Qimeng Li,Ákos Nemecz,Gabriel Aymé,Gabrielle Dejean de la Bâtie,Marie S. Prevost,Stéphanie Pons,Nathalie Barilone,Rayen Baachaoui,Uwe Maskos,Pierre Lafaye,Pierre-Jean Corringer
Generation of nanobodies acting as silent and positive allosteric modulators of the α7 nicotinic acetylcholine receptor
α7-nAChR,Nicotinic acetylcholine receptor,VHH,Nanobody,Allosteric modulator
The α7 nicotinic acetylcholine receptor (nAChR), a potential drug target for treating cognitive disorders, mediates communication between neuronal and non-neuronal cells. Although many competitive antagonists, agonists, and partial-agonists have been found and synthesized, they have not led to effective therapeutic treatments. In this context, small molecules acting as positive allosteric modulators binding outside the orthosteric, acetylcholine, site have attracted considerable interest. Two single-domain antibody fragments, C4 and E3, against the extracellular domain of the human α7-nAChR were generated through alpaca immunization with cells expressing a human α7-nAChR/mouse 5-HT3A chimera, and are herein described. They bind to the α7-nAChR but not to the other major nAChR subtypes, α4β2 and α3β4. E3 acts as a slowly associating positive allosteric modulator, strongly potentiating the acetylcholine-elicited currents, while not precluding the desensitization of the receptor. An E3–E3 bivalent construct shows similar potentiating properties but displays very slow dissociation kinetics conferring quasi-irreversible properties. Whereas, C4 does not alter the receptor function, but fully inhibits the E3-evoked potentiation, showing it is a silent allosteric modulator competing with E3 binding. Both nanobodies do not compete with α-bungarotoxin, localizing at an allosteric extracellular binding site away from the orthosteric site. The functional differences of each nanobody, as well as the alteration of functional properties through nanobody modifications indicate the importance of this extracellular site. The nanobodies will be useful for pharmacological and structural investigations; moreover, they, along with the extracellular site, have a direct potential for clinical applications. Supplementary Information The online version contains supplementary material available at 10.1007/s00018-023-04779-8.
Generation of nanobodies acting as silent and positive allosteric modulators of the α7 nicotinic acetylcholine receptor

The α7 nicotinic acetylcholine receptor (nAChR), a potential drug target for treating cognitive disorders, mediates communication between neuronal and non-neuronal cells. Although many competitive antagonists, agonists, and partial-agonists have been found and synthesized, they have not led to effective therapeutic treatments. In this context, small molecules acting as positive allosteric modulators binding outside the orthosteric, acetylcholine, site have attracted considerable interest. Two single-domain antibody fragments, C4 and E3, against the extracellular domain of the human α7-nAChR were generated through alpaca immunization with cells expressing a human α7-nAChR/mouse 5-HT3A chimera, and are herein described. They bind to the α7-nAChR but not to the other major nAChR subtypes, α4β2 and α3β4. E3 acts as a slowly associating positive allosteric modulator, strongly potentiating the acetylcholine-elicited currents, while not precluding the desensitization of the receptor. An E3–E3 bivalent construct shows similar potentiating properties but displays very slow dissociation kinetics conferring quasi-irreversible properties. Whereas, C4 does not alter the receptor function, but fully inhibits the E3-evoked potentiation, showing it is a silent allosteric modulator competing with E3 binding. Both nanobodies do not compete with α-bungarotoxin, localizing at an allosteric extracellular binding site away from the orthosteric site. The functional differences of each nanobody, as well as the alteration of functional properties through nanobody modifications indicate the importance of this extracellular site. The nanobodies will be useful for pharmacological and structural investigations; moreover, they, along with the extracellular site, have a direct potential for clinical applications.

The online version contains supplementary material available at 10.1007/s00018-023-04779-8.

Nicotinic acetylcholine receptors (nAChRs) belong to the pentameric ligand-gated ion channel family and play a key role in neuronal communication as well as in non-neuronal cells such as immune and epithelial cells. The major nAChRs in the brain and at the periphery are the homomeric α7-nAChR, and the heteromeric α4β2- and α3β4-nAChRs, a fraction of these later incorporating the accessory α5 or β3 subunits [1]. Acetylcholine (ACh)-binding promotes a global reorganization in nAChRs, whereupon their intrinsic channel opens, while the prolonged binding of ACh promotes a second reorganization, where the channel closes in what is termed the desensitized state. Among nAChRs, α7-nAChR displays unique properties, including a low probability of channel opening and rapid desensitization [2]. The α7-nAChR has attracted considerable interest and been pursued as a potential therapeutic target for numerous indications [3]. The α7-nAChR is abundant in brain regions such as the hippocampus and the prefrontal cortex that are important for cognitive functions. Therefore, drugs that activate or potentiate the receptor have been shown to be effective in preclinical models for cognitive disorders [4]. Additionally, several therapeutics were tested through clinical trials in the context of Alzheimer’s and Parkinson’s diseases, as well as schizophrenia [5]. However, as of yet there has not been any approval for clinical use, either due to lack of efficacy or to adverse effects [6]. The α7-nAChR is also an essential component of the cholinergic anti-inflammatory pathway, specifically its activation through excitation of the vagus nerve triggers release of anti-inflammatory cytokines [7]. Of note, the α7-nAChR is not only found as homopentamers in the brain, but also as heteropentamers in complex with the β2 subunit [8], as well as with the dupα7 subunit, which is a truncated subunit, associated with neurological disorders, lacking part of the N-terminal extracellular ligand-binding domain [9]. A lot of effort has been dedicated to developing small molecules specifically targeting the α7-nAChRs. Each nAChR subunit within the pentamer is composed of an extracellular domain (ECD) folded as a β sandwich, a transmembrane domain (TMD) consisting of four α-helices, and an intracellular domain (ICD) consisting of two helices and a variably sized poorly resolved domain connecting the two [10, 11]. The endogenous neurotransmitter’s (ACh) binding sites, also called orthosteric sites, are located at all of the subunit interfaces within the ECD of the homomeric α7-nAChR. Agonists, partial agonists, and antagonists all bind at the orthosteric site and were the first therapeutic focus, whereas negative (NAM) and positive (PAM) allosteric modulators binding outside of this site have also actively been investigated more recently [3]. Indeed, the very rapid desensitization of α7-nAChRs is expected to strongly limit the efficacy of conventional agonists, while allosteric modulators can potentially overcome this issue. In addition, PAMs and NAMs are expected to better maintain the spatio-temporal characteristics of endogenous ACh activation and to target non-conserved sites, increasing the chemical diversity of active compounds. In chronological order, calcium was first identified as a PAM [12, 13] binding in the lower part of the ECD [10, 14]. Ivermectin was then identified as a PAM binding in the TMD [15]. Ivermectin can be classified as a type I PAM, potentiating the ACh-elicited current at the peak of the electrophysiological response but not impairing the downstream desensitization process. Subsequently, a large series of small molecules binding at the TMD were found to strongly modulate the receptor, as exemplified by the type II PAM: PNU-120596, that not only potentiates the ACh-elicited currents but also inhibits desensitization to a large extent [11, 16]. Additionally, the PAM: 4BP-TQS can even activate the receptor by itself, thereby having both agonistic and modulatory properties outside of the orthosteric site (Ago-PAM) [17]. Finally, several modulatory sites for small fragments were identified at different levels of the ECD but have not, as of yet, been exploited for drug-design purpose [18, 19]. In addition to small molecules, an interest has recently grown around single-domain antibody fragments of camelids, generally termed nanobodies, in developing biotechnologies [20]. Nanobodies correspond to the variable domain (VHH) of the heavy chain-only antibodies expressed in these animals. Moreover, they usually bind to surface cavities [21] and motifs that often reorganize during conformational transitions of the receptor, thereby acting as conformation-specific ligands. In addition, nanobodies have a number of advantages over small molecules, notably: they usually have a high affinity, typically in the nanomolar range, as well as a high specificity conferred by the large surface of the nanobody–antigen interaction. As an example: within the pentameric ligand-gated ion channel family, nanobodies acting as PAMs and NAMs were reported on the serotonin type 3 (5-HT3) receptor [22], the GABAA receptor [23], and the bacterial ELIC [24]. The generation and functional characterization of two nanobodies specifically targeting the α7-nAChR is presented herein.

To avoid the time-consuming and expensive production and purification of the α7-nAChR, alpacas were immunized with HEK 293 cells transiently transfected with a cDNA directing the expression of an α7-nAChR/5-HT3A chimera. This chimera, where the ECD of the human α7-nAChR is fused to the TMD of the mouse 5-HT3A receptor (hα7-nAChR/m5-HT3A), is expressed at the surface of the cells at much higher levels than α7-nAChR [25, 26]. In addition, injecting transfected cells ensures that the receptor is correctly folded and inserted in the membrane as compared to a detergent solubilized receptor, thereby increasing the chances of isolating conformation-specific nanobodies. A similar approach has been successful for other membrane proteins such as the metabotropic glutamate receptors [27]. After immunization, the VHH-encoding sequences were amplified from the serum and a phage display library was generated (as described in the “Methods”). In a single round of panning, the library was depleted twice through incubation with non-transfected HEK 293 cells, followed by an incubation with non-transfected Vero cells, after which Vero cells transfected with the hα7-nAChR/m5-HT3A chimera were used to select phages binding to the α7-ECD. Isolated clones from the final two rounds of panning were then screened by an ELISA against transfected Vero cells. Seven unique sequences have been obtained from the combination of the second and third rounds of panning.

The clones were produced with a C-terminal Myc and His tag (named VHH in Fig. 1b) and tested by flow cytometry, using non-fixed live cells expressing the hα7-nAChR/m5-HT3A. They were also tested by immunofluorescence. Among the seven VHHs, C4 and E3 displayed specific labeling both in flow-cytometry and immunofluorescence. Flow cytometry results using the positive control of 0.1 mg/mL (~ 11.7 µM) α-Bungarotoxin (α-Btx) conjugated with Alexa Fluor™ 488 resulted in ~ 30% of the cells bound and, therefore, expressing the hα7-nAChR/m5-HT3A chimera on the cell surface, whereas 0.02 mg/mL (~ 1.27 µM of each) of the C4 and E3 VHHs, detected using an Alexa Fluor™ 488 conjugated anti-C-Myc secondary antibody, bind ~ 9% of the cells (Fig. 2). Because of the use of a secondary antibody, the VHH samples experienced an extra half hour of washing during the secondary antibody binding compared to the positive, α-Btx, control. VHH F5, representative of the other five VHHs, shows no labeling of either transfected or non-transfected cells. Two other variants of C4 and E3 were generated: (1) VHH-CSA, carrying a C-terminal cysteine, allowing direct fluorescent labeling to avoid the use of secondary antibodies, and (2) VHH-Fc, where VHHs are fused at the C-terminus with a human IgG Fc fragment permitting detection through a highly specific secondary anti-human Ig antibody, as well as inclining the formation of dimeric VHH domains due to the dimeric nature of the IgG-Fc, putatively increasing binding avidity (Fig. 1b). The immunofluorescence of both constructs was carried out against non-permeabilized cells expressing the hα7-nAChR (Fig. 3). E3-CSA labeled with Alexa Fluor™ 488, was also tested using CHO cells stably expressing the hα7-nAChR, and showed specific labeling (Fig. 3a). A non-human cell-line, CHO, was chosen for stable hα7-nAChR expression, to avoid cross-reactivity with human proteins in testing of the VHH-CSA construct, whereas a human cell-line, HEK293, was used to test specificity and selectivity of VHH-Fc constructs. The VHH-Fc constructs, combined with an anti-human IgG to label them, displayed a nice decoration of the plasma-membrane for both E3-Fc and C4-Fc on transiently transfected HEK293 cells (Fig. 3b) and, therefore, this construct was used to assess each VHH’s binding specificity. The combination of these results suggests a binding motif in the ECD. The interaction of the C4-Fc and E3-Fc constructs with hα7-, hα3β4-, and hα4β2-nAChRs was tested on permeabilized transiently transfected cells to assess binding specificity. To visually pinpoint transfected cells, through fluorescence, either cytoplasmically fused eGFP (hα4-nAChR) or an internal ribosome entry site (IRES) linked eGFP (hα7- and hα3-nAChR subunits) were used (Fig. 3c). Both C4-Fc and E3-Fc label cells transiently transfected with hα7-nAChR, while no labeling is observed for hα3β4- and hα4β2-nAChR transfected cells, demonstrating a strong selectivity of both constructs. Interestingly, sequence analysis determined that both E3 and C4 diverge from the classical nanobody framework in that C4 contains only a single cysteine and thus no disulfide bridge, whereas E3 contains four cysteines, forming the canonical bridge between framework region (FR) 1 and FR3 domains, but also an unusual bridge flanking both extremities of the complementarity-determining region (CDR) 3 (Fig. 1a).

To elucidate their binding mode, a competition assay with I125 labeled α-Btx, a competitive and highly specific orthosteric antagonist, was performed. HEK293 cells, transfected with the hα7-nAChR/m5-HT3A chimeric construct used in panning experiments, were suspended and incubated with 0.01 mg/mL VHH (~ 633 nM, with a C-terminal Myc and His-tag) for 2 h at 4 °C and compared to 100 µM ACh (incubated for 1 h at 4 °C) as a control (concentrations are indicated as final concentrations, and all results were normalized to a buffer incubated sample). Scintillation reading of filtered samples, after the addition of a saturating, final, concentration of 5 nM of I125-α-Btx was added to this mixture, showed that there is no competition between α-Btx and either VHH (Fig. 4). This indicates that neither VHH binds to the orthosteric-binding site, and therefore, bind to an allosteric site elsewhere within the ECD.

The functional effect of E3 and C4 (with a C-terminal Myc and His-tag) was investigated by two-electrode voltage clamp electrophysiology on Xenopus oocytes expressing the hα7-nAChR (Fig. 5). Perfusion of 1 mM ACh, in this methodology, evokes robust currents characterized by a fast onset of activation, a culmination at a peak, and a slower decay of activation whereupon receptor desensitization through prolonged agonist (ACh) application overcomes newly activating receptors, until the agonist is rinsed, and the receptor returns to its resting state. The effects of the nanobodies were investigated at a concentration of 30 µM ACh, corresponding approximately to an EC10 concentration to ensure maximal sensitivity of the system. E3 does not elicit any current when applied alone (see Fig. 5c right inset for “pre-perfusion” applications of E3 alone before ACh currents). In a first series of experiments, E3 was applied during an application of ACh (“post-perfusion condition”, n = 5, Fig. 5a). At 800 nM, E3 elicits a clear increase of the ACh current, and the rise-time of this potentiation appears relatively slowly in comparison to the rise-time of ACh alone. The potentiation by E3 does not overcome receptor desensitization as seen by a time-dependent decrease during VHH application, indicating that the nanobody favors the activation process but does not preclude the downstream process of desensitization. This potentiating effect is concentration-dependent. To further investigate the kinetics by which E3 modulates the function, several concentration–response recordings were performed where E3 is directly co-applied with ACh (“co-perfusion condition”, n = 5, Fig. 5b), or where it is additionally perfused for periods of 10, 30, 60 (Fig. 5c), and 120 s before the ACh/E3 co-application (“pre-perfusion conditions”, n = 5 each time-point, Fig. 5d). Longer pre-perfusion conditions generated significantly larger potentiation, especially at low nanobody concentrations, where 316 nM E3 obtained near maximal potentiation, indicating that the nanobody associates to the receptor with a slow kinetics in the recording conditions. This slow kinetics is probably the main reason for the moderate potentiation observed in “post-perfusion” conditions. Indeed, in these conditions, E3 will slowly bind and potentiate the receptor, a process during which a significant fraction of the activated receptors will desensitize, generating a net reduction of the peak current. Altogether, the data unambiguously show that E3, with low nanomolar apparent affinity and relatively slow binding kinetics, elicits potentiation of ACh-elicited currents and does not preclude desensitization. In concentration–response curves, PAM binding usually increases the apparent affinity of the agonist [15]. ACh concentration–response curves in the absence or presence of a 1 µM concentration of E3 were, therefore, measured. E3 tends to cause a small decrease in the apparent EC50 of ACh (n = 7, Fig. 5e), but this effect is not statistically significant due to the variability of the responses between individual oocytes. It is noteworthy that the kinetics of the rise-time and decay-time of the responses were also variable as illustrated by the current traces shown in Figs. 5, 6, 7. This precludes a kinetic analysis of the activation and desensitization processes. Further studies would thus be required to investigate quantitatively a possible effect of E3 binding on the kinetics of activation and desensitization.

Conversely, C4 elicited no response on its own nor showed any discernable modification of α7-nAChR function when co-applied with ACh (tested at 316 nM with 15 s perfusion alone or in “post-perfusion” conditions with ACh n = 3 each, data not shown). Interestingly, when using a modified 30s “purely pre-perfusion” procedure (see “Methods”), the ACh-gated current after pre-perfusion of a mixture of E3 (150 nM) with C4 (at either 150 nM or 1.5 µM) is near identical to that in the absence of nanobodies (5 ± 10% and − 9 ± 21%, in the presence of the respective C4 concentrations, of the % potentiation by 150 nM E3 alone), whereas E3 (150 nM) pre-perfused alone on the same oocyte just before the application of these mixtures produced robust potentiation of 30 µM ACh (75 ± 17% and 71 ± 28%, n = 3 and 5 resp., Fig. 6a). These data indicate that C4, which has no discernable functional effect on the α7-nAChR alone, binds to inhibit the potentiating effect of E3. The simplest interpretation is that the C4- and E3-binding sites overlap at least partially, with C4 inhibiting E3 binding in a competitive manner. Whatever the case, the data allow classification of C4 as a silent allosteric modulator (SAM), at these concentrations. To further examine a possible competitive binding mechanism between E3 and C4, a “double purely pre-perfusion” procedure was performed to test whether C4 could displace already bound E3. In this condition, E3 (150 nM) is perfused for 30 s, then a mixture of E3 (150 nM) and C4 (at either 150 nM or 1.5 µM) is perfused for 30 s, followed by activation by 30 µM ACh. It should be noted that the potentiation of E3 (150 nM), pre-perfused alone for 30 s, was less pronounced in these experiments (43 ± 14%, n = 6). 1.5 µM of C4 was found to out-compete 150 nM of pre-bound E3, yielding no potentiation (− 14 ± 18% of E3 potentiation, n = 3), whereas 150 nM C4 only partially blocks the effect of E3 (48 ± 30% of E3 potentiation, n = 3) (Fig. 6b). The data thus suggest that C4 can displace already bound E3 molecules. Whereas, the reduced ability of C4, at 150 nM, to displace already bound E3 is most probably due to the slow binding kinetics of these nanobodies. It is noteworthy that comparison of the sequence of E3 and C4 show significant conservation at CDR1, CDR2 and half of CDR3, further arguing for overlapping binding sites. Most importantly, these data indicate that this allosteric ECD site is capable of various modulatory actions akin to the orthosteric site.

To increase the affinity and avidity of E3 against hα7-nAChR, a bivalent construct was generated, where two E3 nanobodies are separated by a 16-residue flexible linker (Fig. 1). E3–E3 displays potentiating properties similar to that of E3 (n = 11, Fig. 7a, n = 4, Fig. 7b). Strikingly, the potentiating effect of E3–E3 did not vanish upon prolonged wash out of the oocyte (Fig. 7c), achieving 94 ± 12% of the initial maximal potentiating current with repeated applications of 30 µM ACh alone out to ~ 50 min (for n = 4) after the last application of E3–E3. Whereas, the effect of E3 totally vanished upon 3 min of washing (Fig. 5). E3–E3 is at least as efficient as E3 to potentiate the ACh-elicited currents, but evaluation of a concentration dependent curve is rendered moot with the impossibility of washing out the construct. Thus, the avidity conferred by the bifunctional character makes E3–E3 a quasi-irreversible potentiator in the oocyte recording system. Like E3, E3–E3 tends to cause a small decrease in the apparent EC50 of ACh (n = 4, Fig. 7b), but this effect is not statistically significant.

The classical technique to generate specific nanobodies against a given target is to immunize alpacas with purified protein, a procedure that requires large quantities of protein (> 1 mg). Within the pentameric ligand-gated ion channel family, this technique has been successfully applied for members yielding good expression in recombinant systems such as the ELIC [24], the 5-HT3 receptor [22], and the GABAA receptor [23]. This article focuses on the α7-nAChR, a subtype that shows low levels of expression in recombinant systems [10]. To avoid the time-consuming overexpression and purification steps, direct immunization with a cell-line transiently transfected with a hα7-nAChR/m5-HT3A chimera that has good expression levels was performed. Such a procedure is expected to stimulate the production of a wide range of nanobodies recognizing many proteins present at the surface of the cells. Therefore, a carefully designed panning strategy was completed, yielding, after a few rounds, two nanobodies that bind specifically to the α7-nAChR. The procedure has also the advantage of injecting membrane-inserted protein, ensuring native pentameric assembly of the receptor, increasing the chance to isolate antibodies targeting a properly folded ECD in a pentameric conformation. This procedure should be applicable to other pentameric ligand-gated ion channels with weak expression levels and/or low stability after extraction from the plasma membrane. The α7-nAChR is activated by choline with an EC50 around 500 µM in an oocyte, with choline already producing clearly detectable responses at concentrations of 30 µM or less [28]. Since levels of choline in human plasma have been reported to range between 5 and 15 µM [29], it is possible that such a concentration in the alpaca plasma would stabilize a significant fraction of the receptor on the cells which were injected in the active or desensitized conformational states during immunization. This could direct the generation of a PAM, such as E3, that favors the active state and does not preclude desensitization. The generation of a SAM, in C4, is consistent with this assessment as a VHH that equally binds the resting state and active state would be equally possible in such an environment, as an equal conformational affinity would stabilize neither state, and thereby lack a functional modulation. Structural and/or mutational studies of the α7-nAChR in complex with the described nanobodies are required to fully understand their mechanism of action. To date, several nanobodies or even fragments of antibodies have been structurally resolved with pentameric ligand-gated ion channels. These structures help gleam possible binding locations for E3 and C4. From these structures, two regions can be directly excluded from the fact that no competition with α-Btx is observed. The first, an exterior site just below the orthosteric pocket, structurally resolved on GABAA [30, 31] and a nAChR [32] and the second, an exterior binding site directly overlapping and slightly above that of α-Btx, found with the 5-HT3 receptor [22]. A third site on the complementary subunit to the right of and slightly above the orthosteric pocket, visualized on ELIC [24] and GABAA [33], respectively, is likely occluded in the α7-nAChR due to a unique glycosylation site. This site in the prokaryotic ELIC was found to have PAM effects. It may still be possible that the VHH’s accommodate for a sugar moiety in this region. Finally, two apical sites have been observed: the main immunogenic region, bound by an antibody fragment on a nAChR [34], and a single VHH that has multiple interactions with the apex of the ELIC, laying on the top and interacting through the CDRs with multiple subunits in the vestibule [24]. The later was determined to be a NAM and through its binding pose it would be predicted that it would not be conducive to an enhancement of avidity through bivalent binding. Whereas, the former was also found to have a slight increased affinity on agonist binding but no electrophysiological effects at saturating agonist concentrations. Therefore, of the currently resolved binding locations the data would be compatible with two regions, both of which have also hinted to positive modulatory effects. In conclusion, E3 binds outside of and above the orthosteric site, at an apical position. Structural and/or mutational studies are necessary to determine the exact location of VHH binding. Interestingly, the dimerization of E3 allows the formation of a quasi-irreversible PAM. This striking effect is probably related to an increase of the avidity of this bivalent molecule. In retrospect, this feature probably explains why, in immunofluorescence experiments that involves several rinsing steps after VHH binding, the labeling by monovalent E3 was weak, while that of bivalent E3-Fc was robust. Several examples of dimerization of nanobodies directed against viral proteins have been reported to potentiate the neutralizing activities of the parental nanobody [35–38]. This bivalent construct can serve as a unique therapeutic agent, especially for neurodegenerative disorders where α7-nAChR expression is diminished, potentially permanently amplifying nAChR response signals without having a temporal effect (through modification of binding/desensitization properties) on the nAChR response. This possibility should be further studied to see if adverse effects due to prolonged potentiation of α7-nAChR arise, or if the bivalent nature of the VHH yields problems in administration, such as crossing the blood–brain barrier.

The two nanobodies C4 and E3 constitute a novel class of allosteric modulators of the α7-nAChR. They show high specificity among nAChR subtypes, a feature characteristic of antibody–antigen recognition that involve a large area of interaction. These nanobodies are easily expressed in milligram amounts in cell-lines and can be easily engineered as illustrated here by the generation of a quasi-irreversible bivalent potentiator. They will be useful for a wide range of applications, notably the investigation of native receptors in brain tissues in immunofluorescence and immunoprecipitation assays. They will also be precious for the investigation of the receptor and as pharmacological tools to help structural studies. Finally, they constitute an original family of allosteric modulators with far reaching potential medical applications such as cognitive enhancers, or as a potential treatment against α7-nAChR auto-antibodies that are found in some patients diagnosed with schizophrenia [39].

All immunization processes were executed according to the French legislation and in compliance with the European Communities Council Directives (2010/63/UE, French Law 2013-118, February 6, 2013). The Animal Experimentation Ethics Committee of Pasteur Institute (CETEA 89) approved this study (2020-27412). We subcutaneously injected an adult alpaca at days 0, 21, and 28 with approximately 108 hα7-nAChR/m5-HT3A chimera-transfected HEK293 cells mixed with Freund complete adjuvant for the first immunization and with Freund incomplete adjuvant for the following immunizations. Repetitive immunogen administrations were applied to stimulate a strong immune response. A blood sample of about 250 mL of the immunized animal was collected and a Phage-Display library in a pHEN6 phagemid vector of about 2 × 108 different clones was prepared as described before [40], and detailed below.

The plasmids for all nAChR constructs were human (h). The hα7-nAChR/m5-HT3A plasmid was created merging the human α7-nAChR sequence with the mouse 5-HT3A sequence at V202 of the α7-nAChR mature sequence (as described in [26]). pcDNA3.1 + vector was used for all constructs containing an internal ribosome entry site (IRES), which allows for expression of the sequence following the IRES. The expression of this sequence is slightly reduced as compared to the sequence directly behind the promoter sequence and before the IRES. The pMT3 vector was used for the eGFP alone and the hα4-nAChR which contained an ICD linked GFP (hα4GFP); where an eGFP sequence was inserted in the cytoplasmic domain between SCK395/S396PS following the mouse α4-nAChR construct created by Nashmi et al. [41]. The pCMV6-XL5 vector was used for the NACHO construct [42]. Hα7- and hα3-nAChR-IRES-eGFP constructs, used for immunofluorescence experiments, contained the respective nAChR sequence, followed by an IRES element from the encephalomyocarditis virus, and then the coding sequence of eGFP (sequences extracted from pIRES2-EGFP, Clontech). Hβ4StrepTagII-nAChR-IRES-mTurquoise, contained the human β4 sequence with a C-terminal StrepTagII the aforementioned IRES element followed by an mTurquoise GFP. For transduction into the CHO-K1 cell-line hα7-nAChR-IRES-eGFP, along with the chaperone protein constructs: NACHO-IRES-mKate and Ric3-IRES-TdTomato, were cloned into a modified pTRIPΔU3 vector with a CMV promoter, and lentiviral particles created as described in the supplementary methods of Maskos et al. [43]. In the case of the hα7-nAChR plasmid used in two-electrode voltage clamp experiments, the IRES was followed by the coding sequence for NACHO. Synthetic genes of the anti-α7 nanobody derivatives were designed and purchased from EurofinsGenomics (Ebersberg, Germany), digested using SfiI and NotI and ligated into the pHEN6 phagemid [44].

About 250 mL bloodletting samples of the immunized alpaca in EDTA-coated tubes were collected and inverted twice to inhibit coagulation. Histopaque-1077 (Roche) was employed to separate lymphocytes according to the manufacturer’s instructions. Total RNA was extracted, following the RNeasy minikit (Qiagen) protocol, from isolated lymphocytes and its purity verified using the Agilent RNA 6000 Nano Assay system. This total RNA was subsequently reverse-transcripted to generate a diverse cDNA library. This cDNA was then amplified by overlap extension PCR which allows for the isolation of the ~ 400 bp VHH domain. These PCR fragments were also digested using SfiI and NotI and ligated into the pHEN6 phagemid, which was transformed through electroporation into E. coli TG1 cells.

HEK293 and Vero cells were cultured in high glucose Dulbecco’s Modified Eagle Medium supplemented with 110 mg/L sodium pyruvate and 862 mg/L of l-alanyl-glutamine as well as 10% fetal bovine serum (DMEM-FBS) with or without the addition of an antibiotic mixture of penicillin/streptomycin (10 U/mL and 10 μg/mL resp.) at 37 °C with 5% CO2. Expi293F cells were maintained at 99% viability per manufacturer’s recommendations in Expi293™ Expression Medium (ThermoFisher) at 37 °C with 8% CO2 under constant agitation and passed every 3 days. CHO-K1cells were cultured in DMEM/F12 Medium (Gibco) supplemented with 10% FBS and penicillin/streptomycin (10 U/mL and 10 µg/mL) at 37 °C with 5% CO2.

Lentiviral particles were directly added to CHO-K1 cells during their seeding at 1 × 105 cells/well respecting a particle ratio of 5:1 (hα7-nAChR and NACHO-IRES-mKate resp.) which was achieved using 1 µg of p24 for hα7-nAChR particles and 0.2 µg for the chaperone. After 3 days of expression, cells were sorted by FACS (FACS-Aria III; BD Life Sciences) and cells expressing the reporter gene were seeded in 96-well plate to obtain individual clones. Clones expressing a high level of hα7-nAChR at the plasma membrane were selected by α-Btx immunostaining.

To produce nanobody-phages, 100 µL of the E. coli TG1 library was inoculated into 100 mL of 2xYT medium (Tryptone 16 g/L, Yeast Extract 10 g/L, NaCl 5 g/L, pH 7) supplemented with ampicillin (100 µg/mL) and glucose (1%). The culture was grown at 37 °C under shaking at 200 rpm until OD600 (optical density at λ600) reached ~ 0.5–0.6. Recombinant nanobody-displaying phages were rescued with 2 × 1011 PFU of M13KO7 Helper phage (New England Biolabs). Rescued phages were suspended in 1 mL of phosphate buffered saline (PBS, Gibco) supplemented with bovine serum albumin (BSA, Sigma-Aldrich) at a final concentration of 1% (PBS-BSA). In a round of panning, 0.5 mL of produced nanobody-phages was added to 4.5 mL of PBS-BSA solution as a phage panning medium. 1 × T75 confluent HEK cells (~ 107) were washed with PBS and resuspended to individual cells. The suspension was centrifuged at 2000 rpm at 4 °C for 15 min. Cells were resuspended with 5 mL phage panning medium for the first-depletion round, and maintained at 4 °C for 1 h with gentle shaking. The suspension was then centrifuged (same conditions as above) where the supernatant phages were recovered. This depletion step was repeated and then completed once more on Vero cells (5 mL, ~ 27) to eliminate non-specific nanobodies directed against common membrane proteins. Phages were then finally incubated with hα7-nAChR/m5-HT3A chimera-transfected Vero cells, again in 5 mL at 4 °C for 1 h with gentle shaking to select target-specific nanobody-phages. After incubation, suspension was centrifuged (as above) and washed ten times with PBST (PBS with 0.01% Tween 20) (each time for 10 min), followed by two washes with PBS to remove Tween 20. The cells were then lysed with 1 mL of 100 mM triethylamine (Sigma-Aldrich) for 5 min at 4 °C and pH was neutralized with 0.5 mL of 1 M Tris (pH 7.4). Eluted phages (in triethylamine lysate) were amplified by infecting exponentially growing E. coli TG1 at OD600 of ~ 0.5 to propagate phages for the next round of selection.

96 isolated clones from the second and the third rounds of panning were tested for nanobody-phage specific binding to α7-nAChR in a cell-ELISA. H﻿﻿α7-nAChR/m5-HT3A chimera-transfected Vero cells (105 cells/mL) were coated onto 96-well plates pretreated with poly-d-lysine (Sigma-Aldrich), according to manufacturer’s recommendations. A negative control (non-transfected Vero cells) was prepared under the same conditions. Cells were then fixed by addition of 4% (w/v) paraformaldehyde (Sigma-Aldrich) in PBS for 20 min, culture were then rinsed three times with PBS and treated with 3% (w/v) hydrogen peroxide (BioRad) in PBS for 5 min to minimize endogenous peroxidase activity, and finally washed twice in PBS. Plates were then blocked with PBS-BSA for 1 h at 37 °C. Nanobody-phage unique clones were separately grown in 300 µL of 2xYT medium supplemented with ampicillin (100 µg/mL) in a 96-deep-well plate, unique nanobody-phage’s production was induced by co-infection with the Helper Phage and culture was left overnight at 30 °C under shaking. The supernatant was retrieved by centrifugation (2500 rpm for 20 min at 4 °C) and the produced unique phages were tested in parallel for their specific binding on hα7-nAChR/m5-HT3A chimera-transfected Vero cells and on non-transfected ones as a control. The supernatant was diluted to 1/5 in PBS-BSA, and 100 µL of the dilutions were applied to fixed cells in corresponding wells, after incubation for 1 h at 37 °C, plates were washed 3 times with PBST, and bound nanobody-phages were labelled by the addition of anti-M13 antibody [HRP] (SinoBiologicals). After five washes with PBST, HRP substrate reagent (OrthoPhenyleneDiamine, Sigma-Aldrich), prepared according to manufacturer’s recommendation, was added. The reaction was stopped by the addition of 50 µL per well of 3 M HCl, and the absorbance of the samples was measured at 492λ in a spectrophotometer-microplate reader (Sunrise, Tecan). Samples with an absorbance ratio (positive/control) exceeding 3 were considered as α7-positive clones. These were then sequenced, and the sequences were analyzed.

The pHEN6 vector used for library construction allows for direct bacterial periplasmic expression and purification of selected nanobodies with a C-Myc tag and a 6xHis tag at their C-terminal (VHH in Fig. 1). The gene coding for a monovalent nanobody with a 6xHis tag in the N-terminal and an extra C-terminal Cys-Ser-Ala motif (CSA) enables site-specific labeling of the nanobody via maleimide (VHH-CSA in Fig. 1) [45]. The gene for the bivalent derivative is composed of two molecules of the same nanobody linked together by a flexible (GGGGS)3 linker, with a C-Myc tag and a 6xHis tag at the C-terminal (VHH-VHH in Fig. 1). The VHH-Fc gene had the C-terminal linker listed in Fig. 1.

Genes were cloned into the pHEN6 vector for periplasmic expression in the E. coli strain: BL21 (DE3). Proteins were produced as periplasmic components in 1 L of the NZY Auto-Induction TB medium (NZytech) according to the manufacturer’s recommendations and were purified by immobilized metal affinity chromatography on a HiTrap TALON® crude 1 mL column (Cytiva). After extensive washings with PBS containing 150 mM NaCl (PBS/NaCl), proteins were eluted in PBS/NaCl buffer supplemented with 500 mM imidazole. Bacterial production yields varied from 1 to 12 mg/L of culture. Alternatively, the nanobodies’ engineered genes were cloned into a pFUSE-derived vector (InvivoGen); this vector harbors a human IgG1-Fc domain. Consequently, the nanobody was expressed as a Fc-fusion bivalent antibody. The vector was used to transfect Expi293F mammalian cells (ThermoFisher), and protein expression was carried out according to manufacturer’s recommendations. Protein was then purified from the expression medium by affinity chromatography on a 1 mL protein G column (Cytiva). After sample application, the column was washed with 20 column volumes of PBS and the protein was subsequently eluted with 10 column volumes of PBS supplemented with 0.1 M Glycine (pH = 2.3). Production yields were above 25 mg/L of culture.

Site-specific labeling of the engineered nanobody was done using maleimide Alexa Fluor™ 647 C2 or Alexa Fluor™ 488 (ThermoFisher). Briefly, the anti-α7 nanobody with additional CSA motif was surrendered to a mild reduction by adding ten molar excesses of tris(2-carboxyethyl) phosphine (TCEP) (Sigma-Aldrich) at 25 °C for 30 min. Reduced protein was then incubated for 2 h with 20 molar excess of the respective maleimide Alexa Fluor™ dissolved in DMSO. Labeled protein was filter-dialyzed against 10 L of PBS using a 3K-CutOff Slide-A-Lyzer™ Dialysis Cassette (ThermoFisher). Labeling quality was assessed by Mass Spectrometry as previously described [46].

1–5 × 106 hα7-nAChR/m5-HT3A transfected cells, with > 90% viability, were centrifuged at 1000g for 10 min at 4 °C, and resuspended to obtain a final concentration of 100–300 cells/µL in ice cold PBS solution supplemented with 10% FBS and 1% NaN3 to prevent the alteration and internalization of surface antigens, which can induce a loss of fluorescence intensity. 100 μL of this cell suspension was added to each well in a 96-well U-bottom plate, and incubated for 30 min with the addition of 0.02 mg/mL or 0.1 mg/mL of a tested VHH (final concentrations) at room temperature or PBS for positive control. Cells were centrifuged at 1000g for 5 min at 4 °C, the supernatant was removed and 200 μL ice-cold PBS added. This wash was repeated three times. Cells were then incubated for 30 min, covered to keep plates in the dark, at room temperature with 1 μg/mL of anti-C-Myc tag Alexa Fluor™ 488 conjugated antibodies (Abcam), or 0.1 mg/mL of Alexa Fluor™ 488 conjugated α-Btx (Abcam) for the positive control (final concentrations). Cells were centrifuged at 1000g for 5 min at 4 °C, the supernatant was removed and 200 μL ice-cold PBS added. This wash was repeated three times, with the final resuspension in ice-cold PBS, 1% NaN3 with 3% BSA. Flow cytometry analyses were performed on a cytoflex S (Beckman Coulter) with the Cytexpert software version 2.2. FITC was read with the laser wavelength of 488λ, using the filter 525/40, whereas PE with a laser 581λ and the filter 586/42.

Transduced CHO-K1 cells expressing hα7-nAChR and a chaperone protein were cultured on 50 µg/mL poly-d-lysine (Sigma-Aldrich) and 330 µg/mL Collagen type 1 (Sigma-Aldrich) coated glass coverslips. 48 h later, the cells were fixed with 2% paraformaldehyde (PFA) for 15 min followed by blocking of non-specific binding, with 3% BSA in PBS for 1 h. The nanobodies were diluted to 5 µg/mL with PBS-BSA and incubated with the coverslips for 2 h at room temperature. HEK293 cells were cultured on poly-d-lysine (Sigma-Aldrich) coated glass coverslips, according to manufacturer’s recommendations. These cells were transfected using 10 μg DNA and the JetPrime transfection reagent (Polyplus), again according to manufacturer instructions. 36–48 h after transfection, cells were fixed with 4% PFA and for permeabilized cells incubated for 2 min with a solution of ethanol + methanol (1:1). Non-specific binding was blocked with 10% BSA in PBS for 5 min at room temperature. The nanobodies were diluted to 5 µg/mL also with 10% BSA in PBS and incubated with the coverslips for 2 h at room temperature. The hα7-IRES-eGFP and NACHO plasmids were transfected together (2:1 ratio), the hα3-IRES-eGFP and hβ4StrepTagII-IRES-mTurquoise were transfected together (1:1 ratio), and a plasmid containing the hβ2-nAChR subunit was transfected together with the hα4GFP construct (1:1 ratio). Proper expression of the respective nAChRs was verified by an anti-StrepTagII antibody for the hα3β4-StrepTagII-nAChR, by the fused GFP for the hα4GFPβ2-nAChR, and with an Alexa Fluor™ 647 labeled α-Btx for the hα7-nAChR (Supp Fig. 1). Anti-StrepTagII antibody and α-bungarotoxin-Alexa Fluor™ 647 (ThermoFisher) were diluted in PBS-BSA. Coverslips were mounted on slides after Prolong-DAPI staining (Invitrogen) and visualized using epi-fluorescence at constant exposure times. Anti-human IgG and anti-mouse IgG coupled to Alexa Fluor™ 647 (ThermoFisher) were diluted in PBS-BSA. All experiments were reproduced ≥ 4 times.

HEK-293 cells were seeded, 48 h before transfection, at a density of 5 × 105 per 100 mm dish in DMEM-FBS supplemented with penicillin/streptomycin (10 U/mL and 10 μg/mL resp.). When cells were approximately 70–80% confluent, they were transfected with 10 µg of the hα7-nAChR/m5-HT3A chimeric construct using the JetPrime reagent (Polypus) according to the manufacturer’s protocol, and incubated for another 48 h. Cells were washed and detached using a cell dissociation solution non-enzymatic (non-trypsin) (Sigma-Aldrich). Cells were resuspended to individual cells in 2 mL of binding buffer (10 mM HEPES, 2.5 mM CaCl2, 2.5 mM MgCl2, 82.5 mM NaCl, pH 7.2) in the presence of cocktail protease inhibitor (one tablet of cOmplete per 50 mL [Sigma-Aldrich]). Three replicates of 150 µL from this resuspension were pipetted to glass vials for each sample. 25 µL of each tested VHH (0.1 mg/mL) was added with 25 µL binding buffer in the control and ACh samples. After an hour incubation at 4 °C under agitation, 25 µL of binding buffer was added to all samples and 25 µL of 1 mM ACh was added to the ACh sample which were all incubated under agitation for 1 h at 4 °C. Finally, 50 µL of 25 nM I125-Tyr54-α-Btx was added, the samples were well mixed and incubated for 2 h at 4 °C. This resulted in final concentrations of 633.8 nM E3 VHH, 632.6 nM C4 VHH, or 100 µM ACh, and 5 nM I125-α-Btx. Glass microfiber papers, blocked using 5% skim milk for at least 30 min, were then used to vacuum-filter the samples and counts per minute measured using a Berthold LB2111 machine.

Xenopus laevis oocytes (EcoCyte Bioscience, Germany and Centre de Resources Biologiques, Rennes, France) kept in Barth solution buffer (87.34 mM NaCl, 1 mM KCl, 0.66 mM NaNO3, 0.75 mM CaCl2, 0.82 mM MgSO4, 2.4 mM NaHCO3, 10 mM HEPES pH 7.6) were nucleus injected with ~ 5–8 ng of hα7-IRES-NACHO and ~ 1 ng eGFP plasmids and stored at 16–18 °C for 48–96 h. Current recordings were performed using: Axon Digidata 1550A digitizer (Molecular Devices), Axon Instruments GeneClamp 500 amplifier (Molecular Devices), a self-built automated voltage controlled perfusion system, which controls an 8-port and a 12-port electric rotary valve (Bio-Chem Fluidics) both connected to a 2-way 4-port electric rotary valve (Bio-Chem Fluidics) which was flush with the recording chamber entrance allowing for rapid solution application and clean solution exchange, and finally pClamp 10.6 software (Molecular Devices). Electrode pipettes were pulled using a Narishige PC-10 puller. GFP positive oocytes were voltage-clamped at − 60 mV, unless otherwise noted, and perfused by Ringer’s solution buffer (100 mM NaCl, 2.5 mM KCl, 10 mM HEPES, 2 mM CaCl2, 1 mM MgCl2, pH 7.3), with sampling at 5 kHz, unless otherwise noted. ACh and size-exclusion purified VHH’s were diluted in Ringer’s buffer as specified. ClampFit 10.6 (Molecular Devices) was used for trace analysis and GraphPad Prism 4 (GraphPad Software) for data plotting and statistical analysis. Data are shown as mean ± standard deviation, where each n represents a different oocyte. The mechanical turning of the valves in the perfusion system produces a noise seen during the recordings, which was not filtered out, allowing for easy recognition of solution exchange times. The main valve allows for one solution to flow to the recording chamber and at the same time the other connected valve, if open, flows to waste. The main two-way/four-port valve exchange time was about 200 ms and there is around a 500 ms delay between the end of the exchange and arrival of the solution to the oocyte. Solution to be perfused to the chamber was started at least 4 s before in the direction of waste to ensure proper rinsing of valve tubing (unless noted otherwise).

The flow of the denoted concentration of VHH was applied 6 s after the start of the sweep to the recording chamber, allowing for a proper analysis of the leak/background current. 10–120 s later the main valve was switched to flow a solution that contained the same concentration of VHH with 30 µM ACh (or the denoted concentration in the case of ACh concentration–response curve). The valve flowing the VHH alone solution (now to waste) was switched to Ringer’s solution shortly after. Five seconds later, the main valve was changed back to flow the Ringer’s solution to the chamber and the other side valve was closed with the sweep finishing recording 8 s later. There was a three-minute start to start interval between all sweeps which continued washing with Ringer’s solution.

Once it was determined that the VHH’s had a slow on and offset time in order to conserve product and simplify solutions, the pre-perfusion protocol was changed to have only a 30 µM Ach solution applied for the 5-s activation after pre-perfusion of VHH in Ringer’s solution, rather than the mixture of ACh and VHH described above.

Oocytes were voltage clamped at − 70 mV (for 1.5 µM C4) and − 80 mV (for 150 nM C4) and sampled at 2 kHz. The flow was switched, without pre-rinsing, to apply a mixture of VHHs at the indicated concentrations directly at the beginning of the sweep for 30 s, directly, without pre-rinsing, switching to a solution with 30 µM ACh alone applied for 5 s and finishing the sweep with an 8.5 s wash (for 1.5 µM C4) and a 60 s wash (for 150 nM C4). The next sweep began directly after the termination of the current sweep.

Oocytes were voltage clamped at − 80 mV and sampled at 2 kHz. Valve switching in all cases was done without pre-rinsing times. For the first sweep, 60 s of wash buffer was perfused before switching to a solution with 30 µM ACh alone for 5 s, the subsequent sweep had 30 s of wash buffer then switching to apply VHH E3 at 150 nM for 30 s, before the 30 µM ACh alone application, and finally, the last sweep had E3 at 150 nM directly at the beginning of the sweep, then switched to a solution mixture containing E3 at 150 nM along with indicated concentrations of C4 for another 30 s, followed by 30 µM ACh alone. All sweeps finished with a 56 s wash, and the next sweep began directly after the termination of the current sweep.

The flow of denoted concentrations of VHH mixed with 30 µM ACh was applied 10 s after the start of the sweep for a duration of 5 s, followed by 15 s of recorded wash, with a 3-min start to start sweep interval.

In order to properly switch solutions just after the on-set of desensitization, there was not enough time to rinse solutions and therefore the main valve could not be used for switching. As a result, the solution was switched between 30 µM Ach to 30 µM ACh with the denoted concentration of VHH in the secondary valve where the delay of solution arrival is around 1.2 s. Therefore, the main valve was switched to flow 30 µM ACh 10 s after the start of the sweep, with the secondary valve switching to a solution of 30 µM ACh with VHH 0.5 s later. This achieved the arrival of the VHH around 2 s (including valve exchange time) after application of ACh alone. The combination was perfused for 6 s before switching back to ACh alone, and the main valve was switched back to Ringer’s after 3 s effectively creating a 10 s application of 30 µM ACh which included a combination of ACh with VHH for 6 s directly in the middle. There was a 5 min 20 s start to start sweep interval which washed the oocyte.

Below is the link to the electronic supplementary material.Supplementary file1 (DOCX 170 KB)