary lysates of various genotypes stained for Osk, pAbp and β-tubulin. Osk protein levels are greatly reduced in all Mkrn1 mutant alleles. 1 day-old young females have not yet completed oogenesis and were used as a control for Mkrn1S and Mkrn1N ovaries which also lack late-stage egg chambers, where Osk is most abundant. (C) RT-qPCR experiments measuring ovarian osk mRNA levels (normalized to RpL15 mRNA) in the same genotypes as (B). mRNA levels of ovaries from adult females were compared to Mkrn1W ovaries. For Mkrn1S and Mkrn1N ovaries, mRNA levels of 1 day-old young ovaries was used as normalization. Error bars depict Stdev, n = 2.

Mkrn1 mutants affect localization of other maternal mRNAs

We further used fluorescent in situ hybridization to investigate the distribution of several other mRNAs involved in patterning in Mkrn1 mutants. Consistent with what we observed for Grk protein, localization of grk mRNA was similar to wild-type in Mkrn1W, but grk mRNA remained at the posterior in Mkrn1S oocytes (S6A–S6C Fig). Posterior accumulation of osk, nos and polar granule component (pgc) mRNAs was also lost in Mkrn1W embryos (S6D–S6I Fig).

Mkrn1 associates with factors involved in osk mRNA regulation

To gain further insights into the molecular pathways underlying Mkrn1 function we sought to identify potential cofactors. For this purpose, we expressed Myc-tagged Mkrn1 in Drosophila S2R+ cultured cells and carried out immunoprecipitation (IP) experiments followed by mass spectrometry analysis. We also repeated this experiment using a version of Mkrn1 carrying a point mutation in the RING domain (Mkrn1RING), as we noticed that this construct was expressed at a higher level compared to the wildtype one, which appears to be unstable after transfection in cells (S7A and S7B Fig). Similar stability characteristics have been reported for mammalian MKRN1 [34]. Numerous RNA-binding proteins were enriched after IP (S7C and S7D Fig). Among those, several have been already linked to osk mRNA localization and translation [21,40,4345]. To validate these interactions, we performed co-IP experiments in S2R+ cells between Mkrn1RING and various interaction partners in the presence or absence of RNase T1. Using this approach, we could confirm the interaction of Mkrn1RING with poly(A) binding protein (pAbp), IGF-II mRNA-binding protein (Imp), eukaryotic initiation factor 4G (eIF4G), Squid (Sqd) and maternal expression at 31B (Me31B) (S8A–S8E Fig). All of these interactions persisted upon RNase treatment, suggesting they are direct. We can however not exclude the possibility that the poly(A) tail, which is not affected by treatment with RNase T1, mediates these interactions. Interestingly, several of the identified proteins have already been shown to interact with each other [43,44,4648]. We also confirmed that interactions between FLAG-tagged Mkrn1 and pAbp as well as eIF4G also occur in ovaries (Fig 5A and S8F Fig).

Fig 5. Mkrn1 interacts strongly with the poly(A) binding protein.

(A) Western blot analysis of co-IP experiments between Venus-Mkrn1 and pAbp. α-Tubulin (lanes 1, 2) and ovaries lacking the Venus-Mkrn1 transgene (lane 4) were used as negative controls. (B) Co-expression of pAbp stabilizes Mkrn1. FLAG-Mkrn1 was co-transfected with increasing levels of HA-pAbp in S2R+ cells. Left: Proteins were examined using immunoblotting. Right: Intensities of FLAG-Mkrn1 levels were quantified and normalized to intensities of β-tubulin. The relative intensity was normalized to Mkrn1 mRNA levels (normalized to RpL15 mRNA) analyzed by RT-qPCR. Error bars depict SEM, n = 9. (C) PAM2 motif alignment in different species. Comparison between Drosophila and human PAM2 motif revealed a Glu to Val substitution (orange) in the consensus sequence. The conserved amino acid sequence to Drosophila (dark purple) is indicated below. The PAM2 motif was mutated using two amino acid substitutions at positions 90 and 92 to alanine (F90A and P92A). (D) Immunoblot analysis of co-IP experiments between FLAG-Mkrn1 and pAbp in S2R+ cells. The interaction of pAbp and Mkrn1 is reduced when the PAM2 motif is mutated. (E) Rescue experiments of wild-type or mutant Mkrn1 in Mkrn1N mutants. FLAG-Mkrn1 or FLAG-Myc-Mkrn1PAM2 was overexpressed in ovaries using a nos>Gal4 driver line. Ovarian protein lysates from rescued females were analyzed by immunoblotting together with wild-type and Mkrn1N as controls. While Mkrn1 overexpression could restore Osk protein level to approximately wild-type, Mkrn1PAM2 depicted decreased protein levels similar to Mkrn1N. (F) Egg chambers from (top panel) Mkrn1W, (middle panel) pAbp/+, and (bottom panel) pAbp/+; Mkrn1W females stained with DAPI and immunostained for Orb, an oocyte marker. pAbp/+; Mkrn1W ovaries show diverse developmental defects. Scale bars, 25 μm except for the lower left panel, where the scale bar is 50 μm. (G) Time course of fecundity of Mkrn1W and pAbp/CyO; Mkrn1W females.

Furthermore, we found that the stability of Mkrn1 itself was enhanced upon co-transfection of pAbp in S2R+ cells (Fig 5B). Mammalian MKRN1 contains a PCI/PINT associated module 2 (PAM2) motif, that is present in several pAbp binding proteins and is required in MKRN1 for binding to PABP [39,49]. We identified a similar motif in Drosophila Mkrn1 (Fig 5C), but with one variation compared to human (V instead of E at position 9) that likely explains why this PAM2 motif was not recognized previously. To address the functionality of this motif we repeated the co-IPs, and found that when this domain was mutated (Mkrn1PAM2, Fig 5C), the interaction between Mkrn1 and pAbp was compromised in S2R+ cells (Fig 5D). Based on these data, we conclude that Mkrn1 exists in one or several complexes that contain factors involved in the regulation of osk mRNA translation, and stably interacts with pAbp via its PAM2 motif. If the interaction of Mkrn1 with pAbp is indeed required for the function of Mkrn1, Mkrn1PAM2 should not be able to rescue the Mkrn1N phenotype. Indeed, we found that overexpression of Mkrn1PAM2 in Mkrn1N ovaries could not rescue Osk protein levels and posterior localization compared to wild-type Mkrn1 (Fig 5E and S9B Fig). Moreover, we observed a strong modifier effect between Mkrn1W and pAbp mutations; Mkrn1W homozygotes and pAbp heterozygotes complete oogenesis, but many egg chambers from pAbp/+; Mkrn1W females show severe defects, including supernumerary germ cells, missing or duplicated oocytes, or more extreme dysmorphologies (Fig 5F). These females can produce eggs, but only for the first 2–3 days of life (Fig 5G), and these eggs did not support embryonic development. We thus conclude that the interaction of Mkrn1 with pAbp is essential for its function during oogenesis.

Mkrn1 associates specifically with osk mRNA in vivo

The effects we observed on osk translation in late Mkrn1 egg chambers prompted us to test whether Mkrn1 can interact with osk mRNA. First, to assess whether Mkrn1 can bind to RNA in general, we immunoprecipitated FLAG-Mkrn1 after transfection of S2R+ cells and UV crosslinking. Mkrn1-bound RNA was subsequently labeled, and the protein-RNA complexes were visualized by autoradiography (S10A Fig). While a higher concentration of RNase I (1/50 dilution) resulted in a focused band, a lower concentration (1/5000 dilution) produced a shift of the Mkrn1-RNA complexes, demonstrating the RNA binding ability of Drosophila Mkrn1. We next repeated this experiment with various mutations in different Mkrn1 domains (S7A and S10A Fig). While mutations that alter the RING (Mkrn1RING) or the ZnF2 domain (Mkrn1ZnF2) behave as wild-type Mkrn1, deletion of the ZnF1 domain (Mkrn1ΔZnF1) resulted in a reduction of labeled Mkrn1-RNA complexes. These findings demonstrate that Drosophila Mkrn1 can bind to RNA and the ZnF1 domain is critical for this binding.

To confirm that Mkrn1 binds osk mRNA in vivo, we overexpressed either FLAG-tagged wild-type Mkrn1 or Mkrn1ΔZnF1 in ovaries and performed RNA IP (RIP) experiments. The enrichment of different mRNAs was analyzed by qPCR using primers that bind to the 3’ UTRs of the respective transcripts. Interestingly, we observed that osk mRNA was substantially enriched in Mkrn1 IPs, but much less so when using Mkrn1ΔZnF1 (Fig 6A and S10B Fig). On the other hand, bicoid (bcd) and grk mRNAs were not detected above background levels in either RIP experiment. This provides evidence that Mkrn1 binds specifically to osk mRNA in ovaries and that its ZnF1 domain is important for this interaction.

Fig 6. Mkrn1 associates specifically with the 3’ UTR of osk mRNA.

(A) RIP experiment. Either FLAG-tagged Mkrn1 or Mkrn1ΔZnF1 was overexpressed in Mkrn1N ovaries using nos>GAL4 driver. Enrichment of different transcripts was analyzed by RT-qPCR using primers that bind to the respective 3’ UTRs. Fold enrichment is presented relative to the control (nos>GAL4 driver alone, ctrl). Error bars depict SEM, n = 3. Multiple t-test was used to analyze significant changes compared to control RIP. (B) iCLIP results from S2R+ cells showing specific binding of Mkrn1 to osk in a region of the 3’ UTR that partially overlaps with the BRE-C site (yellow). The peaks (purple) indicate crosslinking events of Mkrn1 to osk. Data of two technical replicates for FLAG-Mkrn1 is shown. The same experiment performed with FLAG-GFP (ctrl) did not show specific peaks. (C) RIP experiments of FLAG-Mkrn1RING in S2R+ cells. Enrichment of luciferase-osk-3’UTR transcript was analyzed by RT-qPCR compared to IP experiments with FLAG-GFP. Mkrn1RING Binding to osk 3’ UTR is compromised when introducing a deletion of the Mkrn1 binding site (oskΔMkrn1, deletion of nucleotides 955–978 of osk 3’ UTR). Error bars depict SEM, n = 4. (D) Binding of Mkrn1RING to luciferase-osk-3’UTR reporter is reduced in S2R+ cells when using a deletion of the A-rich region of osk 3’ UTR (oskΔAR, deletion of nucleotides 987–1019 of osk 3’ UTR). Fold change illustrates the difference of pulled-down oskΔAR reporter compared to IP with wild-type osk 3’ UTR. The RIP experiments were normalized to FLAG-tagged GFP. Error bars depict SEM, n = 4. (E) RIP experiments were performed in either control cells or upon depletion of Imp or pAbp. Enrichment was calculated compared to FLAG-GFP. The relative change in Mkrn1RING binding to luciferase-osk-3’UTR reporter in knockdown cells compared to LacZ-depleted cells is depicted. Depletion of pAbp compromises binding of Mkrn1. Error bars depict SEM, n = 3. (F) RIP experiments showing that FLAG-Mkrn1 binding to luciferase-osk-3’UTR is dependent on the ZnF1 domain as well as on the PAM2 motif. Enrichment was analyzed using RT-qPCR and the relative change in binding compared to RIP of FLAG-Mkrn1 is illustrated. RIP experiments were performed in S2R+ cells using FLAG-GFP as control. Error bars depict SEM, n ≥ 3.

To determine precisely where Mkrn1 binds to osk mRNA, we performed individual nucleotide resolution cross-linking and immunoprecipitation (iCLIP), an unbiased approach to identify RNA-binding sites of a protein of interest [50]. This condition ensured that all Mkrn1 protein-RNA complexes were potentially recoverable in the immunoprecipitations. To this end, we overexpressed FLAG-tagged Mkrn1 in S2R+ cells and performed iCLIP experiments (S10C Fig). Since osk is poorly expressed in these cells, we co-transfected a genomic construct of osk under the control of an actin promoter. We found specific binding sites in a handful of genes, including osk, ranking at third position in term of read coverage (S10D Fig), in which Mkrn1 binding sites were located in the distal part of the 3’ UTR (Fig 6B). These sites fall just upstream of an A-rich sequence that associates with pAbp [40]. Moreover, the binding site of Mkrn1 partially overlaps with the BRE-C site, which is bound by Bru1 and is required for both repression and activation of osk translation [25].

To validate the identified Mkrn1 binding sites, we performed RIP experiments in S2R+ cells using different 3’ UTRs fused to the firefly luciferase coding sequence. We found that Mkrn1 binds strongly to osk 3’ UTR but not significantly above background levels to grk 3’ UTR (S11A Fig). In addition, deletion of the Mkrn1-bound site identified with iCLIP in cells (oskΔMkrn1, deletion of nucleotides 955–978 of osk 3’ UTR) greatly reduced the interaction of Mkrn1 to osk 3’ UTR (Fig 6C and S11B Fig).

As the Mkrn1 binding site in osk 3’ UTR lies just upstream of the A-rich region (AR), we wondered whether the AR would also have an impact on Mkrn1 binding. To test this possibility, we deleted the AR (oskΔAR, deletion of nucleotides 987–1019 of osk 3’ UTR) and examined Mkrn1 binding in S2R+ cells. We observed a decrease of Mkrn1 binding similar to that observed when deleting the Mkrn1 binding sites (Fig 6D and S11C Fig). Thus, we conclude that the AR enhances Mkrn1 binding to osk 3’ UTR. As Mkrn1 forms a stable complex with pAbp, our results further suggest that pAbp binding to the AR stabilizes Mkrn1 and therefore enhances its interaction with osk. Accordingly, reducing pAbp levels by RNAi, but not the level of Imp, another Mkrn1 interactor, dramatically decreased Mkrn1 association with osk mRNA in Drosophila cultured cells (Fig 6E, S11D and S11E Fig). Mutation of the PAM2 domain that enables the interaction with pAbp also resulted in reduced binding to osk 3’ UTR (Fig 6F and S11F Fig). Consistent with these results, mutating both the ZnF1 domain and the PAM2 motif led to almost complete loss of Mkrn1 binding to osk 3’ UTR in S2R+ cells. Collectively, our results indicate that Mkrn1 binds specifically to the 3’ end of osk 3’ UTR via its ZnF1 domain and this association is further stabilized through the interaction with pAbp.

Mkrn1 competes with Bru1 for binding to osk 3’ UTR

Our observation that Mkrn1 binds to the osk BRE-C region prompted us to test whether Mkrn1 and Bru1 may compete for binding to osk 3’ UTR. To this end, we first examined whether we can recapitulate Bru1 binding to osk mRNA in S2R+ cells. As Bru1 is normally not expressed in this cell type, cells were co-transfected with GFP-tagged Bru1 along with the luciferase-osk-3’UTR reporter. RIP experiments confirmed previous findings that Bru1 strongly associates with osk 3’ UTR (S12A Fig, [18]). We next repeated this experiment upon knockdown of Mkrn1 mRNA. Strikingly, while the protein level of Bru1 was not affected (S12B Fig), its binding to osk 3’ UTR was significantly increased in Mkrn1-depleted cells (Fig 7A and S12B–S12D Fig). As pAbp is required to stabilize the interaction of Mkrn1 to osk 3’ UTR, we wondered whether it is necessary for modulating Bru1 binding as well. Indeed, knockdown of pAbp in S2R+ cells resulted in an increased association of Bru1 to osk 3’ UTR (Fig 7B and S12E Fig).

Fig 7. Mkrn1 competes with Bru1 for binding to osk mRNA.

(A) RIP experiments in either control S2R+ cells, or upon knockdown of Mkrn1. Binding of the indicated proteins to the luciferase-osk-3’UTR reporter was monitored by RT-qPCR. The relative fold change in recovered RNA upon Mkrn1 knockdown is illustrated, compared to RIP experiments in LacZ-depleted cells. For every RIP experiment, the enrichment was calculated using GFP. Error bars depict SEM, n ≥ 4. (B) Bru1 binding to luciferase-osk-3’UTR upon pAbp knockdown was analyzed using GFP-RIP with subsequent RT-qPCR. The relative fold change in binding of GFP-Bru1 to luciferase-osk-3’UTR compared to control knockdown is illustrated. The individual enrichments were normalized to IP experiments using GFP alone. Error bars depict SEM, n = 3. (C) RIP experiments in either heterozygous (wild-type) or homozygous Mkrn1W ovaries using α-Bru1 antibody. The relative fold change in recovered endogenous osk mRNA in wild-type compared to Mkrn1W ovaries is depicted. As control RIP, normal IgG was used for every condition. Error bars indicate SEM, n = 4. (D-G) Immunostaining experiments showing Bru1 distribution in (D-E) wild-type and (F-G) Mkrn1W early-stage egg chambers. Note the more prominent accumulation of Bru1 in the oocyte in the Mkrn1 mutant. Scale bars, (D and F) 25 μm; (E and G) 20 μm. (H-M) Stage 10 egg chambers of the indicated genotypes immunostained with α-Osk. Posterior accumulation of Osk is restored to a variable degree (K-M) in Mkrn1W oocytes when heterozygous for bru1. Scale bars, 25 μm. (N) Quantification of posterior Osk localization in oocytes depicted in (H-M). The thresholds for weak, moderate, and strong are arbitrary. The photographs in the H-M panels illustrate what is meant by the different categories. n = 21 for wild-type, n = 52 for Mkrn1W, n = 100 for bru1/+; Mkrn1W. (O) Immunoblot analysis of protein lysates from ovaries depicted in (D-G). Heterozygous mutation of bru1 led to an increase of Osk protein levels in Mkrn1w ovaries.

Next, to assess if these observations made in cultured cells are relevant to Mkrn1 function in vivo, we repeated RIP experiments using ovarian extracts. Bru1 binding was assessed using an antibody directed against endogenous Bru1 and its association with osk mRNA was subsequently analyzed by qPCR. Similar to S2R+ cells, the interaction of Bru1 with osk was significantly increased in Mkrn1W mutant ovaries (Fig 7 and S12F Fig). Thus, we conclude that Mkrn1 restricts Bru1 binding to osk 3’ UTR and this effect is enhanced by the interaction of Mkrn1 with pAbp.

To further address the relationship between Mkrn1 and Bru1, we examined whether the Mkrn1W mutation affects Bru1 accumulation during oogenesis. In wild-type ovaries, Bru1 is expressed in all germline cells and accumulates to a modest degree in the oocyte during early oogenesis (Fig 7D and 7E, [20]). However, in Mkrn1W ovaries, oocyte accumulation of Bru1 during early stages was much more pronounced (Fig 7F and 7G). As osk mRNA accumulates in early oocytes, this result is consistent with Bru1 having an increased binding affinity for osk in the absence of Mkrn1, even though Bru1 can also accumulate in the absence of osk RNA [51].

If Mkrn1 activates osk translation by displacing Bru1, we would predict that lowering bru1 genetic dosage should suppress the Mkrn1 phenotype. To test this hypothesis, we used a strong bru1 allele (bru1QB, [20,52]). We found that removing one copy of bru1 was sufficient to substantially rescue Osk protein level and posterior localization in Mkrn1W female oocytes as analyzed by immunostainings (Fig 7H–7M). Semi-quantitative analysis of Osk-immunostained ovaries confirmed a clear suppression of the Mkrn1W phenotype by one copy of bru1QB (Fig 7N) that was further confirmed by immunoblotting (Fig 7O). We also observed a higher survival rate of embryos produced from Mkrn1W females that were heterozygous for bru1QB, as compared to controls (620/2058, 30.1% vs 40/1222, 3.3%). Taken together, these experiments demonstrate that Mkrn1 activates osk translation, most likely by displacing Bru1 binding at the osk 3’ UTR (Fig 8).

Fig 8. Model depicting activation of osk translation via Mkrn1.

Mkrn1 is recruited to the osk 3’ UTR and stabilized by pAbp. The recruitment of Mkrn1 leads to the displacement of Bru1 promoting translational activation at the posterior pole of the oocyte.


Our data indicates that Mkrn1 is essential for oogenesis, embryonic patterning, and germ cell specification. An essential role for Mkrn1 in oogenesis has also been recently reported [53]. By taking advantage of a new allele that specifically disrupts Mkrn1 binding to RNA, we demonstrate that Mkrn1 exerts its function in embryogenesis and germ cell specification, primarily via regulating osk translation by antagonizing Bru1 binding.

Control of osk translation has been studied in depth, revealing a complex spatio-temporal interplay between repressing and activating factors [19]. Relief of translational repression and activation of osk translation is likely to involve multiple redundant mechanisms. For example, Bru1 can be phosphorylated on several residues, and phosphomimetic mutations in these residues inhibit Cup binding in pulldown assays. However, these do not seem to affect translational repression activity in vivo [24]. Stau, Aub, Orb and pAbp have also been implicated in activating osk translation [14,29,40,54]. However, it is unlikely that Mkrn1 controls osk translation by recruiting Stau, as Stau still colocalizes with osk mRNA in Mkrn1W oocytes (S12G–S12I Fig). Instead, we propose that Mkrn1 exerts its positive activity by competing with Bru1 binding to osk 3’ UTR (Fig 8). This is evidenced by the overlap of their binding sites, the increased association of Bru1 to osk mRNA upon Mkrn1 knockdown and by our observation that reducing bru1 dosage is sufficient to partially alleviate osk translational repression.

Two distinct Bru1 binding regions (AB and C) are present in the osk 3’ UTR and are required for translational repression. However, the C region has an additional function in translational activation. Indeed, it was hypothesized that an activator binds the C region to relieve translational repression [25]. This activator was proposed to either be Bru1 itself, or a different protein that can bind the BRE-C, which is what we observed for Mkrn1 (Fig 6A). Our results suggest that the interaction of pAbp with the nearby AR region, and the consequent stabilization of Mkrn1 binding, contributes to the role of BRE-C in osk translational activation. Other factors may also be involved. For instance, Bicoid Stability Factor (BSF) binds the C region in vitro at the 3’ type II Bru1-binding site [55], at a similar site to where Mkrn1 binds osk. Deletion of this site impacts embryonic patterning, yet depletion of BSF has no effect on Osk protein expression up to stage 10, indicating that initial activation of osk translation is effective even in the absence of BSF [55]. In this case, only late stage oocytes display reduced Osk accumulation. Therefore, it is possible that a concerted action of Mkrn1 and BSF exists at the osk 3’ UTR site to activate translation and sustain it at later stages.

The binding of Mkrn1 to mRNA seems to be extremely specific. We found that the binding to osk is dependent on a downstream A-rich sequence and on interaction with pAbp. A few other targets we identified also display enrichment for downstream AA nucleotides (S13 Fig). and human MKRN1 has recently been shown to associate preferentially to such sequences [49]. Relevant to this, Bru1 binds to grk 3’ UTR in addition to osk [56,57], and several proteins that associate with Mkrn1 also associate with grk mRNA [46,47]. However, we found no evidence that Mkrn1 binds specifically to grk, which lacks poly(A) stretches in the proximity of its Bru1 binding sites, and consistently, we did not observe a regulatory role of Mkrn1 on Grk translation.

In addition to pAbp, it is noteworthy that Mkrn1 associates with other proteins previously implicated in osk localization and translational activation. Its interaction with eIF4G would be consistent with a role in alleviating Cup-mediated repression, as it could recruit eIF4G to the cap-binding complex at the expense of Cup. However, we did not observe an interaction between Mkrn1 and eIF4E (S7C and S7D Fig, S1 and S2 Tables). The association between Mkrn1 and Imp is also intriguing as the osk 3’ UTR contains 13 copies of a five-nucleotide motif that interacts with Imp [28]. This region is essential for osk translation but Osk accumulation is unaffected in Imp mutants, suggesting the involvement of another factor that binds these motifs [26,28,46]. In contrast to pAbp, we did not observe alteration of Mkrn1 binding when Imp was depleted, indicating that Imp is not required to stabilize Mkrn1 on osk mRNA.

The molecular links we uncovered between Mkrn1 and RNA-dependent processes in Drosophila are consistent with recent high-throughput analysis of mammalian MKRN1 interacting proteins [37,49]. RNA binding proteins, including PABPC1, PABPC4, and eIF4G1, were highly enriched among the interactors. Moreover, human MKRN1 was also recently shown to bind to RNA, dependent on the PAM2 motif and the interaction with PABPC1 [49]. In addition, the short isoform of rat MKRN1 was shown to activate translation but the underlying mechanism remained unknown [39]. Since in vertebrates MKRN genes are highly expressed in gonads and early embryos as well, it is possible that similar molecular mechanisms are employed to regulate gene expression at these stages [33]. Consistent with this, MKRN2 was recently found to be essential for male fertility in mice [58]. Thus, our study provides a mechanism that explains the role of Mkrn1 in translation and constitutes a solid framework for future investigations deciphering the roles of vertebrate MKRNs in post-transcriptional control of gene expression during gametogenesis and early development.

Materials and methods

Generation of Mkrn1 mutants using CRISPR/Cas9

The guide RNAs used were cloned into expression vector pDFD3-dU63gRNA (Addgene) according to manufacturer’s instructions. Different guide RNAs were used either alone (gRNA1 starting at nucleotide 64 of Mkrn1 CDS and gRNA2 starting at nucleotide 363 of Mkrn1 CDS) or in combination (gRNA3 starting at 387 nt of Mkrn1 gene and gRNA4 starting at position 2239 nt). vas-Cas9 Drosophila embryos were injected with the purified plasmids containing the gRNA (500 ng/μl in H2O) and allowed to develop to adulthood. Each male was crossed with double balancer females. Genomic PCR from single flies was prepared and tested for CRISPR/Cas9 induced mutations using the T7 endo I (BioLabs) assay or by PCR using primers that bind in proximity to the guide RNA targeting site. A list of gRNAs as well as primers is appended (S3 Table).

Immunostaining and confocal imaging

Ovaries were dissected and fixed in 4% paraformaldehyde in PBS for 20 min at room temperature (RT). After 4–5 washes in PBST (PBS containing 0.3% Triton-X100) ovaries were permeabilized with 1% freshly prepared Triton-X100 in PBS for 1 h. The ovaries were blocked in 2% BSA/PBST overnight. Dispersed egg chambers were then incubated with the primary antibodies diluted in 2% BSA/PBST at RT for 4 h or overnight at 4°C. The washed egg chambers were incubated with conjugated secondary antibodies at 1:500 at RT for 4 h or overnight at 4°C. DAPI (1 ng/ml) was added in the last wash to counter-stain the nuclei for 30 min. After 2–3 washes with PBST the mounting medium containing 1% DABCO was added and the samples were equilibrated for 30 min or overnight. The stained samples were mounted on glass slides and sealed with nail varnish for microscopy imaging. Rabbit polyclonal antibodies against Vas, Osk, Aub, Grk were generated in the Lasko lab; rabbit α-Stau is from the St Johnston lab; rabbit α-Bru1 is from the Ephrussi lab and rabbit α-pAbp is from the Sonenberg lab; mouse monoclonal antibodies against Orb, Sqd, and Lamin were purchased from the Developmental Studies Hybridoma Bank; mouse α-GFP and rabbit α-Flag were purchased from Abcam and Sigma. Alexa Fluor 488 or 555 conjugated secondary antibodies were purchased from Molecular Probes, and pre-absorbed with fixed and blocked wild type ovaries to reduce background. Stained egg chambers were examined using a confocal microscope (Leica). Images were taken under 40 x oil lens by laser scanning and processed with ImageJ.

In situ hybridization of embryos and ovaries and RNA-protein double labeling

cDNAs were used as templates for PCR to generate an amplified gene fragment with promoter sequences on each end. PCR products were purified via agarose gel extraction and used for in vitro transcription to generate digoxigenin-labeled RNA antisense probes with MAXIscript kit (Ambion). The length of each probe was about 1000 nt. In situ hybridization experiments were performed as described [59], using biotinylated α-DIG antibody and streptavidin-HRP followed by tyramide conjugation for development of FISH signal. For RNA-protein double labeling, ovaries or embryos were incubated in primary antibody against the protein of interest along with biotinylated α-DIG antibody at 4°C overnight. The tissue was washed, then detection reagent (fluorochrome-conjugated secondary antibody) along with streptavidin-HRP was added and incubated at 4°C overnight. Images were taken with confocal microscope (Leica).

Embryo cuticle preparation and staining

Flies were transferred into egg-laying cages with apple juice agar plates and incubated at 25°C in the dark. Embryos were collected when 50–100 eggs had been laid and allowed to age for 24 h at 25°C. Embryos were collected in a sieve, dechorionated with 50% bleach for 2.5 min, washed with water, then transferred into PBST buffer (PBS + 0.1% Tween 20). For cuticle preparations, PBST buffer was removed, then 40–50 μl of Hoyer’s solution was added and embryos were kept at 4°C overnight. Embryos in Hoyer’s solution were mounted on a glass slide, covered with a cover slip and incubated at 60–65°C overnight. Dark-field images were taken with Leica DM6000B microscope.


Staging experiment was performed as described [60] using D. melanogaster w1118 flies.

Generation of transgenic flies

The constructs were made using Gateway technology (Invitrogen). Full-length wild-type Mkrn1 cDNA was cloned into the pENTR entry vector using the pENTR/D-TOPO cloning kit (ThermoFisher). After verifying the sequence by PCR, the insert was subcloned into the expression vectors containing UASp promoter with different tags (pPVW and pPFW with Venus and FLAG tags at N-terminal respectively), and (pPWV and pPWF with Venus and FLAG tags at C-terminal respectively) by LR in vitro recombination. For Mkrn1ΔZnF1 pPFMW vector was used. Constructs were verified by sequencing and then injected into yw embryos. Progeny harboring the transgenes were crossed with double balancer flies to establish a variety of lines, and the insertion sites were mapped to either the second or third chromosome. Mkrn1 expression was then driven by crossing the transgenic lines with a nos>Gal4 line (MTD). Expression of tagged Mkrn1 was verified by western blot analysis and immunostaining using anti-GFP (Abcam) or anti-FLAG (Sigma).

Rescue experiment

Flies carrying Venus- or FLAG-Mkrn1 on the second chromosome were crossed with the nos>Gal4 driver lines in three different Mkrn1 mutant backgrounds (Mkrn1W, Mkrn1S, and Mkrn1N). Progeny were collected and separated into two groups: (1) Venus- or FLAG-Mkrn1/ nos>Gal4; Mkrn1W (S or N)/ Mkrn1W (S or N) and (2) nos>Gal4/CyO; Mkrn1W (S or N)/ Mkrn1W (S or N). To perform hatching tests the same number of flies from each group was fed with yeast butter on apple juice plates for 1 d, embryos were collected and incubated at 25°C for 48 h to allow completion of hatching. Hatched and unhatched embryos were counted for each group. The data from several tests in the same group were pooled and the hatching percentage was calculated.

Cell line

Drosophila S2R+ are embryonic derived cells obtained from Drosophila Genomics Resource Center (DGRC, Flybase ID: FBtc0000150).

Cell culture, RNAi, transfection

Drosophila S2R+ cells were grown in Schneider’s medium (Gibco) supplemented with 10% FBS (Sigma) and 1% Penicillin-Streptomycin (Sigma). For RNAi experiments, PCR templates for the dsRNA were prepared using T7 Megascript Kit (NEB). S2R+ cells were seeded at the density of 106 cells/ml in serum-free medium and 15 μg/ml of dsRNA was added to the cells. After 6 h of cell starvation, serum supplemented medium was added to the cells. dsRNA treatment was repeated after 48 h and cells were collected 24 h after the last treatment. A list of primers used to create dsRNA templates by PCR is appended (S4 Table). Effectene (Qiagen) was used to transfect vector constructs in all overexpression experiments following the manufacturer’s protocol.

Immunoprecipitations (IPs)

For IP experiments in S2R+ cultured cells, protocol was followed as described [60] with minor changes: 2 mg of the protein lysates was incubated for 2 h with 10 μl of either Myc-Trap or GFP-Trap beads (Chromotek). To determine the dependence of interactions on RNA, 50 U of RNaseT1 (ThermoFisher) were added to the respective IP. To ensure the activity of RNase T1, lysates were incubated 10 min at RT prior to the incubation of lysate with antibody.

For IP experiments in ovaries, 150 μl of wet ovaries from 3–5 day old flies expressing Venus-Mkrn1 was homogenized on ice in 2 ml of cold IP buffer (1 X PBS, 0.4% Triton X-100, 1 mM MgCl2, 5% glycerol), containing protease inhibitors and PMSF. The extracts were diluted to 1.5 mg protein/ml. Each extract (0.66 ml) was mixed with 24 μg of anti-pAbp Fab antibody (Smibert lab, [61]), 17 μg of α-eIF4G rabbit antibody, or 15 μl of rabbit anti-α−Tubulin antibody (Abcam). When present, 100 μg RNase A (Qiagen) was added to the samples. Samples were incubated with rotation at 4°C overnight, then mixed with 30 μl of protein A agarose beads (wet volume, Invitrogen) and incubated with rotation at RT for 1.5 h. The beads were washed three times with IP buffer. Bound material on the beads was eluted by boiling for 2 min in 40 μl of SDS loading buffer. 20 μl of the eluted sample, together with input samples, was used for western blot.

RNA- Immunoprecipitation (RIP)

For RIP, S2R+ cells or ovaries were harvested and lysed in RIP buffer (150 mM NaCl, 50 mM Tris-HCl pH 7.5, 0.5% NP-40, 1 mM EDTA) supplemented with proteinase inhibitors (1.5 μg/ml Leupeptin, 1.5 μg/ml Pepstatin, 1.5 μg/ml Aprotinin and 1.5 mM PMSF) and RNase inhibitors (20 U/μl). S2R+ cells were lysed for 20 min at 4°C, subtracted to 2 cycles of sonication on a bioruptor (Diagenode) with 30 sec “ON”/“OFF” at low setting and the remaining cell debris was removed by centrifugation at 21,000 g for 10 min at 4°C. To remove lipids and cell debris, ovary lysates were centrifuged 4 times. Protein concentrations were determined using Bradford reagent (BioRad). 2 mg of protein lysate were incubated for 3 h with 2 μg of α-FLAG M2 antibody (Sigma-Aldrich) pre-coupled to 20 μl of protein G Dynabeads (Thermo Fisher Scientific) head-over-tail at 4°C. For RIP experiments analysing binding of Bru1 in ovaries, either 1 μl of rabbit α-Bru1 (gift from A. Ephrussi) or 2 μg of rabbit IgG (Millipore) were incubated with ovarian lysate over night at 4°C. 20 μl of protein G Dynabeads were added for 2 h after the incubation. For every RIP experiment, beads were washed 4 x for 10 min in RIP buffer at 4°C.

For immunoprecipitation of GFP-tagged Imp and Bru1 15 μl of GFP-Trap (Chromotek) were used. Lysates were prepared similar as above using RIPA buffer (140 mM NaCl, 50 mM Tris pH 7.5, 1 mM EDTA pH 8, 1% Triton X-100, 0.1% SDS, 0.1% sodium deoxycholate) supplemented with proteinase and RNase inhibitors. IP was performed for 2 h at 4°C and subsequently washed 4 x for 10 min with RIPA buffer.

RNA was eluted in TRIzol Reagent (ThermoFisher), 10 min at RT and subjected to RNA isolation and RT-qPCR. To obtain the depicted fold enrichment, individual transcripts were normalized to either 18S or RpL15 (S5 Table). At least three biological replicates were performed for each experiment. If not stated differently statistical analysis was performed using one sample t-test.

To analyze IPs, 30% of beads were eluted in 1x SDS buffer (50 mM Tris pH 6.8, 2% SDS, 10% glycerol, 100 mM DTT, 0.05% Bromphenol Blue) at 95°C for 10 min. Eluted IP proteins were removed from the beads and analyzed by western blot together with input samples.

Western blotting

Western blotting was performed as described [60]. Primary antibodies used were: mouse α-Myc 9E10 antibody (1:2000, Enzo Life Sciences); mouse α-FLAG M2 antibody (1:1000, Sigma-Aldrich); rabbit α-GFP TP401 antibody (1:5000, Acris Antibodies); mouse α-HA F7 (1:1000, Santa-Cruz) rat α-HA (1:750, Roche); mouse α-β-Tubulin (1:5000, Covance), mouse α-α-Tubulin (1:20,000; Sigma), mouse α-GFP (1:500; Molecular probe), mouse α-ubiquitin (1:1000; Santa Cruz) Fab α-pAbp (2.5 μg in 5 ml), α-eIF4G rabbit antibody (1 μg in 5 ml), rabbit α-Osk (1:1000) antibody was a gift from A. Ephrussi.

RNA isolation and measurement of RNA levels

Cells or tissues were harvested in TRIzol Reagent (ThermoFisher) and RNA was isolated according to the manufacturer’s instructions. DNA was removed with DNaseI treatment (NEB) and cDNA was prepared with M-MLV Reverse Transcriptase (Promega). The transcript levels were quantified using Power SYBR Green PCR Master Mix (ThermoFisher) using the indicated primer (S5 Table).


To identify binding partners of Mkrn1, either Myc-GFP as control or Myc-Mkrn1 were ectopically expressed in S2R+ cells. Upon lysis, Myc-GFP or Myc-Mkrn1 were immunoprecipitated as described above (see IP methods) with small adjustments: The IP buffer was additionally supplemented with 10 mM N-ethylmaleimide, 1 mM sodium orthovanadate, 5 mM β-glycerophosphate and 5 mM sodium fluoride. After IP, samples were eluted in 2x LDS buffer (Life Technologies) supplemented with 1 mM dithiothreitol for 10 min at 70°C and incubated with 5.5 mM 2-chloracetamide for 30 min at room temperature in the dark. All samples were prepared in parallel.

Conventional interactome analysis of the IP samples was performed as described before [62] with the following changes: The enriched proteins were separated by SDS-PAGE with a 4–12% Bis-Tris protein gel (NuPAGE, Thermo Scientific) and stained with Colloidal Blue Staining Kit (Life Technologies). Subsequently, proteins were in-gel digested using trypsin and digested peptides were then extracted from the gel. Concentration, clearance and acidification of peptides, mass spectrometry analysis, and peptide identification were performed as described before [62]. For peptide identification in MaxQuant (version 1.5.28), the DROME database from UniProtKB (release May 2016) was used. For label-free quantification (LFQ) at least 2 LFQ ratio counts (without fast LFQ) were activated.

The data table of LFQ values resulting from MaxQuant was filtered for potential contaminants, reverse binders and protein groups only identified by site. Furthermore, protein groups with less than two peptides and less than one unique peptide were also removed from further analysis. After log-transforming all remaining LFQ values, missing values were imputed by beta distributed random numbers between 0.1% and 1.5% of the lowest measured values. As a final filtering step, only protein groups having measured values for at least two replicates of at least one experimental condition were kept for further analysis. All filter and imputing steps were done with an in-house R script.

Differential protein abundance analysis was performed on log-transformed LFQ values between two conditions at the time using the R package limma (version 3.34.9, [63]). For each such comparison, only protein groups found in at least two replicates of at least one condition were kept and used. To visualize the interactome, the R package ggplot2 [64] was used. All protein groups with an FDR ≤ 0.05 and a log2 fold change of ≥ 2 were considered significantly changed.

The mass spectrometry proteomics data have been deposited to the ProteomeXchange Consortium via the PRIDE partner repository with the dataset identifier PXD011802.

PAM2 motif alignment

Ortholog searches were performed using HaMStR-OneSeq [65]. Human MKRN1 and MKRN2 (UniProt identifiers: Q9UHC7, Q9H000) served as seed proteins and orthologs were searched within data from the Quest for Orthologs Consortium (release 2017_04, [66]). In order to identify functionally equivalent proteins, we calculated a unidirectional Feature Architecture Similarity (FAS) score that compares the domain architecture of the seed protein and the predicted ortholog [67]. Predicted orthologs with FAS < 0.7 were removed. The multiple sequence alignment of PAM2 motifs of Makorin orthologs from selected arthropod and vertebrate species was generated using MAFFT v7.294b L-INS-i [68]. Since the PAM2 motif in all Makorin proteins differs from the described consensus, a PAM2 hidden Markov model was trained on Makorin PAM2 motifs and used for a HMMER scan ( of the orthologs. Orthologs include species name, UniProt identifiers and amino acid (aa) positions of the PAM2 motif within the protein: Drosophila melanogaster, Q9VP20, 81–95 aa; Anopheles gambiae, Q7QF83, 57–71 aa; Tribolium castaneum, A0A139WP96, 159–173 aa; Ixodes scapularis, B7QIJ9, 119–133 aa; human, Q9UHC7, 163–177 aa; mouse, Q9QXP6, 163–177 aa; zebrafish, Q4VBT5, 120–134 aa.

Individual-nucleotide resolution UV CrossLinking and ImmunoPrecipitation (iCLIP) and autoradiography

The iCLIP protocol was performed as in [69] with the following adaptations: S2R+ cells were crosslinked with 150 mJ/cm2 of UV light and subsequently harvested. Cells were lysed in urea cracking buffer (50 mM Tris pH 7.5, 6 M urea, 1% SDS, 25% PBS) and sonicated using 2 cycles with 30 sec “ON”/“OFF” at low setting. Remaining cell debris was removed by centrifugation at 21,000 x g for 10 min at 4°C. Lysate was diluted 1:5 in IP buffer (150 mM NaCl, 50 mM Tris pH 7.5, 0.5% Tween-20, 0.1 mM EDTA) and incubated with 4 μg of anti-FLAG M2 antibody (Sigma-Aldrich) pre-coupled to 100 μl of protein G Dynabeads (ThermoFisher Scientific) for 2 h at 4°C. After IP, the pulled-down RNA-protein complexes were washed 3x with high salt buffer (1 M NaCl, 50 mM Tris pH 7.4, 1 mM EDTA, 1% NP-40, 0.1% SDS, 0.5% Na-DOC) and 3x with PNK buffer (10 mM MgCl2, 20 mM Tris pH 7.6, 0.2% Tween-20). To trim the length of the crosslinked RNA, on-bead digestion using Turbo DNase (Ambion) and RNase I (Ambion) was performed. Subsequently, the beads were washed again 3x with high salt buffer and 3x with PNK buffer.

For high-throughput sequencing of iCLIP experiments, libraries of 6 technical replicates for FLAG-Mkrn1 and 1 replicate for FLAG-GFP (Control) were prepared as described [69]. Barcodes used for the libraries are listed in S6 Table. Multiplexed iCLIP libraries were sequenced as 75-nt single-end reads on an Illumina MiSeq sequencing system.

Sequencing qualities were checked for all reads using FastQC (version 0.11.5) ( Afterwards, reads were filtered based on sequencing qualities (Phred score) of the barcode region. Reads with more than one position with a Phred score < 20 in the experimental barcode (positions 4 to 7 of the reads) or any position with a Phred score < 17 in the random barcode (positions 1 to 3 and 8 to 9) were excluded from subsequent analysis. Remaining reads were de-multiplexed based on the experimental barcode (positions 4 to 7) using Flexbar (version 3.0.0, [70]) without allowing any mismatch.

All following steps of the analysis were performed on the individual samples after de-multiplexing. Remaining adapter sequences were removed from the read ends using Flexbar (version 3.0.0) with a maximal error rate of 0.1 and a minimal overlap of 1 nt between the beginning of the adapter and the end of the read. Following adapter trimming, the first 9 nt of each read containing the experimental and random barcodes were trimmed off and added to the read name in the fastq files in order to keep this information for downstream analysis. Reads shorter than 15 nt were removed from further analysis.

Trimmed and filtered reads were mapped to the Drosophila melanogaster genome (Ensembl genome assembly version BDGP6) and its annotation (Ensembl release 90, [71]) using STAR (version 2.5.2b, [72]). When running STAR, up to two mismatches were allowed, soft-clipping was prohibited at the 5’ ends of reads and only uniquely mapping reads were kept for further analysis. For further analysis, only unspliced reads were kept and analyzed.

Following mapping, duplicate reads were marked using the dedup function of bamUtil (version 1.0.13), which defines duplicates as reads whose 5' ends map to the same position in the genome ( Subsequently, marked duplicates with identical random barcodes were removed since they are considered technical duplicates, while biological duplicates showing unequal random barcodes were kept.

Resulting bam files were sorted and indexed using SAMtools (version 1.3.1, [73]). Afterwards, bedgraph files were created based on bam files, using bamToBed of the BEDTools suite (version 2.25.0; [74]), considering only the position upstream of the 5' mapping position of the read, since this nucleotide is considered as the crosslinked nucleotide. Using bedGraphToBigWig of the UCSC tool suite [74], all bedgraph files were converted into BigWig files [75].

In order to estimate binding site strength and to facilitate comparisons between binding sites (S10D Fig) we corrected for transcript abundance by representing the crosslink events within a binding site as a ‘signal-over-background’ ratio (SOB). The respective background was calculated as the sum of crosslink events outside of binding sites (plus 5 nt to either side) by the merged length of all exons. 3’ UTR lengths were restricted to 10 nt past the last Mkrn1 binding site or 500 nt if no binding site was present. SOB calculations were performed separately for each replicate and then averaged. No SOB value was assigned for ribosomal genes and genes with a background of < 10 crosslink events, resulting in SOB values for 184 binding sites in 46 targets.

The sequence content around the predicted Makorin 1 binding sites was estimated by counting homopolymeric 2-mers (S13 Fig). All 262 binding sites that fall in 3’ UTRs were centered at their midpoint and a symmetric window was extended 100 nucleotides up- and down-stream. For each position the mean occurrence of each 2-mer was counted.

The iCLIP data has been deposited to the NCBI's Gene Expression Omnibus [76] and is accessible through GEO Series accession number GSE123052 (


To overexpress tagged proteins, the respective coding sequences were amplified and cloned into Gateway plasmids using AscI and NotI restriction sites for plasmids pPFMW and pAHW. The coding sequences of Imp, bru1 and pAbp were cloned using KpnI and XbaI into plasmid pAWG. A list of primers used to introduce the coding sequences as well as to introduce mutations in the Mkrn1 coding sequence is appended (S7 Table). To analyze the binding of Mkrn1 to osk, either the 3’ UTR was cloned downstream of Firefly coding sequence or the complete osk gene was cloned in the same vector backbone of pAc5.1B-EGFP (gift from Elisa Izaurralde, Addgene plasmid #21181). For both, restriction sites of KpnI and SalI were used. To ensure the proper usage of the endogenous poly(A) signal the osk 3’ UTR and the osk gene included 220 and 248 nucleotides of the downstream sequence, respectively. The primers used for cloning and to introduce mutations are listed in S8 Table.

Supporting information

S1 Fig. Four Makorin-related genes are expressed in Drosophila melanogaster.

(A) Sequence alignment of human MKRN1 and the four Makorin-related proteins in Drosophila, Mkrn1, CG5334, CG5347, and CG12477. The ZnF1 domain in Mkrn1 is highlighted green, the PAM2 motif is highlighted yellow, the RING domain is highlighted red, and the ZnF2 domain is highlighted light blue. The RING and ZnF2 domains are conserved in all four proteins, whereas the PAM2 motif is only conserved in CG12477 and CG5347, and ZnF1 is conserved in CG5334 and CG5347. (B) Relative mRNA levels of Mkrn1 and the three other genes encoding predicted Makorin proteins at various stages of development, as measured by RT-qPCR. mRNA levels were normalized to Rpl15 mRNA. Error bars depict Stdev, n = 3.


S2 Fig. Mkrn1 colocalizes with pole plasm components.

All images are from wild-type oocytes expressing Venus-Mkrn1 or FLAG-Mkrn1 as indicated. Overexpression was performed using a nos>Gal4 driver. (A, D,) Immunostaining with α-FLAG to monitor FLAG-Mkrn1. (G and J) Immunostaining with α-GFP recognizing Venus-Mkrn1. (B and E) Immunostaining with α-Osk. (H and K). (C, F, I, L,) Merged images from two preceding panels. Scale bars: (A-C, G-I,) 5 μm; (D-F, J-L) 20 μm.


S3 Fig. Effects of osk and vas mutations on Mkrn1 localization.

(A) Posterior accumulation of either Venus-Mkrn1 or FLAG-Mkrn1 is normal in osk54/+ oocytes but is absent in osk54/Df(3R)p-XT103 (osk) oocytes. (B) Posterior accumulation of either Venus-Mkrn1 or FLAG-Mkrn1 is normal in both vas1/+ or vas1/vasPH (vas) oocytes. Scale bars, 50 μm.


S4 Fig. Mkrn1 genetically interacts with osk and vas.

Pole cell counts from embryos produced by females with the indicated genotypes. Embryos from trans-heterozygotes for Mkrn1 and osk or vas mutations have fewer pole cells than those from single heterozygote controls. Error bars illustrate Stdev, n = 60.


S5 Fig. Transgenic expression of tagged Mkrn1 rescues all Mkrn1 mutant phenotypes.

(A-C) Bright-field micrographs of entire ovaries from (A) Mkrn1N; (B) nos>FLAG-Mkrn1; Mkrn1N and (C) wild-type females, showing overall rescue of oogenesis. Scale bars, 500 μm. (D-F) α-Osk immunostaining on (D) Mkrn1W, (E) Mkrn1S, (F) Mkrn1N egg chambers as negative controls. (G-J) Transgenic expression of tagged Mkrn1 restores posterior localization of Osk protein in Mkrn1W oocytes. (G, H) nos>Venus-Mkrn1; Mkrn1W; (I and J) nos>FLAG-Mkrn1; Mkrn1W. (H and J) Immunostaining with α -Osk; (G) Immunostaining with α-GFP to visualize Venus-Mkrn1; (I) Immunostaining with α-FLAG recognizing FLAG-Mkrn1. (K-N) Transgenic expression of tagged Mkrn1 restores expression and posterior localization of Osk protein in Mkrn1S oocytes. (K and L) nos>Venus-Mkrn1; Mkrn1S; (M and N) nos>FLAG-Mkrn1; Mkrn1S. (L and N) Immunostaining using α-Osk; (K) Immunostaining with α-GFP recognizing Venus-Mkrn1; (M) Immunostaining using α-FLAG to visualize FLAG-Mkrn1. (O and P) Transgenic expression of tagged Mkrn1 restores expression and posterior localization of Osk protein in Mkrn1N oocytes. (Q-T) Immunostaining experiments revealing localization of various proteins in nos>Venus-Mkrn1; Mkrn1N oocytes. (Q) α -Stau; (R) α -Vas; (S) α -Aub; (T) α -Grk. (D-T) Scale bars, 50 μm.


S6 Fig. Mkrn1 mutations affect accumulation of mRNAs involved in axis patterning in embryos.

(A and B) Antero-dorsal accumulation of grk mRNA is similar to wild-type in stage 10 Mkrn1W oocytes. Scale bars, 50 μm. (C) grk mRNA remains associated with the oocyte nucleus and is mislocalized to the posterior in stage 10 Mkrn1S oocytes. Scale bars, 50 μm. In situ hybridization experiments showing posterior accumulation of (D) osk, (E) nos, and (F) pgc mRNAs in wild-type embryos. Scale bars, 100 μm. (G-I) Posterior accumulation of these mRNAs is lost in Mkrn1W embryos. Scale bars, 100 μm.


S7 Fig. Interactome of Mkrn1 in S2R+ cells.

(A) Schematic diagram of Mkrn1 constructs with functional domains highlighted. Differenet mutations were introduced into Mkrn1 protein: Mkrn1RING carries a point mutation that changes histidine 239 to glutamic acid (H239E) while Mkrn1ΔZnF1 contains a deletion of amino acids 26 to 33. To disrupt the ZnF2 domain (Mkrn1ZnF2) three point mutations that mutate cysteines to alanines at positions 302, 312 and 318 (C302A, C312A and C318A) were introduced. (B) Immunoblot showing the relative expression levels of various forms of FLAG-Mkrn1 in S2R+ cells. (C, D) Volcano plots showing the interactome of (C) Myc-Mkrn1 and (D) Myc-Mkrn1RING in S2R+ cells identified using LC-MS/MS and label-free quantification. For both experiments, 3 technical replicates of Myc-GFP (ctrl) and Myc-Mkrn1 IP were performed and compared with each other. The enrichment of proteins compared to the control was plotted in a volcano plot using a combined cutoff of log2 fold change ≥ 2 and an FDR ≤ 0.05. Several proteins of interest are labelled. The entire list of enriched proteins can be found in S1 and S2 Tables.


S8 Fig. Validation of Mkrn1 interactome.

Pulldown experiments to validate binding of tagged Mkrn1RING with (A) GFP-pAbp, (B) GFP-Imp, (C) Myc-eIF4G (D) Myc-Sqd and (E) Myc-Me31B. GFP and Myc IPs were performed in the absence or presence of RNase T1 and enrichment of the proteins was analyzed by immunoblotting. As controls, either GFP alone or Myc-GFP were used. All co-IP experiments were performed in S2R+ cells. (F) Western blot depicting co-IP experiments between Venus-Mkrn1 and eIF4G in ovaries. α-tubulin (αtub, lanes 1, 2) and ovaries lacking the Venus-Mkrn1 transgene (lane 4) were used as negative controls.


S9 Fig. Analysis of the PAM2 motif.

Rescue experiments of either Mkrn1 or Mkrn1PAM2 in Mkrn1N ovaries. FLAG-tagged Mkrn1 transgenes were overexpressed in ovaries using a nos>Gal4 driver line. Ovaries were stained with α-1B1 (red) and α-Osk (green). Nuclei were stained using DAPI (blue). Although overexpression of wild-type Mkrn1 could restore Osk protein at the posterior, Mkrn1PAM2 could not. Scale bar, 50 μm.


S10 Fig. Analysis of the RNA binding ability of Mkrn1.

(A) The RNA binding activity of Mkrn1 is mediated by its ZnF1 domain. Autoradiographs showing association of various forms of Mkrn1 to RNA. FLAG-tagged GFP was used as a negative control. Crosslinked RNA-protein complexes were immunoprecipitated with α-FLAG and treated with different dilutions of RNase I (left: 1/50, right: 1/5000). RNA was subsequently radiolabelled and the RNA-protein complexes were separated by SDS-PAGE. Bound RNA of different sizes is detected by a smear extending upward from the sharp bands that correspond to the sizes of the FLAG-Mkrn1 proteins (arrow). (B) Representative immunoblot of RIP experiment shown in Fig 6A. Either Mkrn1 or Mkrn1ΔZnF1 were overexpressed in Mkrn1N ovaries using a nos>Gal4 driver. The proteins were immunoprecipitated using α-FLAG antibody. Note that Mkrn1ΔZnF1 protein runs higher because of the presence of an additional Myc tag. (C) Validation of iCLIP experiments. Immunoprecipitation of FLAG-Mkrn1 was performed in different conditions. S2R+ cells were transfected and UV-crosslinked prior to IP experiments. Left: autoradiograph showing protein-RNA complexes. Right: Signals of lanes 2, 4 and 5 in autoradiograph were cut and RNAwas subsequently isolated. RNA length was analyzed on a TBE-urea gel. (D) iCLIP datasets with Mkrn1-FLAG in S2R+ cells. The x axis displays maximum binding strength per gene (SOB) and the y axis shows the gene identity. The genes are sorted by SOB with osk mRNA appearing at the third place. Note that ribosomal genes have been excluded for clarity.


S11 Fig. Mkrn1 binding to osk 3’ UTR is dependent on pAbp.

(A) Mkrn1, but not Mkrn1ΔZnF1 binds to the osk 3’ UTR in S2R+ cells. FLAG-RIP of GFP, Mkrn1 and Mkrn1ΔZnF1 was performed co-expressing either luciferase-grk-3’UTR or luciferase-osk-3’UTR reporter. Top: qPCR analysis of the RIP experiments. Fold enrichment is illustrated relative to GFP RIP. Error bars depict SEM, n = 3. Bottom: Immunoblots of a representative RIP experiment. (B-F) Western blot analysis of a representative FLAG-RIP experiment in S2R+ cells summarized in Fig 6C–6F. (B) Either FLAG-tagged GFP or Mkrn1RING was overexpressed. RIP experiments were performed in the presence of a luciferase-osk-3’UTR reporter containing osk 3’ UTR wild-type sequence or deletion of the Mkrn1 binding site (oskΔMkrn1) (C) FLAG-RIP of GFP or Mkrn1RING were performed either using the luciferase-osk-3’UTR reporter. Binding was compared between wild-type osk 3’ UTR and a mutation in the AR region (oskΔAR). (D and E) RIP experiments against FLAG-Mkrn1RING were performed in control (LacZ) condition and compared to (D) Imp or (E) pAbp mRNA knockdown. Right: RT-qPCR analysis of the knockdown efficiency. Imp and pAbp mRNA levels were normalized to Rpl15 mRNA. (F) FLAG-RIP experiments in S2R+ cells using different Mkrn1 mutants. Representative immunoblot is depicted.


S12 Fig. Binding of Bru1 to osk 3’UTR is antagonized by Mkrn1.

(A) RIP experiments of GFP alone or GFP-Bru1 in S2R+ cells. Left: qPCR analysis of RIP experiments analyzing the enrichment of the luciferase-osk-3’UTR transcript. Error bars depict SEM n = 3. Right: Immunoblot of one representative IP using α-GFP. (B-F) Immunoblots of representative RIP experiments summarized in Fig 7A–7C. Right: RT-qPCR validation of the respective knockdown. mRNA levels were normalized to Rpl15 mRNA. (B) RIP experiment of either GFP alone or GFP-Bru1 were performed in control (LacZ) or Mkrn1 mRNA knockdown condition. (C) GFP-RIP experiments were performed in control (LacZ) or Mkrn1 mRNA knockdown condition for either GFP or GFP-Imp. (D) RIP experiment performed against FLAG-tagged pAbp or Sqd in LacZ or Mkrn1 mRNA depleted cells. As control, RIP was performed with FLAG-tagged GFP. (E) GFP-RIP of either GFP alone or GFP-Bru1 in control (LacZ) or pAbp KD. (F) Representative immunoblot of a RIP experiment using heterozygous (wild-type) or homozygous Mkrn1W ovary lysate against endogenous Bru1. As control RIP, normal rabbit IgG was used. (G-I) The three panels show the same Mkrn1W stage 10 egg chamber stained for (G) Stau, (H) osk mRNA and (I) a merged image. There is accumulation of Stau near the pole plasm and co-localization with osk mRNA. Scale bar, 20 μm.


S13 Fig. Makorin1 binding sites display a slight enrichment of “A” nucleotides.

Homopolymeric dimers were counted in 200 a nucleotide wide window centered at 262 binding sites midpoints in 3’ UTRs.


S1 Table. List of identified interaction partners of Myc-Mkrn1 compared to Myc-GFP using mass spectrometry and limma analysis.

All proteins with an FDR ≤ 0.05 05 and log2 fold change ≥ 2 are depicted. (see supplementary file 1)


S2 Table. List of identified interaction partners of Myc-Mkrn1RING compared to Myc-GFP using mass spectrometry and limma analysis.

All proteins with an FDR ≤ 0.05 and log2 fold change ≥ 2 are depicted. (see supplementary file 1).


S3 Table. List of gRNAs used in this study and primers used to validate mutations of the Mkrn1 gene by CRISPR/ Cas9.


S4 Table. List of primers used to create PCR templates of dsRNAs.


S5 Table. List of primers used to in qPCR experiments.


S6 Table. List of barcodes used to prepare iCLIP libraries from material of S2R+ cells.


S7 Table. List of primers used to clone CDSs of proteins as well as primers that were used to introduce mutations in the respective CDS.


S8 Table. List of primers used to clone osk and grk reporter genes and introduce the mutations analyzed.



We would like to thank the Bloomington Drosophila Stock Center for fly reagents, and Anne Ephrussi, Craig Smibert, Daniel St Johnston, and Nahum Sonenberg for antibodies. We also thank Violeta Morin and Beili Hu for fly embryo injections, the IMB Proteomics Core Facility for help with the initial analysis of the mass spectrometry data and the IMB Core Facility Genomics for their helpful support and use of its Illumina MiSeq machine. We also would like to thank the IMB Core Facility Microscopy for support and use of the TCS SP5 inverted microscope P.L. is grateful for sabbatical leave support from the Excellence Initiative of Radboudumc.


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