Introduction

Arabinogalactan proteins (AGPs) belong to the supefamily of hydroxyproline-rich glycoproteins (HRGPs), and most of them are predicted to be tethered to the plasma membrane by a glycosylphosphatidylinositol (GPI) anchor [1,2,3].

These characteristics always made them predictable candidates to be involved in signalling mechanisms, in several plant developmental processes [4]. Showalter et al. [5] identified 85 AGPs in Arabidopsis, divided into five classes: classical AGPs, lysine-rich AGPs, AG peptides, fasciclin-like AGPs (FLAs), and other chimeric AGPs [6, 7]. These glycoproteins, ubiquitous in the plant kingdom, have crucial roles in multiple biological processes, including cell division, cellular communication, programmed cell death, embryogenesis, secondary wall deposition, organ abscission, plant–microbe interactions, and reproductive processes [4, 8,9,10,11,12,13].

AGPs have been subject to innumerous studies in the recent years, which have tried to tackle its functions in plants. Even though, their specific mode of action and the functions of many specific AGPs remains largely unknown.

Due to the complexity of their AG sugar chains and the heterogeneity of their core proteins these molecules are difficult to study. Besides, in large families, redundancy is a problem when one intends to obtain a phenotype and understand the function of a protein [14]. Therefore, the AGPs functional redundancy due to the similarity between its aminoacidic sequences, further interferes with the study of their functions [15,16,17,18]. Despite this, the work being developed with tools such as the anti-AG chain-based immunomicroscopy, β-Yariv reagents, enzymes that target specific parts of AG chains, chemical synthesis of specific structures of AG chains and bioinformatics, is slowly clarifying the nature of AGPs [19]. Moreover, with the development of powerful molecular biology tools, it is possible a genetic approach that offers a great alternative to identify a specific AGP function [20]. The use of several approaches to control gene expression, since the first classical genetic studies until the most recent molecular techniques, has revealed to be essential to determine the functions of different genes correlating them with phenotypes and integrating them in several biological pathways.[21]. In Arabidopsis thaliana, reverse genetic techniques to isolate mutants corresponding to known sequences, such as antisense suppression, co-suppression by overexpression of the target gene, targeted gene disruption, or the PCR approach of screening for T-DNA insertion libraries, have been developed, but are often insufficient and have many unexpected difficulties [22]. These limitations can be partially overcome by new genetic approaches. One classical strategy that has been established for plant functional genetics research, including functional studies for AGPs, is the loss-of-function by RNA interference (RNAi), a great transient gene-expression repression approach discovered over a decade ago [23]. Recently, a new genome engineering technique, using type II clustered regularly interspaced short palindromic repeat (CRISPR) and CRISPR-associated protein 9 (Cas9) from Streptococcus pyogenes, is becoming a powerful tool for functional genomics research in plants [24]. In this review, we describe the best CRISPR/Cas9 and RNAi approaches to obtain AGP mutants, with the intention of getting to know more about the biological function of AGPs.

RNA interference (RNAi)

Possibly, one of the most important advances from the past decades has been the discovery that RNA molecules can regulate the expression of genes [25]. In 1998, the group of Fire and Mello [23] announced their discovery of RNAi—the silencing of gene expression by double stranded RNA molecules—in nematode worms. From this discovery emerged the notion that a number of previously characterized, homology-dependent gene-silencing mechanisms might share a common biological origin. Between the 80's and 90's, plant biologists working with petunias were surprised to find that introducing numerous copies of a gene encoding deep purple flowers led to white or patchy flowers plants, instead of an expected even darker purple color [26, 27]. Somehow, the introduced transgenes had silenced both their own ‘purple-flower’ genes. In parallel, several research groups found that plants responded to viruses RNA by targeting viral RNAs for destruction [28,29,30,31]. Most of the techniques used to induce gene silencing have been shown to share many mechanistic similarities, such as RNAi, co-suppression and virus-induced gene silencing (VIGS). Even the biological pathways which are the core of dsRNA-induced gene silencing are present in most eukaryotic organisms [32].

RNAi is based in the natural pathways of RNA silencing. The first pathway, siRNA silencing, may be important in virus-infected plant cells, where the dsRNA could be a replication intermediate or a secondary-structure feature of single-stranded viral RNA. In plant DNA viruses, the dsRNA may be formed by annealing of overlapping transcripts. The second pathway is the silencing of endogenous messenger RNAs by miRNAs, these are originated from single-stranded transcripts. The miRNAs bind to specific mRNAs by base pairing, and in this way, negatively regulate a specific gene expression, either by RNA cleavage or by disturbing its translation process [33]. Thus, these two classes of silencing RNAs (sRNAs), short interfering RNAs (siRNAs) and microRNAs (miRNAs), affect gene expression in animals and plants, presenting differences between them. The siRNAs are a class of double-stranded RNAs of 21–22 nucleotides in length, generated from dsRNAs. siRNAs silence genes by promoting the cleavage of mRNAs with exactly complement sequences. miRNAs are a class of 19–25-nucleotide, single-stranded RNAs that are encoded in the genomes of multicellular organisms, these are evolutionarily conserved and developmentally regulated. They silence genes interfering with protein translation [25, 34]. sRNAs interfere with normal gene function on several levels, including promoter activity, mRNA stability, and translational efficiency. These small RNAs derive from double-stranded RNA precursor molecules that are cleaved by a specialized class of RNases, the Dicer family which has RNase III domains, into short 21–26 nucleotide small RNAs [33,34,35]. In animals, dicers are named DCRs, and in plants Dicer-like (DCL) proteins.

Chuang and Meyerowitz [22] have shown that it is possible to induce sequence-specific inhibition of gene function in an efficient way by dsRNA-mediated genetic interference in Arabidopsis thaliana. siRNAs and miRNAs are produced in the genome of A. thaliana, by the cleavage of dsRNAs by the Dicer-like gene family, which has only four members: Dicer-like (DCL) 1, 2, 3 and 4. Plant sRNAs precursors are processed in the nucleus by DCL1, releasing the cleaved sRNA duplexes, but usually one of the two constituent sRNAs are preferably associated with ARGONAUTE (AGO), in Arabidopsis AGO1. This strand has been termed the siRNA guide strand, and in the case of miRNAs, corresponds to the mature miRNA. Plant miRNAs pair almost perfectly to their target RNA using preferentially transcript cleavage and subsequent degradation, instead of translation suppression as the silencing mechanism [36].

Silencing RNAs serve as specific components for protein machines known as RNA-induced silencing complexes (RISCs), which contain as catalytic subunits, ARGONAUTE proteins, the mediators of gene silencing, since they cleave target mRNAs, followed often by degradation of the cleaved RNA [33, 37, 38] (Fig. 1).

Fig. 1
figure 1

Schematic representation of the RNAi mechanism. The double-strand RNA (dsRNA) may occur in the cell as exogenous RNAs introduced by viruses or created in laboratory, or as endogenous RNAs transcribed from nuclear genes. These dsRNAs are recognized and processed into small interfering RNAs by Dicer in siRNA or miRNA, respectively. These sRNAs associate with RNA-induced silencing complexes (RISC), which contain a catalytic protein, ARGONAUTE (AGO). If, the pairing with mRNA target sequence and siRNA is 100%, the AGO cleaves target mRNA and promotes its degradation. In the other hand, if the pairing is not perfect (< 100%) this cleavage does not occur and the mRNA/RISC complexes are associated with P bodies with consequent inhibition of translation. The two pathways culminate in the reduction of gene expression

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One of the most developed and effective ways to generate siRNAs in plants is by using long hairpin precursors; this approach is known as inverted repeat, post-transcriptional gene silencing (PTGS) or hairpin RNAi (hpRNAi) [39]. In this case, sense and antisense RNAs are so close that dsRNA is easily formed. The use of hpRNAi is extensively used for many plant species, since many generic plasmids for transgene generation have been made available by the scientific community [34]. On the other hand, plants miRNAs have musch less off targets than animal miRNAs [35, 40], which is a positive feature for most of the silencing studies aiming to silence a specific gene rather than a set of genes. When the artificial miRNAs (amiRNAs) are produced and inserted into the cells, the endogenous miRNAs precursors form sRNAs that consequently lead to gene silencing [35, 41,42,43,44]. miRNA precursors preferentially produce one sRNA duplex, the miRNA–miRNA* duplex. When both sequences are modified without changing structural features, this often leads to high-level accumulation of a miRNA of a desired sequence. amiRNAs are effective when expressed from either constitutive, such as the 35S promotor, or tissue-specific promoters and plant amiRNAs have similarly high specificity as endogenous miRNAs. amiRNAs were used in Arabidopsis [43], where they were shown to effectively interfere with reporter gene expression. The online platform MicroRNA Designer (WMD3) [34, 35] uses sequences of target genes as an input to design artificial microRNAs (amiRNAs), which can be genetically engineered and function to specifically silence genes of interest. After the platform performs a search for candidate 21-mers sequences that are similar to natural miRNAs in the whole length of reverse complements of target transcripts, it is just necessary to select the favorite candidates [34, 35]. Some of the advantages of using amiRNA directed gene silencing are greater specificity and less off-target effects compared to traditional inverted-repeats gene silencing vectors [45]. After choosing the best amiRNA, the WMD includes the ‘Oligo’ tool [34], which allows automatic generation of oligonucleotide primers that can be used in combination with the MIR319a precursor from A. thaliana. Both miRNA and the partially complementary region, the miRNA*, are replaced by amiRNA and amiRNA*, respectively. As structural features are considered important for guiding correct DCL1-mediated processing, the amiRNA sequence is specified so away that mismatch positions to the amiRNA* are retained [34]. Lastly, the chimeric sequence is then transferred to a vector of choice prepared to receive the created construction and transferred to A. thaliana by the Agrobacterium-mediated transformation.

The AGPs are a large family and several T-DNA mutants exist, but not enough to study each AGP specific function. RNAi techniques have been used to elucidate gene function by creating knockdown mutants for these glycoproteins. To define the AGP18 function, Acosta Garcia and Vielle Calzada [46], used RNAi-induced posttrancriptional silencing, specifically degrading the endogenous AGP18 transcripts. The RNAi technique allowed them to demonstrate that this classical AGP is essential for female gametogenesis in A. thaliana. Another work on specific AGP functions is the study of agp6agp11 and their role in pollen grain development [14]. This work has been accomplished using gene silencing studies that created two Arabidopsis transgenic lines by RNAi technology, silencing both AGP6 and AGP11. The comparison of RNAi mutants (knockdown) and knockout mutants created by T-DNA insertion was essential to confirm these AGP phenotypes. Down-regulation of AGP6 and AGP11 by RNAi and artificial microRNA led to pollen grain abortion, inhibition of pollen tube growth, and reduction of fertility [14, 47].

FLA3 is a fasciclin-like Arabinogalactan protein predicted to be involved in microspore development of Arabidopsis. The involvement of this protein in microspore development and pollen intine formation was revealed by RNAi plants, a useful tool to discover AGP functions [48]. More recently, the function of AGP4/JAGGER was identified by studying not only knock out mutants for this glycoprotein, but also one RNAi line [49]. This line (jagger_RNAi) allowed the reduction of JAGGER expression only in certain tissues of the flower, allowing the author to determine the exact pistil tissue responsible for its function. Therefore, in this case the RNAi line was crucial to determine the AGP4 function.

A specific group of chimeric AGPs, belonging to the early nodulin-like proteins (ENODLs), related to the phytocyanin family, are very similar to classical AGPs: EN11-EN15 and were shown to play important roles in plant reproduction [13]. Hou et al. [50] when studying the function of polarly localized ENs, could not obtain null mutations by T-DNA insertion for all the five ENODLs. So they created higher order mutants by introducing an RNAi silencing construct for EN11/EN12 into the triple mutant en13en14en15 and an en-RNAi mutant that contained the loss of function of EN13 EN14 EN15 and lowered expression of EN11 and EN12, respectively. In this case, RNAi technology was crucial to understand that these proteins played an essential role in male–female communication and fertilization, especially in pollen tube reception.

At this moment, it is clear that RNAi technology is vital to discover AGPs specific functions, and the discovery of RNA silencing completely changed the perspective of reverse genetic studies. RNAi is an efficient alternative method to study and determine the function of an individual AGP, and it is reasonable to consider that in the future, RNAi will keep a certain unique space in these studies.

CRISPR/Cas9

With a higher interest in genome editing in the recent years, a new technology has emerged to fulfil the dream of modifying, precisely and efficiently, the genomic DNA of cellular organisms. This technology, based upon the two component CRISPR-associated protein 9 (CRISPR-Cas9) system, is an adjustable bacterial immune system, which helps the bacteria protecting itself against invading foreign DNA, such as the one from a bacteriophage. This process uses RNA-guided nucleases to cleave foreign genetic elements, and in recent years, it has become a resourceful molecular tool for genome editing in various organisms, including plants [51,52,53,54]. These CRISPR/Cas systems can be classified into types II and III, being the type II CRISPR/Cas system adapted as a genome-engineering tool [55]. CRISPR system comprises a group of genes associated with CRISPR, Cas, non-coding RNAs and a distinct matrix of repetitive elements (direct repeats). These repeats are interspersed by short variable sequences derived from DNA exogenous targets, with homology to them, known as protospacers, and together they constitute the CRISPR RNA (crRNA). Within the DNA target, each spacer is always associated with a small conserved sequence named Protospacer adjacent motif (PAM). These small sequences are targets of the Cas endonucleases, thus allowing the system to distinguish its own DNA from foreign DNA. If the bacteria are invaded, a second time by the same invader, the crRNA encoding the 20nt guide RNA and an auxiliary trans-activation crRNA (tracrRNA) generates a complex with Cas9 (crRNA:tracrRNA:Cas9). This tracrRNA usually helps the process as it facilitates the division of the crRNAs in discrete units. The complex formed looks for the DNA sequence with a PAM motif, complementary to the crRNA and binds to it by Watson–Crick base pairing. Finally, Cas9 separates the DNA target from the double strand and cleaves the two strands in a location close to the PAM motif, thus destroying the invader [56,57,58,59]. In order to use this system in genetic engineering, the crRNA and tracrRNA were fused to create a chimeric single-stranded RNA (sgRNA) that present a designed hairpin to mimic the crRNA–tracrRNA complex [51]. This discovery created a simple two-component system (sgRNA and Cas9), being possible to change the genomic target of Cas9 protein, simply by changing the target sequence present in sgRNA [60].

The Cas9 originates from different bacteria, being the Streptococcus pyogenes more used for its isolation. In this system, a Polymerase II promoter [61] expresses this endonuclease. In contrast, Polymerase III promoters, such as U6 and U3 from Arabidopsis [62], typically express sgRNAs. The sgRNA in 5′end has a 20 nucleotide sequence (protospacer) which acts as a guide to identify a target accompanied by the PAM motif (5′-NGG sequence). At its 3′end it presents a scaffold sequence necessary for the binding of Cas9 (Cas9:sgRNA complex), which cleaves the double-stranded DNA and forms a double-stranded breakdown (DSB) at 3 bp upstream of the PAM motif. These DSBs are repaired by evolutionarily conserved DNA repair pathways such as the non-homologous end joining method (NHEJ) or the homology direct repair (HDR). NHEJ is a repair system that connects the DSB by random insertion or deletion of short stretches of oligonucleotide bases. This can lead to a disruption of the codon-reading frame, resulting in wrong transcripts and ablation of gene expression. In HDR, there is the insertion of a DNA segment in regions homologues to the sequences flanking the two sides of the DSB, which makes the cells delivery system to embody an extra segment [63,64,65]. Therefore, NHEJ can lead to ablation of gene mutations and it can be used to knockout specific genes, and HDR can be used to introduce specific point mutations or introduce DNA segments of varying lengths into a specific gene [65]. The NHEJ method is the most used for genome editing because it is more efficient than HDR [66]. To give a more complete view of this technology, Fig. 2 presents a schematic representation of the CRISPR/Cas9 system.

Fig. 2
figure 2

Schematic representation of the CRISPR/Cas9 technique mechanism of action. The sgRNA (single guide RNA - orange) is formed by a sequence of 20nt that defines the genomic target that will be modified and a scaffold sequence (red). The scaffold sequence allows the formation of a complex with the Cas9 protein; the complex can detect target sequences in DNA that are complementary to the target sequence to be modified. If the target sequence is located directly upstream of a PAM (Protospacer adjacent motif- black) sequence, it is recognized by Cas9 leading to a double strand break (DSB) approximately 3 bp upstream of the PAM sequence. This break is usually repaired by NHEJ (non-homologous end joining) in most situations creating insertions/deletions in the gene leading to the complete loss by knockout. However, the break can be repaired by HDR (homology directed repair) creating a precise gene editing introducing specific point mutations. (Color figure online)

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In order to obtain knockout mutants by the CRISPR technology it is necessary to plan the experiment, which normally consists of four principal stages: (i) sgRNA design for the target sequence. For this stage, it is necessary to design the 20nt guiding sequence, specific only for the target sequence, preceded by the PAM motif. There are, nowadays, diverse bioinformatics tools to design sgRNAs, which are able to inform us about the main characteristics needed to consider choosing the best one, depending on the specific target [67]. The selection of a sgRNA has to consider the 5′-NGG PAM for S.pyrogenes Cas9 (a necessary sequence for Cas9 to bind the target DNA) and the minimization of off-target activity. Besides that, to generate genetic knockouts, sgRNAs commonly target 5′ constitutively expressed exons to reduce the chances that the targeted region is removed from the mRNA due to alternative splicing [68, 69]. Also, if the U6 (most common) RNA polymerase III promoter is used to express the sgRNA, the first base of its transcript should be a guanine (G) nucleotide. So, an extra G is added at the 5′ sgRNA, in a way that the 20nt guiding sequence does not start with G [70]. Occasionally, some sgRNAs may not work, thus there is the need of having at least two sgRNAs for each locus and the need to test their efficiencies in the intended cell type [58]. The second stage (ii) is to choose the best vector. In recent years, several researchers have developed vectors encoding the components of genome editing systems for CRISPR in plants. The choice of the vectors largely depends on the type of the expression system to work with, the restriction sites present to insert sgRNA, the sgRNA promotor (RNA polymerase III promotor) and the type of Cas9 system [71]. Several researchers have constructed different binary vectors that combine Cas9 endonuclease with the sgRNA, having the target gene sequence to induce modifications in several plant genes via Agrobacterium-mediated transformation method [72,73,74,75,76]. Xing and colleagues [77] generated a toolkit to set one or more sgRNA expression cassettes into a CRISPR/Cas9-based binary vector, using a Golden Gate Cloning system to amplify sgRNAs [78], this useful toolkit targets the mutation of multiple plant genes. In 2015, other CRISPR/Cas9 vector was reported to allow efficient assembly of multiple sgRNA expression cassettes into a single binary CRISPR/Cas9 vector, only in one cloning round [79], by the Golden Gate Assembly [80] or Gibson Assembly [81]. In the same year, Lowder and colleagues [61] developed a tool that does not require a PCR and can be used for transcriptional regulation with Cas9 fusion in plants. At the same time, Wang and colleagues [82] generated a vector for multiple sgRNAs cassettes with an egg cell-specific (EC1) promoter, to express Cas9 and obtain non-mosaic T1 CRISPR/Cas9 plants, since the mosaicism for the target gene was a problem. To solve this problem and improve the Floral Dip efficiency, a recent study created a extremely efficient CRISPR/Cas9 vector, pKAMA-ITACHI Red, using a RPS5A promoter to drive Cas9 [83]. The RP5A and EC1 promotors for Cas9 endonuclease are constitutively expressed in the egg cells or early embryo stage. If the expression of Cas9 and its subsequent induction of mutations occur in the initial cells or embryos as these promoters allow, the mutations are transferred to the next generation cells, and then all or most of the plant cells, including the meristematic region, will induce this mutation [83]. The pKAMA-ITACHI Red has one more advantage to isolate Cas9-free plants, because it contains an OLE1–TagRFP (red fluorescent protein) that exhibits red fluorescence in seeds, creating an easier and faster selection method, when compared to a PCR reaction. Cas9 deletion is essential to avoid off-targeted mutations and undesirable mutations of a wild-type allele [83]. The third stage (iii) includes the cloning of the sgRNAs in the vector. As already mentioned above, some binary vectors were generated to allow efficient assembly of multiple sgRNA expression cassettes with the Golden Gate or Gibson Assembly [78, 80, 81]. This method reports to its origins in 1996, when it was shown that multiple inserts could be assembled into a vector backbone using the type IIS restriction enzyme sequential or simultaneous activities together with T4 or T7 DNA ligase activities [84, 85]. Golden Gate or Gibson assembly is a flexible, efficient and easy method to clone multiple fragments into a vector, ideal for CRISPR/Cas9 technology, and just needs a recognition site for type IIS restriction enzyme in the final vector and in multiple fragments (sgRNAs), and a T4 or T7 ligase to assemble the fragments. This method works only in one tube and one-step [80]. The last stage (iv) consists in the delivery and expression of the vector into the plant. The most common method to transform plants with the CRISPR/Cas9 final vector is Agrobacterium-mediated transformation, which introduces the T-DNA directly into the plant genome [86]. Cas9 and sgRNA expression cassettes can be easily cloned into Ti plasmid, transformed into Agrobacterium and further introduced into the plants, with the Arabidopsis Floral Dip method, where the egg cell is the target of the T-DNA [87,88,89]. Besides that, the most recent generated vectors of CRISPR/Cas9 technology in plants have shown very positive results with the Floral Dip method [82, 83]. Therefore, this is an easy, efficient and fast method to obtain the transformed seeds that will give rise to the plants (T1 plants) with the desired edited genome.

Actually, the CRISPR/Cas9 technology is being used to obtain knockout mutants for several plant genes. Its efficiency improvement to isolate knockouts of interest was achieved, being important to study plants genetic redundancy, such as the case of AGPs [83]. However, there are still no mutants created by this technology to study the role of the AGPs large family, but the increasing interest in these proteins, together with the few available T-DNA lines and RNAi lines with visible phenotypes, it will not be long before the first CRISPR mutants are created to understand the functions of these glycoproteins.

CRISPR/Cas9 vs RNAi (advantages and disadvantages)

The most correct and usual approach to define gene function is to reduce or interrupt its normal expression. During the last decades, the RNAi technique, together with insertional mutants, has been intensively implemented to discover the function of many genes. However, the emergence of the CRISPR/Cas9 technology came to face these approaches. Nevertheless, while not able to completely disrupt gene function, the use of knockdowns can offer numerous advantages over knockouts. When intended to reduce gene expression only temporarily and if modification of the genetic code is undesirable, the best approach is RNAi-mediated knockdown, because sRNAs in some generations may be lost. It is also advantageous if complete elimination of gene function is detrimental to the cell but a partial loss is not [21, 90]. When one intends to eliminate all variants of transcripts or families of whole genes, this is possible using a single sgRNA against exons that are conserved among all members of the family [91]. This is a very important point in studies of large gene families. The CRISPR/Cas9 technique allows genome editing which leads to precise and predictable modifications [90].

When AGPs are being studied, these two powerful technologies present some advantages and some disadvantages, as summarized in Fig. 3. The main differences are the off-target activity, the length of the effect and the multiple genome editing. In these three cases, CRISPR/Cas9 is more useful because the off-targets can be eliminated, by designing the best sgRNA and choosing the low off-target score [92] and high on-target score [93]. Furthermore, CRISPR/Cas9 assures transmission of the heritable stable mutation [81, 82]. On the other hand, the RNAi technique may or may not generate offspring with reduced expression levels of the gene under study, because although the construct is transmitted to the next generation, the way that the RNAi mechanism acts is always different and sometimes the sRNA can be lost in the next generations [90]. The RNAi system turns out to be less reliable, and always necessary to check the expression levels of the gene of interest in all generations and in all plants, making it a more laborious and expensive method. However, it depends on the research goal, to choose a transient or permanent mutation [21].

Fig. 3
figure 3

Summary of differences, advantages or disadvantages between RNAi and CRISPR/Cas9 techniques

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To explore the role of gene family members with redundant functions, mutations in multiple genes in normally necessary. Therefore, the multiple genome editing is important, because it creates a mutation in multiple similar genes at the same time [81].

This review intends to show that both of these techniques are important and essential to understand the function of AGPs depending on the objective. RNAi has already proven its importance in discovering the roles of various AGPs, as mentioned in the previous section, and certainly, CRISPR/Cas9 will similarly make it soon. Obtaining mutants for these glycoproteins using these techniques is easy and fast, Fig. 4. The AGPs genetic redundancy allows the complementarity of these two techniques [14, 94]. In addition, it is possible to create a higher order mutant by the two techniques at the same time, in case double or triple knockout are not viable. Since most of the AGPs still do not have their function characterized, the application of these two techniques will be of great importance.

Fig. 4
figure 4

The best approaches to obtaining AGPs knockdown or knockout mutants by RNAi and CRISPR/Cas9 methods, respectively. To obtain RNAi mutants, first it is necessary to design an amiRNA in the WMD3 platform. After the chimeric sequence is designed, it is then transferred to a vector of choice using a Gateway cloning system. Lastly, the construction is transferred into A. thaliana by the Floral Dip method and the seeds transformed are selected. When the plants start to grow the genetic techniques such as PCR and RT-qPCR may be used for confirmation of gene knockdown. For the CRISPR/Cas9 technique, the first step is to design the single guide RNA (sgRNA) with 20 nt (blue) and PAM sequence (red) in one of various online platforms (in this case, are shown two sgRNAs for target gene). The sgRNAs may be cloned into a binary vector which contains a Cas9 promotor, being ready to receive the sgRNAs. Multiple sgRNA expression cassettes can be cloned using a Golden Gate assembly (BsaI - IIS restriction enzyme). After cloning, A. thaliana plants may be transformed by the Floral Dip method and the seeds can be selected by red fluorescence (ex. pKAMA-ITACHI Red [83]). When the plants start to grow the genetic techniques such as PCR and Sequencing may be used for confirmation of gene knockout. (Color figure online)

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Conclusion

In recent years, the AGPs have been strong candidates for the performance of various functions in the most varied processes of plant development, especially in the reproductive process, from the development of gametophytes to pollen-pistil interactions, culminating in fertilization and seed formation. However, the mode of action and signaling cascade of most AGPs is still to be unveiled.

Now is the time to unlock the functions of these glycoproteins by taking advantage of these new technologies, gene silencing and genome editing, such as RNAi and CRISPR/Cas9. In this review, it was clear that the two techniques are vital in studies with AGPs. The CRISPR/Cas9 revolutionized current biology, as it is a robust, simple and efficient technology that has opened a new door to genome editing. Several plant biology research groups already use this technology for distinct purposes, with the main goal of increasing and improving agricultural productivity in the future. The application of CRISPR/Cas9 in the AGPs study, will allow to better understand the roles of these essential plant glycoproteins. The work developed for decades, by RNAi, grants that this technique continues to be essential to unravel the function of several genes, such as AGPs. The combination and comparison of results between these two techniques will be valuable in the future, especially in large families of genes as AGPs, where functional redundancy often is a problem.